OF RET, GDNF AND GDNFR-a INAcknowledgements This thesis is dkdicated to the memory of my mother and...
Transcript of OF RET, GDNF AND GDNFR-a INAcknowledgements This thesis is dkdicated to the memory of my mother and...
EXPRESSION OF RET, GDNF AND GDNFR-a IN HUMAN
DEVELOPMENT AND DISEASE
STACEY M. IVANCHUK
A thesis submitted to the Department of Pathology in conforming with the requirements for
the degree of Master of Science
Queen's University
Kings ton, Ontario, Canada
April 1997
copyright 8 Stacey M. Ivanchuk, 1997
National Library Bibliothhue nationale du Canada
The author has granted a non- exclusive licence allowing the National Library of Canada to reproduce, loan, distri'bute or sell copies of hismer thesis by any means and in any form or formaf making this thesis available to interested persom-
The author retains ownership of the copyright in bidher thesis. Neither the thesis nor substantial adacts &om it may be printed or otherwise reproduced with the author's permission.
L'auteur a accorde me licence non
forme cpe ce soit pour mettre des exemplaires de cette th&e a la disposition des persomes ht&e&es.
L'auteurcoaserve IapropriM & b i t d'auteur qyi proege sa t h h . Ni la t h b ni des extmb substantiels & ceile-ci ne doivent &re imprimes ou autrement reproduits sans son
Abstract
The RET protooncogene encodes a receptor tyrosine kinase required for kidney
development. RET is predicted to fuaction in the reciprocal inductive interactions that give
rise to the mature kidney. To investigate the role for RET in human kidney development,
we used RT-PCR analyses to examine RET expression in a panel of fetal kidney RNAs
ranging in gestational age h m 7-5-24 weeks and in adult kidney. We detected expression
of RET and its multiple 5' and 3' coding variants in each RNA sample. RET expression
was developmentally regulated with expression levels 6- to 7-fold higher in the early
gestational ages dative to adult A similar pattern was observed for two alternative RET
transcripts generated by exon skipping at the 5' end of the gene. The expression of a third
&anscrip& RER16, which lacks exons 3-5, was distinct with relatively higher expression
in early gestational ages and a more rapid decrease in expression. RETU6 expression was
highest through a period of rapid bifurcation of the ureteric bud raising the possibility that
RM16 has a role in this process. We detected expression of three alternatively spliced
RET 3' variants ( R E D , REnl and RET43) throughout human kidney development.
RE19 was the most abundant variant in all samples. In contrast, RETSI expression was
almost undetectable early in development but significantly upregulated by 9 weeks
gestation. RETSl expression levels were approximately 35% those of RE19 in later
gestational ages. These results suggest a role for RETSL distinct from that for RET9 during
human kidney development*
The ligand for RET was recently identified as a complex consisting of GDNF and
GDNFR-a. We detected expression of both GDNF and GDNFR-a throughout our panel
of fetal kidney RNA. Developmental regulation of GDNFR-a expression was identified.
The expression pattem was distinct from that identified for RM during human kidney
development and may be indicative of a role for GDNFR-a in regulating RET activity.
In our investigation of RET, GDNF and GDNFR-a expression in the renal
tumours, Wilms' tumour and renal cell carcinoma, no consistent pattem of expression of
the three transcripts was discerned although RET was consistently detected in both tumour
tY pes-
Acknowledgements
This thesis is dkdicated to the memory of my mother and guardian angel, Bernice
(Bunny) Lvanchuk, who taught me the importance of dedication and determination. Her
spirit has found a home in me and she guides me through all the ups and downs that We
brings. I thank my father, Morris, and brother, Bryce, for supporting me in so mauy ways
throughout the course of this degree. Their constant love and encouragement has been my
rock.
I want to thaok Dr. Lois Mulligan for giving me the opportunity to pursue a
graduate degree in her lab. There have been many times when I have wondered what she
saw in me. She bas been a remarkable teacher and mentor but above al l else, a friend- I
don't know what I would have done without her constant encouragement and faith in me.
She has helped cultivate my love of science and research. It has been both a privilege and a
pleasure to work for her.
The people I worked with every day made a l l the hard times so much more
bearable. Shirley Myers has been a wonderful resource and a "running" motivator! Dr.
Harriet Feilotter is, and will always be, my favorite post-doc. I thank her for all her help
and the "Ieaf of hope" which I have kept with me through the course of writing up. I would
also like to thank Lee Fraser, a fellow graduate in the lab, in whom I found someone who
shares my taste in music and Love for sports. Thanks, too, to Nicolina Zakova, a late
addition to our lab.
I would like to thank my committee members, Drs. David Li;Licrap and Peter Greer,
for their constant support, helpful advice and wful discussions. Thanks also to Dr. Jim
Gerlach and Ms. Leah Young for all the help with PCR techniques. To Carla Cuthbert, my
favorite graduate student, I am forever indebted for she has made me feel that I am capable
of pursuing a career in science.
v
Final thanks go to Drs. Robert Hofstra and Marc Billaud for sharing their data prior
to publication and to the Queen's University Department of Pathology for their financial
support over the past three years.
Table of Contents
Abstract
Acknowledgements
Table of Contents List of Figures List of Tables List of Abbreviations
Chapter 1: Introduction
1.1 The REI proto-oncogene 1.2 RET Expression 1.3 The RET Ligand Complex
1.3.1 Glial Cell Line-Derived Neurotrophic Factor (GDNF) 1.3.2 GDNF Receptor-a (GDNER-a)
1.4 The RET Knockout Mouse 1.5 Kidney Development 1.6 Molecules Involved in Kidney Development 1.7 Alternative Splicing 1.8 RET in Disease
1.8.1 RET Expression in Tumours and Tumour Ceil Lines 1.8.2 R l Z Rearrangements in Papillary Thwoid Carcinoma 1.8.3 RET in Inherited Syndromes 1.8 -4 RET Mutations in Sporadic Tumours
Research Objectives
Chapter 2: Materials and Methods
Oligonucleotides RNA . Tissues and Patient Samples
Hirschsprung Patient Samples Fetal Kidney RNA and Renal Tissue Samples
Total RNA Extraction Reverse Transcription-Polymerase Chain Reaction (RT-PCR)
First S m d cDNA Synthesis PCR Using cDNA Templates Semi-Quantitative RT-PCR
Southern Blotting and Hybridization Southern Blotting Oligonucleotide Labeling Hybridization
Sequencing DNA Template Preparation Sequencing Reactions
Chapter 3: Expression of RET and its Multiple Splice Forms in Human Developing Kidney
Introduction
Resuits REl Expression in Human Kidney Development Quantitation of RET Expression During Human Kidney Development RET Alternative Splice Variants Quantitation of RTr Alternative Splice Vadaats
Discussion Materials and Methods
Growth of 'IT Cells M A Extraction Fetal Kidney, Adult Kidney and TT RNA Analyses Semi-Quantitative Reverse Transcription-Polymerase Chain Reaction Southern Blotting
Chapter 4: Expression of RET 3' Splicing Variants During Human Kidney Development
Introduction Results
Expression of RET 3' Alternatively Spliced Transcripts Quantitation of RET 3' Alternatively Spliced Variants
Discussion Materials and Methods
Fetal Kidaey, Adult Kidney and 'IT RNA Analyses Semi-Quantitative Reverse Transcription-Polymerase Chain Reaction
Chapter 5: Expression of Genes Encoding the RET Ligand Complex Components GDNF and GDNFR-a During Human Kidney Development
Introduction Results
Expression of GDNF in Human Fetal Kidney Expression of GDNFR-a During Human Kidney Development Quantitation of GDNFR-a in Human Fetal Kidney
Discussion Materials and Methods
Reverse Transcription-Polymerase Chain Reaction Analyses Semi-Quantitative Reverse Tcanscription-Polymerase Chain Reaction
Chapter 6: AnaIyses of RET, GDNF and GDNFR-u Expression in Human Disease
Introduction Results
Expression of RET, GDNF and GDNFR-a in Wilms' Tumour Expression of RET, GDNF and GDNFRa in Rend Cell Carcinoma GDNF Mutation Analysis in Hirschsprung Patients
Discussion RET/GDNF/GDNFR-a in Wilms' Turnours RET/GDNF/GDNFR-a Expression in Renal Cell Carcinoma
GDNF Mutation Analysis in Hirschspmng Disease Materials and Methods
Reverse Transcription-Polymerase Chain Reaction Conditions Genomic Sequencing
Chapter 7: Discwion
RET in Human Kidney Development RET 5' AIternatively Spliced Variants in Development GDNF and GDWR-a in Human Kidney Development RET 3'Altematively Spliced Variants in Development RET, GDNF and GDNFR-a in Human Disease
Summary
References
Appendix
Curriculum Vita
List of Fi y r e s
Figure
Schematic of the RET Receptor Tyrosine Kinase
Schematic of the RET 3' Alternative Coding Variants
Schematic of the REl Exon Structure and its Relationship with the RET 5' Alternatively Spliced Variants
The E2ETIGDNFiGDNFR-a Signaling Complex
Kidney Induction Cascade
Determination of Conditions for Semi-Quantitative RT-PCR Analysis of O v e d RlTExpression in Human Fetal and Adult Kidney
Expression of RET mRNA Forms Generated by Alternative Splicing at the 5' End of the Gene in Humao Fetal and Adult Kidney
Developmental Expression of RET5' Splice Variants in Human Fetal Kidney
RET 3' Isoforrn Interactions with Downstream Effector Molecules
Schematic of RET 3' Exons and the Locations of Primers Used in RT-PCR Analysis
Expression of REI 3' Coding Variants in Human Fetai and Adult Kidney
Determination of Conditions for Semi-Quantitative RT-PCR Analysis of RET 3' Coding Variant Expression
Developmental Expression of RET 3' Codiag Variants in Human Fetal Kidney
Expression of GDNF and GDNFR-a in Human Fetal and Adult Kidney
Determination of Conditions for Semi-Quantitative RT-PCR Analysis of GDNFR-a Expression
Developmental Expression of GDNFR-a in Human Fetal Kidney
Page
6.1 RET, GDNF and GDNFR-a Expression in W i ' Tuxnoun
6.2 RET, GDNF and GDNFR-a Expression in Renal Cell Carcinoma
6.3 GDNF Mutation in a Hirschpmg (HSCR) Patient
List of Tables
Table
Relative Expression Levels of RET in the Human Fetal Kidney
RET 5' Splice Vadant Expression Relative to Full Length RET Expression in Human Fetal Kidney
REN6 Expression Relative to FL RETExpression in Human Fetal Kidney
RETSl Expression Relative to RE19 Expression in Human Fetal Kidney
Expression of GDNFR-a in Developing Human Fetal Kidney
Histology and REZ: GDNF and GDNFR-a Expression in W h ' Tumours
RET, GDNF and GDNFR-a Expression in Renal Cell Carcinoma
Page
35
Abbreviations
bek BMP b~ BWS
C cDNA CJD CNS C-tenninus "c DEPC DNA dNTP dpc dT m EDTA EGFR ENS
FFI FGF FGFR FISH M C
G GDNF GDNFR-a GPI GUSB
HC1 HSCR
KC1 KGF KGFR
Id LMP LOH
adenosine triphosphate avian m ~ e l ~ b I a s t ~ ~ i s virus reverse trans&iptase adenosine triphosphate
basic mrobiast growth factor receptor bone morphogenic protein base pair Beckwith-Wiedemann syndrome
cytosine complementary deoxyn'bonucleic acid Creutzfeldt-lakob disease central nervous system carboxy terminus degrees Celsius
diethyl pyrocarbonate deoxyribonuclek acid deoxynucleoside triphosp hate days post-coitum deoxythymine dithiothreitol
ethylenediamhetetraacetic acid epidermal growth factor receptor enteric nervous system
fatal familial insomnia fibroblast growth factor fibroblast growth factor receptor fluorescence in sim hybridization familial medullary thyroid carcinoma
guanosine trip hosphate glial cell linederived neumtrophic factor glial cell linederived neurotmphic factor receptor-alpha glycosylp hosphatidylinositol beta-glucuronidase
hydrogen chloride Hinchsprung disease
immunoglobulin
potassium chloride keratinocyfe growth factor keratinocyte growth faftor receptor
limb deformity Low melting point loss of heterozygosity
M MAPK MEN MM Mrn2 min mRNA MTC
N NaOH NF N G F R P ~ ~ NK at N-terminus
P PCR PNK PNS m PTC PY
RA RAR-a RB RCC RET RNA RNase R7K RT-PCR
SCG sd SDS SH SLF SSC
T TBE TGF-P TK TPE
molar mitogen activated protein base multiple endocrine neoplasia metanephric mesenchyme r n ~ a i u m chloride minute mssenger ribonucleic acid medullary thyroid carcinoma
normal sodium hydroxide neurofibromatosis low-affinity nerve growth factor receptor normal kidney nucleotide - amino-terminus
phosphate polymerase chain reaction polynucleotide kinase peripheral nervous system phosphostyrosine binding papillary thyroid carcinoma phosphotyrosine
retboic acid retinoic acid receptor-alpha retinoblastoma renal cell carcinoma rearranged in transfection ninucieic acid ribonucIease receptor tyrosine kiaase reverse transcription-polymerase chain reaction
superior cervical ganglia standard deviation sodium dodecyl sulphate Src-homology steel factor saline sodium citrate
thymine Tris-borate EDTA transforming growth factor-beta tumour kidney Tris-phosphate EDTA
untranslated region volts von Hippel-Lindau weeks
Chapter 1
Introduction
1 .I The RET Proto-oncogene
RET (REarranged in Transfedon) was first isoiated as a dominant transforming
gene by transfection of turnour DNA into fibrobIasts 2. The gene was found to be
activated by recombination between two unlinked segments of DNA. The 5' portions were
different, however, the 3' segments of the isolated transforming genes were identical and
corresponded to the tyrosine kinase domain of a novel gene, RET 3. The gene consists of
2 1 exow that span 58 kb of DNA 4-7. Fluorescence in sim hybridization (FISH) analyses
were used to assign RET to chromosome 10q11.2
RETencodes a receptor tyrosine kinase (RTK) (Figure 1.1) 3. The yosine kinase
domain of RET is split by an insertion sequence of 27 amino acids. In addition to the
b a s e domain and short transmembrane domain cbaractedsac of RTK family members,
RET consists of a large extracellular domain comprising a signal peptide, a region of
cadherin homology and a cysteine residue-rich domain 9- lo. The cysteine-rich domain
contains 16 cysteine residues in a stretch of 120 amino acids. The translation start site and
amino 0-terminal signal sequence both lie within RET exon 1 5. Twelve possible N-
linked glycosylation sites are predicted in the exmcellular domain of the protein 97 10.
Five RET transcripts of 7.0,6.0,4.6,4.5 and 3.9 kb are detected by northern blot
analysis 11- 12. The differences in size are due to alterations in the 3' end of the gene 6. 12.
Splicing of RE;T 3' exons generates transcripts which encode several different carboxy (0-
termini. AU transcripts share. the first 19 exons after which sequences diverge. Splicing
may not occur at the end of exon 19 in which case the coding sequence continues into
intron 19 sequence coding for a further nine codons (Figure 1.2) 12. These transcripts
encode proteins designated RET9. Alternatively, exon 19 may be spliced to exon 20 or
exon 2 1 generating RET aanscripts with a novel 5 1 (RETS 1) or 43 (RET43) amino acid C-
terminus respectively (Figure 1.2) 12. W T 5 1 manscripts generate a 1 1 14 amino acid
Figure 1.1 Schematic of the RET receptor tyrosine kinase. The characteristic domains
contained within the extra- and intracellular domains of the protein are indicated
Signal Peptide
Cad he tin Homology
Region
Cysteine Rich Region
Transmembrane Domain
Kinase lnterkinase
Domain
Extracellular Domain
lntracellular Domain
Figure 1.2 Schematic of the RET 3' alternative coding variants. All transcripts share the
k t 19 exons of RET . The coding sequence for each isoform is the same up to and
including sequence for tyrosine residue 1062 (Y1062) after which the sequences diverge.
Splicing may not occur at the 3' and of exon 19 in which case the sequence reads into
intron 19 (RE19). Alternatively, RETexon L9 may be spliced to exon 20 (RETS1) or exon
21 (RET43). Coding regions are given as boxes and non-coding regions are given as solid
Lines. Dashed lines are used to indicate splicing. Polyadenylation sites are indicated by
(AM-
RET protein while RE79 transcripts generate a 1072 amino acid isoform 12. RET43 is
predicted to encode a protein of 1106 amino acids.
Alternative splicing also occurs at the 5' end of RET. Multiple transcripts are
possible as a result of exon skipping (Figure 1.3) 13. Exon 2 may be spliced to exon 3
resulting in transcripts that encode the complete extracellular domain. When exon 2 is
spliced to either exon 4 or 6, the resulting transcripts encode proteins that lack portions of
the region of cadherin homology 13. When exon 2 is spliced to exon 5. transcripts
encoding truncated products result due to a frameshift and consequent premature stop in
exon 5 13. In vino translation of proteins from the cDNAs corresponding to the RET 5 '
alternative splice variants has been described, however. it is not yet clear whether these
isoforms are functional in vivo,
1.2 RET Expression
In rodents. northern blot, in situ hybridization and immunohistochemistry analyses
have been used to determine the dismbution of RETexpression. During development, RET
transcripts have been found predominantly in subsets of cells of the centraI nervous (CNS)
and peripheral nervous systems (PNS) and of the excretory system l l v 14-16- Within the
CNS* RET expression has been localized to the motor neuron Lineages of the spinal cord
and hindbrain 14. Expression has also been detected in subsets of neuroretinal cells. Within
the PNS, RET expression has been localized to the sensory ganglia of the head and neck.
the dorsal root ganglia and its prrcursors. the cranial ganglia and the vagal neural crest and
myenteric ganglia of the gut I4l6. Expression in the embryonic kidney has been detected in
the early pro- and mesooephric structures as well as in the metanephros which matures into
the functional kidney lCL6. REZexpression in the developing kidney has been found to be
strongest early in development and to subsequently decmase with increasing gestational age
14, 15.
Figure 1.3 Schematic diagram of the RET pmto-oncogene and its protein products. A] The
relationship of RET coding exons and the corresponding protein domains. B] Predicted
products of alternatively spliced RET transcripts with exon skipping of 5' exom.
FL=M length
2/4=lPET exon 2 spliced to exon 4
US=RETexon 2 spliced to exon 5
2/6=-RETexon 2 spliced to exon 6
Additional norneural structures that express RET during embryogenesis include
salivary glands, spleen and lymph nodes 11- 16. RET expression has also been detected
in the embryonic liver. however, the period of expression is brief (125-14.5 days post-
coitum (dpc)) 149 1s.
In the adult, RETexpression has been found in subsets of PNS and C N S neurons
16, 17. Tmmunohistochemistry has been used to detect RFT expression in the sympathetic
ganglia and neuroepitheLium-derived astrocytes and cortical neurons 17. Northern blot and
in situ hybridization analyses have been used to detect low levels of RET expression in
adult lung, heart. spleen, lymph nodes, thymus and small intestine while stronger
expression has been detected in adult brain and salivary glads 14* 16. These analyses have
failed to detect RET expression in the adult Liver, kidney or thyroid 1 1 - 14. However, the
more sensitive reverse transcription-polymerase chain reaction (RT-PCR) has been used to
detect RET expression in the latter two tissues 13- Is.
1.3 The RET Ligand Complex
1.3.1 Gliai Cell Line Derived Neurotrophic Factor (GDNF)
The ligand for RET has recently been identified as a multicomponent complex.
Members of this complex include glial cell line-derived neurotrophic factor (GDNF) and
GDNF receptor-a (GDNFR-a) (F~gure 1.4) 19-22. Lin et al. 23* t4 identified GDNF as a
neurotrophic factor with the ability to sustain dopaminergic neurons. GDNF is synthesized
as a preproprotein containing an N-terminal signal sequence required for secretion. The
mature human 134 amino acid protein is a glycosylated disulfide-linked homodimer.
GDNF has seven conserved cysteine residues in the same relative spacing found in
memka of the TGF-P family 23. Mature GDNF shares less than 20% homology with any
family member 24.
The human GDNF gene has been mapped to chromosome 5p 12-p 13.1 and
consists of two exons 23. The use of an alternative splice site within the first exon results
Figure 1.4 The RETfGDNFfGDNFR-a signaling complex. GDNFR-a, a GPI-linked cell
surface protein, is required to mediate GDNF homodimer binding to RET. Whether the
GDNF dimer binds one or two molecdes of GDNFR-a is not known, thus, both
possibilities axe illustrated. GDNF in complex with GDNFR-a is capable of activating
RET, resulting in receptor autophosphorylation (indicated by P enclosed in a circle).
GDNF Ihnnnf imcr
in the deletion of 78 nucleotides affecdng sequence encoding the potential secretion signal
and the consensus sequence for proteolytic processing which are both absent in the rnature
GDNF protein 23. Thus, both the full length and alternatively spliced mRNAs encode the
same mature protein and the signiticance of these isoforms is unclear *6* 2'.
GDNF is widely expressed in many non-neural as well as neural tissues 26+ 2'. In
the developing murine embryo, GDNF is first detected in the neuroectoderm. Low levels of
GDNF expression have been detected throughout the C N S from early embryonic ages to
adulthood. Highest levels of GDNF expression during development have been detected in
skin. whisker pad, kidney, stomach and testis 28. Expression levels in the gut and kidney
decrease after birth similar to RET expression 28- 29. In comparison, notable increases in
GDNF expression Levels have been observed in adult liver, lung, testis and ovary 2'- 28.
Recently, a GDNF-related molecule has been identified. Human neurmrin has 42%
amino acid homology with human GDNF 30. 31. Both GDNF and neurmrin can stimulate
the MAP kinase signaling pathway in cultured sympathetic neurons and support the
survival of sympathetic as well as sensory neurons in vim0 3 While GDNF has been
shown to interact with RET and stimulate RET activation, neurturin's ability to bind to RET
has not yet been investigated
1.3.2 GDNF Receptor-a
GDNFR-a is the other identified member of the RET multicomponent receptor
complex. This glycosyLphosphatidylinosito1 (GPO-Linked protein is a membrane-bound
molecule required to mediate GDNF binding to RET (Figure 1.4) Z1- 22. Human GDNFR-
a encodes a 465 amino acid protein with highly hydrophobic amino 0- and cvboxy (C)-
termini characteristic of GPI-linked proteins (reviewed in 32). GDNFR-a contains 3
potential glycosylation sites and 30 cysteine residues 21. The spacing of the cysteine
residues is not related to that found in any extracellular cysteine-rich domain reported for
known receptors 21.
GDNFR-a has been mapped to l0q25-26. In the rat, GDNFR-a expression has
been detected in both neural and non-nets.rai t issws in a pattern similar to both RET and
GDNF. Expression has been detected in the dopaminergic, spinal motor and subsets of
dona1 root ganglia neurons, in developing nephrons and in embryonic smooth and striated
muscles of the enteric nervous system (gut, esophagus, stomach) 21- 22. Expression has
also been detected in the retina, thalamus, pons, medulla oblongata, pituitary and urogenital
trac to
GDNFR-a is required to mediate GDNF binding to RET. In the absence of
GDNFR-a, GDNF binding to RET and autophosphorylation of the receptor are minimal
21. 22. Treanor et ol. 22 have proposed that a GDNF hornodimer binds to GDNFR-a
forming a composite ligand that is capable of binding to and activating RET.
Recently, RElTL2 has been identified as a GDNFR-a family member 33. Human
RETL2 shares 49% amino acid homology with human GDNFR-a. Common features of
both RETL2 and GDNFR-a are a hydrophobic N-terminus indicative of a signal sequence
and a hydrophobic C-terminus indicative of a GPI-linkage motif 21- 22. 33. Both GDNFR-
a and RETL2 are expressed in embryonic brain, lung, kidney and intestine. However,
GDNFR-a is expressed at relatively higher levels in the kidney and intestine while RETL2
is expressed at relatively higher levels in the lung 33. Sanicola et a[. 33 have shown that, in
the absence of RET, GDNFR-a binds to GDNF with greater aftinty than does RETL2.
This suggests that RETL2 requires RET to facilitate binding to GDNF. Consistent with
this, RETL2 forms a high affinity complex with GDNF in the presence of RET.
1.4 The RET Knockout Mouse
While mice heterozygous for functional RET appear normal, RET knockout
(4) mice develop to term and die 16-24 hours after birth 34. Dissection of the RET -1- mice
revealed absent or rudimentary kidneys. Histological analysis of the mutant kicky
rudiments has shown severe dyspiasia characterized by reduced ureteric bud branchings
and absence of a mature collecting duct system as well as large areas of undifferentiated
mesenchyme 34. Some RET-f- mice contain blind-ending ureters with no renal tissue and
others display a complete absence of the ureter and kidney as either uni- or bilateral renal
agenesis. The histology of the kidney rudiments in the RET-/- animals is consistent with
failure of the ureteric bud to grow and bifurcate properly 35.
In addition to remi dysmorphology, the phenotype of the RET-I- mice is
characterized by absence of neurons of the myenteric plexus from the small and large
intestines, esophagus and stomach 34- 36. Enolase and peripherin, enteric neuron markers,
have not been detected in the myenteric and submucosal plexi of the small and large
intestines in the RET-I- mice 34. RET-I- mice also display complete absence of superior
cervical ganglia (SCG), the most anterior ganglia of the sympathetic chain, which are
believed to be derived from a pool of precursor cells that also gives rise to the enteric
nervous system (ENS) 34. 36. Anatomical abnormaiities have not been detected in other
parts of the developing nervous system that normally express RD' including cranial, dorsal
root and sympathetic ganglia as well as spinal cord motor neurons and brain 34.
1.5 Kidney Development
The mammalian kidney develops through a series of reciprocal inductive
interactions between two distinct cell types, the ureteric bud epithelium and the metanephric
mesenchyme (MMJ 35. Interactions between these two cell types result in the growth and
branching of the ureteric bud as well as in the condensation and epithelialization of the MM
(Figure 1.5) (reviewed in 35 and 37). As the kidney matures, the ureteric bud develops into
the collecting duct system while the MM gives rise to both the nephrons and the connective
tissues.
One of the first signs of kidney induction is the formation of the ureteric bud off the
Wolftian duct 35. The evagination of the ureteric bud is under the control of signals from
Figure 1.5 The kidney induction cascade. The two cell lineages that give rise to the kidney
are the ureteric bud epitheiium and the metanephric mesenchyme (MM). Arrows are used to
indicate progressive events in kidney development The ureteric bud gives rise to the
collecting duct system while cells derived from MM give rise to the nephrons and
connective tissue.
Requirement
Differentiation Lr' Growth and Bifurcation
Stromagenic
Condensation Mesenchyme-Epithelium
Transition
Nep hrons I Oifferentiaring I I ColIecting Duct System I
Induction
Adapted from Bard et al., 1994
Duct Bikat ion Ceases
the MM (Figure 1.5). In the young embryo, the MM is fmt visible as a discrete zone of
blastema 3-4 cells thick 35- 37. The blastema is induced to divide and enter a stem cell phase
by signals from the newly formed ureteric bud (reviewed in 38). The stem cells of the MM
give rise to progeny which are either stromagenic or nephrogenic (reviewed in 38 and 39).
Further induction signals derived from the ureteric bud stimulate the MM nephrogenic cells
to aggregate, epithelialize and form nephrons and the stromagenic cells to differentiate into
connective tissue. Signals derived h m the MM supplement ureteric bud growth and lead
to bud bihucation (Figure 1.5) (reviewed in 38). At the more advanced stages of kidney
organogenesis, these inductive interactions take place only in the nanow region around the
outer edge of the kidney referred to as the nephrogenic zone 35. Early in kidney
development, the metanephric blasted cells are separated from the Wolffian duct by a
greater physical distance than the MM stem cells are fkom the ureteric bud epithelia 35. This
suggests that the earlier inductive interactions represent long range signaling in comparison
to subsequent inductive interactions where the two cell types are in close proximity.
In humans, the nephrogenic cells fit begin to differentiate into the various cell
types of the mature nephron around 8 weeks gestation (reviewed in 35 and 37). From 8
until 14-15 weeks, nephrons attach to tubules within the zone of wteric bud anterior
growth. During this period, the rate of ureteric bud bifurcation is rapid (reviewed in 35 and
37). Undifferentiated MM covers the entire ureteric bud during the initial two divisions of
the bud (reviewed in 35 and 37). As more branches are formed and the bud elongates,
undifferentiated mesenchyme advances with the actively growing tips of the ureteric bud.
This constitutes the nephrogenic zone. Around 15 weeks gestation. the rate of ureteric bud
bifurcation slows through to 19-20 weeks (reviewed in 37). Branching of the bud rarely
occurs between 20 and 32 weeks gestation and anterior extension at this time is minimal.
1.6 Molecules involved in Kidney Development
In the mouse, formation of the kidney is initiated around 10.5-1 1.5 dpc when the
ureteric bud emerges near the caudal end of the nephric duct and grows dorsally (reviewed
in 38). As the ureteric bud invades the MM and begins to branch, RET expression is
observed throughout the bud 14- 15. With the progression of kidney development, RET
expression is restricted to the growing tips of the ureteric bud within the nephrogenic zone.
The requirement for RE' for the development of the ureteric bud has been confirmed in
organ culture experiments 40. Ureteric bud and MM tissues isolated fiom RET-/- and
normal control rnurine embryos can be co-cultured in vino. m e n RET-I- bud and MM
tissues are cocultuced, the ureteric bud fails to grow in the majority of cases and any
degree of branching is rare 40. Additionally, differentiation of the MM is not observed In
co-cultwes of normal ureteric bud tissue with RET-I- MM tissue, the mutant mesenchyme
is capable of inducing growth and branching of the ureteric bud *. However, when
REW- ureteric bud tissue is co-cultured with MM tissue from a normal embryo, branching
of the ureteric bud does not occur 40. These results suggest that the failure of ureteric bud
development to proceed in RET-I- embryos was due to the absence of functional RET in the
bud epithelium preventing response of the ureteric bud to mesenchyme-derived signals.
Maturation of the ureteric bud and metanephric mesenchyme are interdependent and
expression studies have implicated more than 50 molecules in the regulation of induction
andlor early or later differentiation in the mammalian kidney (reviewed in 38 and 39) Many
of the molecules identified as essential for proper kidney development are absent in the
adult organ indicating developmental regulation of expression (reviewed in 39). Assigning
specific roles to the molecules involved in mammalian kidney development has proven to
be difficult. Targeted disruption of more than 30 genes known to be expressed during
kidney development has produced a "helpful" phenotype. characterized by some degree of
renal dysmorphology. in only 6 knockout mice (reviewed in 38 and 39). Aside fiom gene
knockouts. however, the effects of deregulated gene expression or mutations that alter the
n o d function of the gene product have provided insight into the roles of other molecules
involved in kidney development.
Knockout mice that fail to show early signs of kidney development include the
WT- I-/-. RAR-ay-I-. and GDNF-/- mice suggesting roles for these molecules in
kidney induction. The WI-14- mouse is characterized by a lack of ureteric bud outgrowth
41. Targeted disruption of the RARa and y g e n s in mice results in a similar renal
abnormality 42. WT-1, RARa and RARy are expressed in the uninduced MM suggesting
that both play a role in kidney inductive events 4245. The phenotype of the RET-/- mouse,
described in section 1.4, includes a variable degree of failure of the ureteric bud to invade
the MM, grow and branch as well as large areas of undifferentiated mesenchyme 34. When
GDNF h c t i o n is abolished, the mice resemble the RET-I- mice in terms of renal
dysmorphology confirming that the RET signaling pathway is required for proper kidney
development 46-48. A role for the limb deformity (14 gene, mutations in which are
responsible for limb deformity in mice, in kidney induction is suggested by the phenotypes
of mice with recessive mutations in id. Mice homozygous for any of the id mutations have
rend dysplasia characterized by the absence or delay of ureteric bud outgrowth 4?
Molecules implicated in early kidney differentiation include bone morphogenic
protein (BMP)-7 and PAX-2. BMP-74- mice exhibit lethal kidney hypoplasia 50. These
mice develop normally until L2.5 dpc, however, fewer nephrons develop than in the wild
type mice and ureteric bud branching is stopped prematurely. Deregulation of PAX-2
expression, normally spatially and tempomlly restricted in the developing kidney. results in
failure to develop ureteric buds and mature nephric tubules Normally, PAX-2
expression is quickly downregulated in the developing kidney suggesting that properly
timed activation of PAX-2 expression is essential 51.
Molecules involved in subsequent differentiation of the maturing kidney include
WNT4 and WT-1 (reviewed in 39). WNT-4 transcripts are expressed in induced regions
of the developing kidney undergoing extensive differentiation during the mesenchyme-to-
epithelium transition and a role for the molecule in this process has been suggested 52.
Normally, WNT-4 is expressed in induced aggegates of mesenchymal cells and their
derivatives 52. The kidneys of WNT-41- mice display mesenchymal condensations but few
of these condensations epitheliahe or express such markers for late differentiation as PAX-
8. Branching of the ureteric bud remains unaffected 52. The upregulation of WT-I
coincides with downregulation of PAX-2 in cells differentiating into glomerular structures
53. WT-1 expression peaks in glomerular epithelium, one of the latest stages of kidney
differentiation 43* 44. Ryan et ol. 54 have shown that WI-l is in fact a repressor of PAX-2
expression in the mesenchymal cells which coexpress the two.
I. 7 Alternative Splicing
Alternative splicing at both the 5' and 3' ends of RET can result in multiple
different transcripts which translate into distinct proteins. W e little is known about the
function of the RET 5' isoforms (discussed above in section 1-2). in vitro studies have
suggested functional differences between RET9 and RET51, two of the 3' isoforms.
Activated RETS I constructs tramfected into a phaeochromocytoma cell line (PC 12) induce
more prominent neurite outgrowth than activated RET9 constructs 55. Binding assays have
suggested differences in the abilities of the EUX 3' isoforms to interact with the Src-
homology 2 (SEI2) and phosphotyrosine binding (PTB) domains of adapter molecules Shc
and Grb2 56. 57. This raises the possibility that RET9 and RET51 have different
downstream signaling capabilities .
Alternative splicing events occur in many developmentally important genes in
addition to RET. Individual members of the Trk family of RTKs use differential splicing of
alternative exons to generate transcripts encoding tmcated receptors that lack the entire
catalytic domain (reviewed in 58). The in vivo functional sigruficance of these truncated
Trk isoforms is unclear, however, roles in the active tramport of Ligaods or receptor
clearing have been suggested 59. TrkC, one of the Trk f d y members, additionally
encodes a family of full length receptors with catalytic domain insertions which coder
differential signaling properties to these receptors 60-62. This is similar to RE' where
alterations at the C - t e e of the RET isofonns affect interactions with downstream
effector molecules.
The fibroblast growth factor receptor (FGFR) f ' y consists of four
trammembrane receptor tyrosine kinases which have immunogIobulin (Ig) repeats in their
extracellular domains (reviewed in 63). Expression of the FGFRs is upregulated upon
cellular differentiation 64. The use of alternative splice sites within the sequence encoding
the extracellular domains of the FGFRs gives rise to muidpie protein isoforms with
differential ligand binding specificities 65-67. Two variants of FGFR-2 are generated from
differential use of exons encoding the third extracellular immunoglobulin domain. The
resulting receptors, keratinocyte growth factor receptor (KGFR) and bek (basic FGFR),
display different affinities for KGF/FGF-7 and basic FGFEGF-2 respectively 68. 69. Eariy
in development, the overall expression level of KGFR is consistently higher than that of
bek 70. Shi et al. 71 identified mutually exclusive expression patterns of the FGFR-2
variants which were tissue-specific suggesting different requirements for FGFR-2 variants
during development.
Due to exon skipping, similar to that seen in RET, the single id gene gives rise to
four major mRNAs (I-IV) that are expressed in two distinct patterns during development
72. Transcripts encoding isoforms EIII each encode a basic amino terminus but differ with
respect to coding exons. These isoforms are coordinately expressed during development in
the nervous system and kidney but not in the limb bud 72- 73. Isofom I transcripts contain
the full exon complement. Isoform I1 transcripts lack exons 2 and 3 while isoform III
-scripts lack exons 2 ,3 and 4 and, as a result of being translated out of frame, result in a
truncated product. Isoform IV differs £?om I-III in that it contains an acidic amino terminus
and is expressed in both the embryonic kidney and limb bud 73.
1-8 RET in Disease
1.8.1 RET Expression in Twnours und Turnour Cell lines
Turnours of neural crest origin have been shown to express RET at high levels.
Santoro er al. 74 found RET was consistently expressed in medullary thyroid carcinomas
and phaeochromocytow (see section 1.5). High levels of RET expression have
been reported in surgically resected neumblastomas and in human neuroblastoma cell lines
3 9 759 76- However, no mutations in RET have been identified in cases of neuroblastoma
examined 77.
RET expression has also been detected in promyelocytic and monocytic leukemia
cell lines 3 and papillary thyroid carcinomas 78-80- The latter are discussed in section 1.5.1.
1.8.2 RET Rearrangements in Papillary Thyroid Carcinoma
The RET protooncogene is found rearranged and constitutively active in a
proportion of papillary thyroid carcinomas (PTC) 78-82. The rearrangements occur in vivo
as tumour-specific events. The characterized recombination events result in the fusion of
the sequence encoding the RET tymsine kinase domain with the 5' sequences of different
genes. These 5' sequences contain elements responsible for RET expression in a cell type
where it is not normally expressed The chimeras encode molecules with Ligand-
independent dimerization ability. The first of these rearrangement events to be characterized
involved a paracentric inversion of the long arm of chromosome LO, inv( lO)(q 1 1.2q2 1) 83,
which resuited in the fusion of RET C-terminus encoding sequence with the H4 locus
(DIOS170) 81. Rearrangements involving the gene encoding the RIa regulatory subunit of
protein b a s e A 79 and ELI3 80- 82, a ubiquitously expressed gene localized on
chromosome 10, have since been described. Together, rearrangements in RET have been
recognized in up to 35% of papillary thyroid carcinoma cases 82.
1.8.3 RET in Inherited Syndromes
Germline mutations in RET are responsible for its conversion to a dominant
oncogene in the hereditary cancer syndrome multiple endocrine neoplasia (MEN 2)
subtypes 2A and 2B 8487. MEN 2A is- the most common MEN 2 subtype encompassing
greater than 90% of cases of MEN 2. Patients can present with medullary thyroid
carcinoma (MTC), phaeochromocytorna and/or hyperthyroidism (reviewed in 8 8).
However, penetrance is incomplete and 30% of patients have no symptoms of m C ,
phaeochromocytoma or hyperparathyroidism by the age of 70 (reviewed in 88). RET
mutations have been identified in 95% of MEN 2A families. Affected family members have
germhe rnissense mutations in sequence encoding one of five cysteine codons (codon
609,6 L 1,618 or 620 in exon 10; codon 634 in exon 11) 8" 89* These same RET
mutations have been identified in 85% of cases of familial medullary thyroid carcinoma
(FMTC) where MTC is the only clinical feature 86* 899 Two novel mutations associated
with FMTC have been identified. These mutations result in amino acid substitutions at
codons 768 (exon 13) and 804 (exon 14) and are predicted to modify the kinase activity of
RET 9 1-93
Clinical presentation of the MEN 2B subtype is similar to that for MEN 2A.
However, MTC and phaeochromocytoma develop much earlier in MEN 28 patients,
parathyroid involvement is rare and patients may present with developmental abnormalities
including ganglioneuromatosis, myelhated corneal nerves and marfanoid habitus (reviewed
in 88). Approximately 5% of all MEN 2 cases are the 2B subtype. A point mutation at RE'
codon 9 18 (exon 16) has been identified in 95% of MEN 2B patients 94-96.
HSCR occurs in 115000 Live births and can be sporadic or familial 97. Mutations in
the RET protosncogene have also been identified in 10-4045 of cases of Hirschsprung
disease (HSCR). a congenital abnormality characterized by the absence of sympathetic
neurons in the hindgut (reviewed in 88 and 98). The RET mutations associated with HSCR
are inactivating and result in loss or abrogation of RET function 99. Rarely, HSCR patients
have chromosome lOq11.2 deletions that result in complete loss of a single RET d e l e loo*
l . More common are mutations in RET which are found throughout the entire gene.
Frameshift and nonsense mutations are predicted to result in RET protein truncations 102-
107. Missense point mutations can also cause RET inactivation n- 99 (M. Billaud, personal
communication). No genotype-phenotype correlation has been identified to date. These data
suggest that haploinsufficiency for RET results in the disease phenotype.
I .8.4 RET Mutations in Sporadic Tumours
Somatic mutations of RET have been described in a proportion of sporadic MTCs
and phaeochromocytomas (reviewed in 88). The frequency of RET mutations in sporadic
MTC varies from 23 to 86% depending on sample size and population studied 94- 95- 108-
113- The majority of reported mutations affect RET codon 918, however, infkquent
mutations of codons 634.768 and 883 have also been described 95- 1099 1 13-1 16 (reviewed
in 88). In sporadic phaeochromocytomas. RET mutations have been identified in
approximately 10% of tumours 95- 1 17. 18. Reported mutations affect codons 620, 630,
634 as well as codon 9 18 9% 1 19.
RESEARCH OBJECTIVES
The objectives of this project were:
11 To identify RETexpression in developing human kidney ranging in gestational age from
7.5 through 24 weeks and to quantitate RETexpression in these samples.
21 To determine the expression patterns of both the 3' and 5' RET alternatively spliced
variants in human kidney development and quantitate relative expression levels of these
alternatively spliced variants.
31 To characterize the expression of GDNF and GDNFR-a, genes encoding members of
the multicomponent RET receptor complex, in developing human kidney.
41 To investigate a role for RET signaling complex molecules in disease by i] examining
expression of RET, GDNF and GDNFR-a in a panel of Wilms' turnours and renal cell
carcinomas and ii] by screening a panel of HSCR patients for GDNF mutations.
Materials and Methods
Oligonucleotides
The sequences of the primers used in PCR analyses are listed below. Primers were
synthesized either by Cortec (Kingston, Ontario) or by Genosys (The Woodlands, TX).
For reverse primers, the position of the most 3' base is given first.
The primers used for PCR amplification of the RET gene were 5- 84:
Forward primers used in RET 5' alternatively spliced variant expression analyses
consisted of the terminal 10 nucleotides of RET exon 2 and the first 10 nucleotides of the
exon to which exon 2 is spliced (any of exons 3.4'5 or 6) 5* 13* 84:
p25F exon ZS; 477 nt 5'-AGTGTCCGCAGACACCGTGG-3 ' ESA exon 5; 1203 nt 5'-GTACGGTCGCCCGCACGAAm-3'
Additional primers used in semiquantitative reverse transcription-polymerase chain
reaction (RT-PCR) anaiyses of RETexpression were designed using the program OIigo 18.
120,
The primers used for amplification of the RET 3' alternatively spliced transcripts
were according to Myers et al. 6. Nucleotide position start sites correspond to genomic
RET sequence:
The primers used in PCR analyses of GDNF expression were 121:
GDXlF exon 1; 3 nt 5'-GAATTATGGGATGTCGTG-3' GDN7R exon 2; 240 nt 5'-ATCTGGTGACCITITCAGTC-3 ' GDX3R exon 2; 45 1 nt 5'-CATCGCAAGAGCCGCTGCAG-3'
The primers used in PCR analyses of GDNFR-a expression were:
Primers specific for the P-glucuronidase gene (GUSB) used in semiquantitative
RT-PCR analyses were 18:
GUSB3 exon 2: 53 1 nt 5'-ACTATCGCCATCAACAACACACI'CACC-3' GUSBS exon 3; 725 nt 5'-GACGGTGATGTCATCGATGT-3'
RNA, Tissues and Samples
Hirscbsprung Patient Samples
DNA was extracted from the peripheral blood of a collection of HSCR patients by
Dr. Lois Mulligan as described in Mulligan et aL 122.
Fetal Kidney RNA and Renal Tissue Samples
Human fetal kidney samples ranging in gestational age from 8 through 24 weeks
were obtained from therapeutic abortions conducted at Children's Hospital in Montreal,
Quebec. Additional human fetal kidney sampies were obtained from the Central Laboratory
for Human Embryology at the University of Washington (Seattle, WA). All human fetal
kidney samples were collected under ethically approved protocols issued by the host
institution. Wilms' turnour samples were obtained from either the Divisions of Hematology
and Oncology, Children's Hospital Medical Center in Cincinnati, OH or the Children's
Hospital of Philadelphia, PA under ethically approved protocols 123. Three of six Wilms'
tuxnow samples used in analyses were obtained fkom mouse xenografts. The remaining
three samples were obtained from primary tumours. Renal tumour and corresponding
normal tissues were obtained following nephrectomies conducted at the Kingston General
Hospital with the help of Drs. Iain Young and Sandy Boag. Tissues were snap h z e n in
liquid nitrogen and stored at -800C. Human tumour analyses described in chapter 6 were
performed as a project which had separate and additional ethical approval.
Total RNA Extraction
RNA was extracted from human fetal kidney ranging in gestational age from 8
through 24 weeks by Dr. Lois Mulligan essentially by the method of Chomczynski and
Sacchi 1z4. Snap-frozen tissues were pulverized using a mortar and pestle. Ground tissue
or tissues too small to grind were transferred to a dounce homogenizer. One millilitre
TRIzol (Gibco-BRL, Gaithersburg, MD) was added per lOOmg tissue and the sample was
homogenized. Samples were transferred to sterile lOmL polypropylene tubes and incubated
at room temperature for a minimum of 5 minutes. 0.2 volumes chloroform was added to
the sample. Samples wen centrifuged in a Sowall RC-SB superspeed model (Dupont.
Wilmington, VA) at 10000 rpm for 15 minutes (40C) using Sorvall fixed angle rotor type
SS-34. The upper aqueous layer containing RNA was transferred to a new lOmL
polypropylene tube. 0.5 volumes isopropanol was added to precipitate the RNA. Samples
were centrifuged at 1OOOO rpm for 10 minutes (40C). The pellet was washed with 1
volume ethanol. Samples were then centrifuged at 8000 rpm for 5 minutes (4OC). The
ethanol was decanted and the pellets air dried for 5 to 7 minutes. Care was taken not to
allow the pellets to dry too long as this would make resuspension difficult, The pellets were
resuspended in 25pL diethyl pyrocarbonate @EPC)-treated water per 1mL TRIzoi. The
EWA concentration was determined by specaophotomeUy using an Ultraspec JII
spectrophotometer (Pharmacia, Baie d'Urf', Quebec). Absorbance readings at 2 6 h and
28Onm wavelengths were recorded RNA concentration was determined according to the
formula 125:
(absorbance at 260nrn)(40pg/mL,)(dilution factor)
where 40pg/mL is an estimate of the amount of RNA required to produce an absorbance
reading of 1. Integrity of RNA was c o w e d by elecnophoresis on ethidium bromide-
stained 1% agarose gels.
Reverse Traascription-Polymerase Chain Reaction
First strand cDNA synthesis
One pg of RNA was suspended in LOW DEPC-treated water, heat denatured at
700C for 5 minutes and cooled on ice briefly. F i t strand cDNA was generated fkom RNA
templates by incubating at 420C for 1 hour in 50mM Tris-HCl (pH8.3)- 8mM MgC12,
3OmM KCI, lOmM dithiothreitol (DTT). 2mM deoxynucleotide triphosphates (dNTPs)
(Pharmacia, Baie d'Urf6. Quebec), 7 units avian myeloblastosis virus reverse transcriptase
(AMV-RT) (Promega, Madison, WE) and 10 units human placental RNase inhibitor
(Pharmacia, Baie d'UrE, Quebec). 2jM random hexamer primers (Pharmacia, Baie
d'Urf6, Quebec) were used for RT-PCR analyses of RET and RET 5' alternatively spliced
variants expression. 2pM oligo dTls primer (Genosys, The Woodlands, TX) were used in
all other analyses. The enzyme was inactivated by incubating at 650C for 10 minutes then
freezing at -200C. Negative control reactions were performed identically but lacked RNA.
PCR Using cDNA Template
One tenth of a first s m d cDNA reaction was used in each PCR. Amplfication was
performed in solution containing lOmM Tris-HCl (pH8.3). 50mM KCl, 0.01% gelatin.
2OOpM d N T P s , 1 -5 units Taq DNA polymerase (Gibco-BRL, Gaithersburg. MD). 0.75-
1.75mM MgC12, 1p.M of both forward and reverse primers and deionized water to a
volume of to@. Samples were laye~d with light mineral oil and amplified in an
HybaidlOmnigene automated DNA t h e d cycler (Interscience. Markham, Ontario) using
1 min at 950C to denature, 1 rnin at 550C to anneal primers and 1 minute at 720C to extend
repeated for 40 cycles. Reactions were concluded with an extension period of 720C for LO
minutes. PCR products were eiectmphoresed on 2% agarose gels stained with ethidium
bromide and visualized under ultravioiet Light. LOO base pair molecular weight standard
(Pharmacia, Baie d'Urf6. Quebec) was used for band size estimation.
Semi-Quantitative RT-PCR
Experimental details for individual quantitative studies ace given in chapters 3-5.
Briefly, 0.1p.M [PPI-ATP labeled fonvard primer was included in PCRs to pennit liquid
scintillation of incorporated counts. cDNA templates were subjected to increasing numbers
of PCR cycles. PCR products were separated on 2% agarose gels and appropriate bands
were excised. Measurements of counts per minute (cpm) obtained fkom liquid scintillation
were plotted as a hction of cycle number to determine the range of cycles for which
amplification was hear.
Two-fold serial dilutions of cDNA template were subjected to cycles of PCR within
the linear range to determine amplification efficiencies. Where plots of cpm versus dilution
factor were linear, the conditions wen conside~d reliable for quantitation analyses.
Southern Blotting and Hybridization
Southern Blotting
PCR products from amplifcation of RET 5' alternatively spliced variants were
electrophoresed on 2% agarose gels in 1X TPE buffer at 120V for 2 hours. Gels were
denatured in 0.4N NaOH for 30 minutes. Gels were placed onto a sheet of 3MM filter
paper (Ahlstrom Filtration, Philadelphia, PA) wetted with 0.4N NaOH. The 3MM paper
was laid over a glass plate support such that the ends soaked in a reservoir of 0.4N NaOH.
A piece of Hybond N+ nylon membrane (Amersham, Arlington Heights, IL) cut to fit the
gel was wetted in 0.4N NaOH and placed directly on the gel. Care was taken to prevent air
pocket formation between the gel and the membrane. A single sheet of 3MM paper cut to fit
the gel was soaked in 0.4N NaOH and placed on the membrane. Multiple sheets of
adsorbent paper were cut to size and placed onto the 3MM paper. Capillary blotting
proceeded for a minimum of 16 hours. The nylon membrane was then washed briefly in
2X SSC and allowed to air dry prior to use in hybridization protocols.
Oligonucleotide Labeling
40pmol of oligonucleotide was radiolabeled in a reaction conraining 30pCi [y 32Pj -
ATP, 50mM Tris-HCl (pH 7.6), lOmM MgC12, 5mM DTT. LOOmM spennidine-HC1.
1OOmM EDTA (pH 8.0) and LO units T4 polynucleotide kinase (New England Biolabs,
Beverly, MA). The reaction was incubated at 37% for 1 hour then heated to 650C to
inactivate the enzyme. Oligonucleotide probes were ethanol precipitated prior to use by
adding two volumes ice cold 100% ethanol, 1/10 volume of ammonium acetate and 1pg
tRNA to the radiolabeled mixture. The samples were mixed well and cooled at -700C for 1
hour. Reactions were then centrifuged at 15000 rpm for 15 minutes (40C) using a Hettich
Mikroliter model D7200 microcenaifuge (Tuttlingen, Germany). The pellet was washed in
two volumes cold 7096 ethanol and the mixture centrifuged for 5 minutes at 15000 rpm
(4OC). The pellet was air dried then dissolved in deionized water.
Hybridization
Filters were placed in plastic hybridization bags and pre-hybridized at 37OC for 3
hours in 6X SSC, 0.1% SDS, 5X Denhardt's solution and lOOpg/m.L sheared and
denatured heterologous DNA. Re-hybridization solution was removed and a fresh aliquot
of the same solution containing the radiolabeled probe added. Hybridization proceeded
overnight at 370C in a shaking water bath. Following hybridization, blots were rinsed in
solution containing 2X SSC and 0.18 SDS then washed for 15 minutes in 2X S SC/O. 1%
SDS solution at room temperature. An additional wash in O.1X SSC/O. 1% SDS for 15
minutes at room temperature! was followed by washing in 0.1X SSCIO. 1 B SDS at 650C
for up to 30 minutes. The filters were exposed to Dupont Ulaavision G autoradiographic
6I.m (Wilmington, VA) with Dupont Lightning Plus intensifying screens (Wilmington, VA)
at -8OOC.
Sequencing
DNA Template Preparation
DNA templates for sequencing reactions were derived from PCR products
electrophoresed on 2% low melting point agarose gels (Gibco-BRL, Gaithenburg, MD).
Appropriate bands were excised, placed in sterile 1.5mL microcentrifuge tubes and heated
at 7OOC until agarose melted completely. PCR products were purified using the WizardIM
PCR preps DNA purification system (Promega, Madison, WI) according to manufacturers'
instructions.
Sequencing Reactions
AU sequencing reactions were performed using the 8hq cycle sequencing kit
(Amenham, Arlington Heights, IL) according to the manufacturer's instructions for use
with [f*P]-ATP end-labeled primer. Primers were labeled as previously described. Cycle
conditions for the termination reaction consisted of 950C for 30 seconds followed by 7 P C
for 120 seconds repeated for 30 cycles. Sequencing reactions were analyzed on 5%
denaturing acrylamide gels (see Appendix). Biorad's Sequi-Gen GT System sequencing
apparatus (Hercules, CA) was used to cast gels. 0.025% ammonium persulfate and
0.0 15% TEMED (Fisher Chemicals, FairIawn, VA) were included to polymerize gels.
Denaturing gel loading buffer was added to samples as 53% reaction volume, samples were
heated at 950C for 5 minutes and maintained at 850C prior to loading. Sequencing
reactions were electrophoresed in 1X TBE at a constant voltage of 2000V for 1.5-2 hours.
Gels wereblotted to 3MM paper and dried using Biorad's model 583 gel drier (Hercules,
CA). Dried gels were exposed to Dupont Ultravision G autoradiographic film (Wilmington,
VA) at -800C with Dupont Lightning Plus intensifying screens (Wi ig ton , VA)
Chapter 3
Expression of RET and its Multiple Splice Forms in Developing Human Kidney
1 performed all the analyses of RET and RET 5' splice variant expression in human kidney
development. The results of this work have been accepted for publication in Oncogene 18.
Introduction
The mammalian kidney develops through a series of reciprocal inductive
interactions between two cell groups that share a common mesodemal origin: ureteric bud
epithelium and metanephric mesenchyme 35. Upon induction. the ureteric bud an
outgrowth of the Woffian duct, grows and branches repeatedly to produce the collecting
duct system of the kidney while undifferentiated metanephric mesenchyme condenses and
epithelializes, forming glomeruli and proximal and distal convoluted tubules. A number of
molecules, including WT-141, WNT-4 52 and Pax-2 I26 and members of the Hox family
(reviewed in 39), have been implicated in induction of these differentiating events, as
described in Chapter 1 (see Figure 1.5). Recent studies have suggested that the RET proto-
oncogene may also be essential to these processes. RE'Tencodes a receptor tyrosine kinase
with roles in migration, development and survival of neural crest cells and their derivatives
14-16- 127. Multiple RET transcripts, generated by alternative splicing of RET exons
encoding the extracellular Ligand-binding and C-terminal domains, are expressed in cells
and tissues derived from the neural crest, branchial arches and ureteric bud I*-14.
Several pieces of evidence have suggested the involvement of RET in kidney
induction. Fist, in situ hybridization studies in murine embryos have identified RET
expression in the kidney as early as 8.5 dpc with highest levels in that portion of the
Woffian duct that will evaginate to produce the ureteric bud 14. RET expression is later
localized to the ureteric bud epithelium and the branching tips of the bud. Levels of RET
peak at 11.5 dpc then decrease with time. Second. the phenotype of the RET-I- mice
indicates that RET is essential to kidney development RET -1- mice display kidney
agenesis or severe dysgenesis characterized by reduced branching of the ureteric bud.
absence of a mature collecting tubule system and large areas of undifferentiated
mesenchyme 34. Third, ureteric bud tissue fiom RET+f+ mice is able to grow and branch
in culture in the presence of REI+/+ or -1- rnetanephric mesetlchymal tissue. However,
ureteric bud tissue from RET-/- mice fails to branch in the presence of either REW- or
RET+/+ mesenchyme suggesting that RET 4- bud is unable to transduce a mesenchyme-
derived signal 34-40. Finally, several recent studies have identified a ligand for RET which
is also implicated in kidney morphopnesis. The RET ligand is a multimeric complex
composed of GDNF, a soluble molecule, and GDNFR-a, a GPI-linked cell surface
receptor without an intraceIlular domain which must interact with RET to trmsduce signals
intraceilularly 21*2. GDNF -I- mice have phenotypic characteristics similar to their
RET-I- counterparts: kidney agenesis or severe dysgenesis and absence of the enteric
ganglia 46-48. Consistent with RET's proposed role as a transducer of mesenchyme-derived
signals in kidney induction, GDNF expression has been localized to the metanephric
mesenchyme 29.
Although murine studies have suggested developmental regulation of RET in
kidney organogenesis, the expression of RET in human kidney development has not been
investigated. In this study, we examined RET expression in a panel of human fetal kidney
RNAs using semiquantitative reverse transcription-polymerase chain reaction (RT-PCR).
We have found that RET expression is developmentally regulated with highest expression
in the earliest gestational ages decreasing with time and with lowest levels of RET being
detected in adult kidney. In addition, we show that the developmental expression patterns
are dissimilar amongst the various RET alternative transcripts. Our data suggest that an
alternatively spliced form of RET. which encodes a product lacking a portion of the
extracellular ligand-binding domain (Figure 1.3), has a higher prevalence and perhaps a
greater sigruficance at the earliest developmental stage of the human kidney.
Results
RET Erpression in Human Kidney Development
We examined the expression of RET in a panel of RNAs prepared from human fetal
kidneys ranging in gestational age from 8 to 24 weeks and from adult kidney. RNA from
medullary thyroid carcinoma cell line TI; known to express JET at high levels, was used
as a positive control 74- 128. Owing to limited quantities of RNA available for analysis, RT-
PCR was used to investigate RET expression. Initial analyses were conducted using
primers CRTl7S and CRT17A which amplify RET sequence coding for the region just
within the RET tyrosine base domain 9. This 122 bp amplicon is present in all
transmembrane RET isoforms and would thus serve as an indicator of overall RET
expression. RT-PCR of total RNA identified an amplification product of the predicted size
for a l l ages of fetal kidney examined as well as for adult kidney and the TT cell Line (data
not shown). Initial inspection suggested that the level of RET amplification for adult kidney
was relatively lower than the levels observed for our fetal kidney samples and the IT cell
he, suggesting a developmentally regulated RET expression pattern. This is consistent
with previous mouse and rat studies which showed that levels of RET expression decrease
with time during kidney development 1.14-16.
Quantitation of RET EApression During Human Kidney Development
To investigate relative REl expression levels during human kidney organogenesis,
we developed a semiquantitative RT-PCR assay that compared relative expression level of
RET and a housekeeping gene, P-glucumnidase (GUSB), in a given RNA sample using
multiplex PCR. Qualitative RT-PCR is used to determine the presence or absence of gene
expression whereas quantitative RT-PCR is used to determine how many target molecules
are present in a given sample. Semiquantitative RT-PCR lies somewhere in between the
two and is used to investigate the expression level of a target gene relative to a standard
reference gene. The accepted term for assays investigadng the comparison of relative
expression levels is semiquantitative RT-PCR 13'. Previous studies have shown that
GCrSB is consistently expressed in kidney throughout the examined developmental stages
129- 130. PCR was performed with primers CRTlTS and CRT17A to amplify RET and
GUSB3 and GUSBS to amplify a GUSB product of 195 bp. A LO: 1 molar ratio of RET
primers to GUSB primers proved to be optimal for co-amplification of both products. PCR
amplification proceeds exponentially; therefore, for reliable quantitation of product, PCR
conditions must be selected so that quantitation is pedormed in the linear phase of
arnplitication where concentrations of product are proportional to starting levels of target
131. Experiments were conducted to determine the kinetics of arnpiif?cation over a range of
cycle numbers to select conditions for which amplification was linear. End-labeled forward
primers were included in PCRs and the quantity of PCR product was represented by the
amount of radioactive incorporation. Template cDNAs were amplified for 12, 16, 20, 24,
28, 32 or 36 cycles. The relevant products were quantitated by separation on 2% agarose
gels, excision of the appropriate bands and measurement of incorporated counts (cpm). We
found that amplification was linear for both GUSB and RET between 18 and 26 cycles
(Figure 3.1). To ensure that amplification occurred with e q d efficiency regardless of
amount of starting template, we performed PCR using a two-fold serial dilution of TI'
cDNA for 22, 25 or 26 cycles. A linear relationship between input cDNA and amount of
PCR product was identified for each of GUSB and RET when PCR proceeded for 25
cycles (Figure 3.1).
In our analyses, we chose to investigate RETexpression in six kidney RNA
samples that spanned the range of gestational ages available: 7.5,8.5, 10.5, 14, 18 and 24
weeks gestation as well as adult kidney. The reliability of the conditions established for
quantitation of transcripts in the TI' cell Line was confumed for fetal kidney. Quantitation of
RET expression relative to GUSB expression during human kidney development was
performed at 25 cycles of PCR. Semiquantitative assays were repeated five times for each
of the human fetal kidney samples as well as for human adult kidney and mean expression
Figure 3.1 Determination of conditions for semi-quantitative RT-PCR analysis of o v e d
RET expression in human fetal and adult kidney. A] Kinetics of simd*laeous ampLification
of RET and 8-glucuronidase (GUSB). Amounts of REl and GUSB product amplified in a
single multiplex reaction were quantitated by liquid scintillation counting of radioactivity
incorporated in PCR products which had been resolved on 2% agarose gels and excised.
Counts (measured in cpm) were plotted relative to the number of ampLification cycles. The
exponential reaction was linear between 22 and 26 cycles. At 26 cycles, rates of
amplification for both RET and GUSB products decreased and approached plateau B]
Confirmation of amplification efficiencies of RET and GUSB primers used in multiplex
PCR for semiquantitative analyses of overall RET expression. A two-fold serial dilution of
TI' cDNA was subjected to 22, 25 or 26 cycles of PCR. The results for 25 cycles are
shown. Linear results were obtained when counts were plotted relative to dilution factor for
amplification of both RET and GUSB transcripts indicating comparable amplification
efficiencies for these primer pairs.
4 b
too0
, . b
a m - 100 a* -
LO me- GUSB S I
4 b . b
I I 1 I m I 1 ~ 1 ~ 1 I
16 18 20 22 24 26 28 30 32 34 Number of PCR Cycles
Two-Fold Serial Dilution Factor
with standard deviation calculated. The expression of REl relative to GUSB was assessed
by comparison of incorporated counts, where RET product was expressed as a fiaction of
GUSB product (Table 3.1). RETexpression levels were highest in the 7.5 week kidney
but lower in the 14 week sample by 3.7 fold RET expression differed between 14 week
and 18 week kidney by 1.5 fold. Expression was only slightly Lower in 24 week kidney.
differing from expression in 18 week kidney by about 2%. RET level in adult kidney was
1.2-fold lower than those in 24 week kidney and almost 7-fold lower compared to 7.5
week kidney. Thus, RETexpression appeared to decrease with increasing gestational age.
RET Alternative Splice Variants
Our initial analyses indicated that RET was expressed in a developmentally
regulated fashion in the human kidney. Although this may reflect overall reduction in RET
expression, it could equally represent differences in expression of the many RET mRNA
forms generated by differential splicing. Alternative RET transcripts in which exon 2 may
be juxtaposed to any of exons 3, 4, 5 or 6, resulting in a shorter putative RET ligmd
binding domain, have been reported (Figure 1.3) 13. Using the sample panel described
above, we investigated the expression of these variant RET transcripts during human
kidney development In order to distinguish the various RET -As generated by
alternative splicing of RET 5' exons, RT-PCR analyses were conducted using primer
combinations that ampLified each independently and exclusively (Figure 3.2). Speciticity
was ensured by using a forward primer that spanned the splice junction of exon 2 and the
downstream exon and a reverse primer within the downstream exon. Amplicoos predicted
for full length (FL) transcript and those lacking exon 3 (2/4), exons 3 and 4 (215) and
exons 3,4 and 5 ( 2 6 ) were 210 bp, 262 bp, 196 bp and 148 bp respectively.
PCR amplification specific for each aanscript was performed using the panel of
fetal and adult kidney samples descnid above. Products were resolved on agarose gels.
Southern blotted and probed with an end-labeled oligonucleotide specific for the 3' exon
Table 3.1. RET expression ~lat ive to GUSB expression in human fetal kidney.
Quantitation of RET relative to GUSB was based on multiplex RT-PCR analyses. GUSB
expression levels have been normalized to 1-00 in al l samples- Means and standard
deviations (sd) for five repeats are given in the table.
Sample Mea-sd
7.5 week 6.68+0.05
8.5 week 3.83k0.27
10.5 week 2.53&0.20
14 week 1 -83+0. 1 1
18 week 1 -29H.02
24 week 1 -25fl.02
Adult 1 *05+0.0 1
Figure 3.2. Expression of RETmRNA forms generated by alternative splicing at the 5' end
of the gene in human fetal and adult kidney. PCR amplification of the four RET mRNA
forms was conducted using primer pairs described in Chapter 2. The predicted product size
for each amplification, as well as the exon location of the primers used to amplify the
specific products, is indicated. PCR products were resolved on 2% agarose gels, gels were
Southern blotted and membranes were hybridized to a second labeled primer corresponding
to the 3' exon.
present in each amplified product. A single PCR product corresponding to each of the
predicted sizes was observed in all samples of fetal and adult kidney indicating that each
RET 5' spliced variant is expressed from 8 weeks through 24 weeks gestation (Figure
3 -2).
Quuntitation of RETAItemolive Splice Varimts
We addressed the possibility of variation in expression of RET 5' alternative splice
variants using a semiquantitative RT-PCR assay similar to that described above. W e
compared the expression level of each RET alternative transcript to that of FL RET in our
panel of human kidney RNA by pairwise amplifications using three primers in each
reaction: a single forward primer in exon 2 (X2S) and two reverse primers, one in exon 3
(CRT7A) and the other in one of exons 4 (X4A), 5 (E5A) or 6 (E6A). In combination with
a f o m d primer in exon 2, the latter primers would amplify alternative splice variants 2/4,
215 and 2/6 respectively. Although, in theory, the forward primer and any of the reverse
primers would amplify full length transcripts as well, these Longer products were not
detected.
As described above, optimal RT-PCR conditions for comparison of expression of
the different RET transcripts were chosen based on experiments which defined the linear
range of amplification. Amplification was found to be linear between 22 and 30 cycles for
all primer combinations (data not shown). Quantitative PCR analyses were performed at 28
cycles of amplification which was both within the hear range for all primer combinations
and permitted visualization of even the least abundant transcript upon electrophoresis. To
ensure that amplification occurred with equal efficiency regardless of amount of starting
template, we performed PCR using two-fold serial dilutions of 14, 18 and 24 week human
fetal kidney samples as well as adult kidney and TT cell line cDNAs.
Initially, we investigated RET expression in RNA samples From 14, 18 and 24
week as well as adult kidney. RT-PCR experiments were performed at 28 cycles of
amplification and the expression levels of alternative RET transcripts were calculated as
fractions of ET RET. Quanatation of each alternative RET =dpt in a sample was
repeated twice for each of three independent cDNA preparations and the data summarized in
Table 3.2. We found that FL, RET was the most highly expressed RET transcript in each
sample analyzed The expression Levels of the RERI4 and REZ2/5 W p t s were both
much lower than those of FL, RET . These aaDmipts maintained a level of expression
approximately 113 that of FL, RET at al l stages of development
The REN6 transcript was the least abundant transcript in all samples tested, being
expressed.at 0.22fl.02 times the levels of K RET in 14 week kidney and at lower levels
in 18 week (O.18fl.02) and 24 week kidney (O.l&O.O3) (Table 3.2). In adult kidney, the
expression level of W 6 was approximately 116 that of FL RET. Our data suggested that
expression of the RETU6 transcript was higher in eadier stages of human kidney
development relative to other RET 5' splice variants and decreased more rapidly through to
24 weeks gestation.
In order to confirm this observation, we compared the expression of FL RET and
W 6 in our full panel of human fetal kidney RNAs. The expression level of the R E W 6
transcript relative to FL, RET was calculated as described above. We found that RE7216
was expressed at higher levels in the eariiest gestational ages of human kidney we
examined (0.26&@02 in 8 week kidney), approaching the relative levels of -4 and
REZ2/S seen throughout our tested samples (0.15H.02 in 24 week and 0.149.02 in adult
kidney) (Table 3.3, Figure 3.3).
Discussion
The mature metanephric kidney arises from inductive interactions between epithelial
(ureteric bud) and mesenchymd (metanephric mesenchyme) cells. It is clear that this
complex process involves a number of biochemical signals rather than a single molecular
event. The RET RTK and members of its Ligand complex, GDNF and GDNFR-a, are
likely to play roles in both kidney induction and morphogenesis. Using semiquantitative
Table 3.2. RET 5' splice variant expression relative to full length RET (FL, RET)
expression in human fetal kidney. Quantitation of multip1e RET alternative transcripts
dative to FL RET was based on muitiplex RT-PCR analyses. Means and standard
deviations were calculated from the results of six individual assays.
RE71u4 RE;IZ/S W 6
Sample FL REl Mkanksd Neanksd Meauksd
14 week 1 .OO 0.32H.04 0.3 1H.04 0.22H.03
18 week 1 .OO 0.3SH.05 0.3 1H.06 0.20_+0.02
24 week 1 .OO 0.3m.05 0.33fl.05 [email protected]
Addt 1 .OO 0.32H.05 0.29fl.05 0 .1w.02
'IT ceUs 1 .OO 0.3 1H.04 0.3 1fl.04 O.l4&0.02
Table 3.3 Quantitation of RETZ16 relative to FL RET based on muItiplex RT-PCR
analyses. Means were calculated based on six individual v a t s of the assay.
-6
Sample FL RET MeankSD
8 week 1-00 0 . 2 w - 0 2
12 week 1 .OO 0.25H.04
13.5 week 1 .00 0.25fl.05
14 week 1.00 0.22&0.03
14.5 week 1.00 0.23+0.04
15 week 1.00 0.23a.03
15.5 week 1.00 0.2 1fl.02
16 week 1.00 0.20+_0.03
16.5 week 1.00 0.2 1M.03
18 week 1.00 0.20+0.02
20 week 1.00 0.18~0.04
21 week 1.00 0.19k0.02
22 week 1 .00 0. I7fl.02
23week 1 .OO 0.15fl.02
24 week 1.00 0.15+0.02
Adult Kidney 1.00 O.lck_O.O2
TT cells 1.00 O.lS+0.02
Figure 3 -3. Developmental expression of RET 5' splice variants in human fetal kidney.
A] Levels of alternatively spliced RM transcripts were calculated as fractions of the FL
RET transcript amplified in the same RT-PCR reaction for a given sample. After
electrophoresis of PCR products, quantitation was achieved by scintillation counting of
radioactivity incorporated in PCR products, made possible by including 0.1w of end-
labelled s e w strand primer in reactions. B] Rome of developmental expression of
RETU6 transcript generated by splicing exon 2 to exon 6. Expression levels of RETU6
were calculated as fractions of FL RET as described above.
0 12 14 16 18 20 22 24
Gestational Age of Kidney (weeks)
rn FLRET RETU4
A RETUS RETU6
Gestational Age of Kidney (weeks)
RT-PCR methodology, we have shown that RET is expressed in human fetal kidney
during the 8 to 24 week period of gestation. Further, RETexpression is highest early in
development but decreases through to 24 weeks gestation relative to expression of a
housekeeping gene control. This is consistent with the RETexpression pattem observed in
mice and rats where RETexpression has been localized to the ureteric bud in early kidney
development but later appears in the actively growing tips of the bud branches lCL6.
The relatively high RET expression level early in development coincides with a
stage of kidney morphogenesis in which the ureteric bud undergoes rapid bifiucation (fkom
8 until 14 weeks human gestation). A period of rapid branching is initiated at 8 weeks and
continues until 14- 15 weeks when the rate of branching slows. During this period, cells of
the metanephric mesenchyme condense, epithelialite and begin to differentiate to form the
nephrons while the ureteric bud continues to branch and bud cells proliferate (reviewed in
37). While the ureteric bud is active fkom the time of its development through to 36 weeks
intrauterine Life, the role of the bud varies during the process of kidney development.
During this period, the bud induces condensation and epithelialization of the surrounding
mesenchyme, resulting in nephrons which attach to tubules that form within the zone of
bud growth. Branching seldom occurs between 20 and 32 weeks (reviewed in 37). Given
the relatively higher expression level of RET we observed in 7.5 week human fetal kidney
compared to 24 week fetal kidney, it is possible that RET's significance changes according
to the stage of renal development. The RET expression pattern suggests a more significant
involvement of RET in earlier developmental stages, however, whether it functions in cell
differentiation, proliferation or both requires further investigation.
The developmentally regulated pattern of M T expression in human kidney
suggests that RE' may have varying roles or signiscame at different stages of kidney
development. It is possible that this effect is simply mediated by the relative level of overall
RET expression. However, it is also possible that differences in expression of the various
RET alternatively spliced transcripts &ect RET's contribution to the process of kidney
development. Multiple isoforms of RET arise as a result of alternative splicing events 6. 12+
L3. These RET isoforms may have different roles in human renal development, perhaps by
recognizing different RET ligands or binding the same Ligand with different affinities. We
have shown that all RE15' spliced variants are expressed in the human kidney throughout
the 8 to 24 week gestational period but that the relative levels of these alternative RET
forms vary (Figure 3.3). FL RET was most abundant in all samples while -4 and
RET 2/5 transcript expression levels were consistently about 113 that of FL RET.
Interestingly, however, REW6 expression levels varied with respect to all other RET
splice forms, being relatively more abundant in the early kidney developmental stages
(0.26fl.02 in 8 week sample) and decreasing more markedly to low adult levels
(0.15fl.02) (Figure 3.3).
Although all RET mRNA forms are expressed at relatively high levels during early
kidney development and decrease with time, the variation in RETU6 expression is most
striking. In neural crest-derived cells, RET is predicted to function in both differentiation
and proliferation processes. Activated fonns of RET have the ability to induce
differentiation in PC 12 cells 132-134. In contrast, activated RET is transforming in N W T 3
cells and results in proliferation 81- 134. 135. In human kidney, it is not clear which role is
chiefly attributable to RET. However, it is conceivable that different RET isoforms may
have different roles. Lorenzo et al. examined the relative levels of RET 5' alternatively
spliced transcripts in a panel of hunours of neural crest origin 13. In these analyses,
RE12/6 expression was approximately 1/10 FL RET expression, similar to the expression
levels we detected in adult kidney. Our data show that the high expression level of RE2216
coincides with the period of rapid bud bifiucation and growth of the ureteric bud. If
R E W 6 was simply a marker of rapidly dividing cells, we would expect to see similar
levels of this transcript in developing fetal kidney and nunours. However, our data suggest
that levels of RETU6 are comparable in neural crest-derived tumours and cell lines and in
human adult kidney, tissues with very different proliferative profdes. In fact, RER/6 was
2.5-fold more abundant in 8 week human fetal kidney than in either human adult kidney or
the TT cell line. These data suggest that the RER16 product may have a non-proliferative
role in human kidney morphogenesis.
Many RTKs generate multipie isoforms by alternative splicing. When such events
occur near the 5' end of the gene, ligand-binding domains can be affected resulting in
altered ligand-binding specificities. In the case of fibroblast growth factor receptor type 2,
for example, alternative exon usage in the immunoglobulin-like loop region results in
receptor variants with different Ligand-binding affinities 6** 69- These transcripts are
expressed in a tissue- and developmental stage-specific fashion 64* 70- The relatively
high expression of RERI6 in early human renal development may represent a requirement
for this specific RJX isofom during that time. The RETU6 transcript encodes a molecule
that lacks 239 amino acids spanning four potential N-linked glycosylation sites, seven
cysteine residues and the region of cadherin homology which are a l l present in FL RET
(Figure 1.3). Ligand binding is thought to involve all or part of this region 9. Given the
decreased Length of this region in -6, it is possible that this molecule binds a different
ligand than its full length counterpart or that it binds the same ligand with differential
affinity.
Recently, the RET ligand was identified as a novel form of multicomponent Ligand
complex, consisting of GDNF and GDNFR-a 21. 22. GDNF is a soluble molecule which
forms disulfide-linked dimers that bind to a novel GPI-linked protein, GDNFR-a. The
GDNFIGDNFR- a complex then binds to RET which dirnerizes. resulting in
autophosphorylation and downstream signaling 21. 33. We have identified expression of
both GDNF and GDNFR a in human fetal kidney ranging in gestational age from 7.5 to
24 weeks (discussed in Chapter 5). Expression of these transcripts during kidney
development is consistent with their role as RET ligands. The phenotype of RET-I- and
GDNF-f- mice and in vitro explant studies have clearly shown that both RET and GDNF
are required for inductive events during kidney development. Interestingly, the differences
in phenotype between RET-I- and GDNF-/- mice have suggested that another RET ligand
may exist. In REF/- mice, the superior cenical ganglion neurons are absent 349 36 while
they are only moderately reduced in GDW-/- mice 46-4*. In other respects. these mice have
very similar phenotypes. The RETU6 transcript is predicted to encode a molecule that
differs fiom its full length counterpart in that it lacks a portion of the protein thought to be
involved in Ligand-binding. Thus, RETU6 is a logical candidate as a receptor for an
alternative ligand.
Our data have shown that multiple RET 5' splicing variants are expressed in a
developmentally regulated fashion during human kidney development (Figure 3.3). 'The
relatively high expression levels and clear developmental differences in expression of these
variants suggest that they represent fuactional isofonns and not tolerated artifacts of
splicing. Interestingly, RET2/6, the RET isoform with the shortest extracellular domain,
had the strongest developmental variation in expression. REW6 lacks part of the predicted
region of ligand binding present in FL, RET which raises the possibility that it interacts with
a different Ligand with relevance to mammalian kidney development. Thus, metanephric
kidney formation may be dependent on more than one role for RET: the
RETIGDNFIGDNFEt-a interaction and another as yet uncharacterized signaling molecule.
Materials and Methods
Growth of 77' Cells
The medullary thyroid carcinoma cell line 'IT was grown at 370C in humidified air
in L-L5 medium (Gibco-BRL Life Technologies) supplemented with 10% fetal calf serum
(Wisent) and gentamycin (50 pg/ml). Cells were grown as monolayers and replated
weekly.
RNA Eitraction
Total RNA was isolated fiom TT cells using the TRIzol method according to
manufacturers' instructions as described in Chapter 2 (Gibco-BRL Life Technologies).
Total RNA was isolated &om adult kidney tissue and feral kidney tissue ranging in
gestational age Earn 8 weeks to 24 weeks essentially by the method of Chomczynski and
Sacchi 124-
Feral Kidney, Adult Kidney and lT RNA Analyses
One pg of total RNA was heated at 7WC for 5 minutes and cooled on ice briefly.
First strand cDNA was generated from these templates by incubating in 50mM Tris-HCl
(pH 8.3), 8mM MgC12. 3 W KCl, lOmM dithiothreitol 0. 2mM deoxynucleoside
hiphosphates (dNTE%), 7 units AMV reverse transcriptase (Promega). 2 units human
placental RNase inhibitor (Pharmacia) and either Z p M random hexamer primers
(Pharmacia) or 2p.M oligo dT15 primer (GENOSYS) at 420C for 1 hour. To inactivate the
enzyme, samples were incubated at 650C for 10 minutes and then fkozen at -200C. PCR
amplification of cDNA templates was pedonned in lOmM Tris-HCl (pH 8.3). 50mM KCl.
0.0 1% gelatin. 1pM of each primer. 2OOw dNTPs and 1.5 units Toq DNA polymerase
(Gibco-BRL Life Technologies) with 0.75-1.5mM MgCI2 depending on primers being
used. Unless otherwise stated, PCR amplification was carried out for 40 cycles of 95oC 1
min/S50C 1 min/72OC 1 min.
Semi-quuntifative PCR
himers used in semiquantitative RT-PCR analyses are described in Chapter 2. For
~uantitation experiments, RT-PCR was performed in 10pL volumes using the PCR
conditions described above but including O.1p.M 32P-end-labeled sense-strand primers and
varying the amounts of cold primers used and MgC12 buffcr concentrations. Specifically, in
multiplex PCR to amplify RET and GUSB products, 1pM RET primers (CRT17S,
CRT17A) and 0.1pM GUSB primers (GUSB3, GUSBS) were used in 1SmM MgClz
buffer conditions. To amplify the REl alternative splice variants, 1p.M concentrations of all
primers were used in pairwise amplification experiments (CRVAK2SIX4A,
CRT7A/X2S/ESA, CRT7A/X2S/E6A) in buffer containing 0.75mM MgC12. Analyses to
determine the hear range of amplification wen performed using 1/10 of a cDNA reaction
as described above in PCR for 12, 16, 20, 24, 28, 32 or 36 cycles. PCR products were
separated on 2% agarose gels and appropriate bands were excised. Quantitation of PCR
products was determined by liquid scintillation of incorporated radioactivity. Plots of
incorporated counts (cpm) versus cycle number were examined to define the range of PCR
cycle numbers for which amplification was linear (Figure 3.1). Two-fold serial dilutions of
cDNA were subjected to cycles of PCR within the hear range to confirm the number of
cycles which would amplify with similar efficiency regardless of amount of starting
template. PCR products were separated on 2% agarose gels, appropriate bands were
excised and Liquid scintillation counting was used to measure incorporated radioactivity
(measured in cpm). If the relationship of cprn versus dilution factor was bear, the
conditions were considered reliable for quantitation purposes (Figure 3.1). For quantitation
of RET relative to GUSB, 25 cycles was chosen for al l funher studies while for
quantitation of RET alternative splice variants relative to FL RET, 28 cycles was used for
al l fuaher experimentation.
Southern Blomkg
PCR products were resolved on 2% agarose gels and transferred to Hybond N+
membranes (Amenham). OLigonucleotide probes were labeled in a reaction containing
30pCi **P]-ATP. 10 units of T4 polynucleotide kinase (Gibco-BRL Life Technologies),
SOmM Tris-HC1 (pH 7.6), lOmM MgC12, 5mM D'IT, lOOmM spermidhe-HC1, lOOmM
EM'A (pH 8.0) at 370C for 30 minutes. Probes were ethanol precipitated prior to use.
Blots were prehybridized and hybridized at 37OC as described in Lorenzo et al. '3 and
washed in 0. 1XSSCIO. 1 %SDS at 650C.
Chapter 4
Expression of RET 3' Splicing Variants During Human Kidney
Development
I performed all the analyses of RET 3' coding variant expression in deveioping human
kidney. The results of these experiments have been submitted to the journal Oncogene for
publication.
Introduction
The development of the mature mammalian kidney requires a series of reciprocal
inductive interactions between ureteric bud epithelium and metanephric mesenchyme.
Mouse metanephric kidney development begins around 10.5-1 1 dpc when induction of the
WoEl5an duct produces a diverticulum, the ureteric bud 35. Metanephric mesenchyme, a
dense blastema of mesenchyme in the vicinity of the W o E a n duct, induces the ureteric bud
to grow and branch repeatedly giving rise to the collecting duct system. At the same time,
the ureteric bud induces undifferentiated metanephric mesenchyme to condense,
epithelialize and uldmately differentiate to form the glomeruli and proximal and distal
convoluted tubules. The precise mechanisms of the differentiation events are unclear.
However, a number of molecules, including WT-I 41, W-4 52, PAX-2 126 and HOX
family members (reviewed in 39), have been implicated in the induction of these processes.
In addition, recent studies suggest a requirement for the RET receptor tyrosine kinase in
kidney induction. RET is expressed in cells and tissues derived from the neural crest,
branchid arches and kidney 12- 14. In situ hybridization studies have localized RET
expression to the ureteric bud in embryonic rnurine kidney i4. Consistent with RE'
involvement in tbe induction of kidney morphogenesis is the phenotype of the RET -/-
mouse which includes kidney agenesis or severe dysgenesis 34. In v i m tissue mixing
experiments using ureteric bud and mesenchyme tissues from RET-I- murine embryos and
normal control murine embryos coatirm that hctional RET expression in the ureteric bud,
but not in rnetanephric mesenchyme. is required for the induction of bud growth and
branching 34- 40. RET's proposed role as a transducer of mesenchyme-derived signals in
kidney induction is supported by the localized expression of GDNF, which encodes a
soluble member of the RET ligand complex, to the rnetanephric mesenchyme 20. 29.
Phenotypic similarities between REF/- and mice null for GDNF, including kidney
ageaesis or severe dysgenesis, have recently been descnid confirming the requirement for
both RET and GDNF in kidney induction 4648.
RET encodes multiple transcripts resulting b m alternative splicing of 5' or 3 '
exons 6- 12- 13- Splicing of exon 2 to any of exons 3, 4, 5 or 6 at the 5' end of RET
generates transcripts predicted to encode proteins with altered extracellular domains. As
described in Chapter 3. expression of RET 5' alternatively spliced variants is
developmentally regulated during human kidney organogenesis 18.
Alternative splicing at the 3' end of RET results in transcripts encoding RET
isoforms with different C-tennind amino acids 6- 12. RET exon L9 is present in all
transcripts, however, Merentid splicing at the 3' end of exon 19 results in transcripts
where exon 19 is unspliced spliced to exon 20 or spliced to exon 21 (Figure 1.2). These
transcripts encode RET isofonns with distinct 9 (RET9)' 5 1 (RETS I) or 43 (RET 43) C-
tenninal amino acids respectively. Multiple polyadenylation sites and 3' UTRs associated
with these three coding variants have also been identified 6. 12. h this chapter. we have
confined ourselves exclusively to the discussion of the tbRe different coding sequences
irrespective of the associated UTR. The sequences of the proteins encoded by the RET 3 '
alternatively spliced transcripts diverge at amino acid 1063 12. The final common amino
acid for all three isoforms is a tyrosine (Y1062) which has been shown to be
phosphorylated on RET activation 136. Alternative splicing places Y 1062 in different amino
acid contexts in the three RET isoforms coderring it with different binding capabiIities 9.
In the sequence context of RETS 1, pY 1062 can interact with the Shc-PTB domain (Figure
4.1). While pY1062 in the sequence context of RET9 can also interact with the Shc-PTB,
the same pY has a higher affinity for the ShcSH.2 domain F~gure 4.1) (M. Billaud,
personal communication) 57. RETS 1 contains two additional tyrosine residues (Y 1090 and
Y lO96) not present in either of RET9 or RET43 6. 12. Y lO96 has been identified as an
autophosphorylation site 136 able to interact with Grb2-SH2 domains directly 4.1)
56. Y 1090 has not been demonstrated to become phosphorylated on RET activation.
Functional evidence that these differences in effector binding alter cell phenotype
has been shown by Rossel et al. who observed more prominent neurite outgrowth in PC 12
cells transfected with activated RET5 1 compared to activated RET9 constructs 55. The data
are conflicting with respect to the relative transforming potentials of the RET9 and RET5 1
isoforms, however, in the only study to compare the transforming abilities of RET9 and
RETS 1 directly, no differences were observed 55. The muscript encoding RET43 has only
recently been identified and the hction and interactions of this isofom have not yet been
investigated. However, we have identified expression of the RE143 transcript in human
thyroid and kidney and in neural crestderived hunours 6. 18.
In this study, we examined the expression of RET 3' alternatively spliced variants
in a panel of human fetal kidney RNAs using semiquantitative reverse-transcriptase
polymerase chain reaction (RT-PCR). We observed expression of transcripts representing
RE79 and RET43 throughout our sample panel. RE19 was the most abundant of the 3'
splicing variants in all samples examined while RET43 levels were not high enough for
accurate quantitation (42% of RET9 expression levels). Interestingly, we observed very
low levels of RET5 1 expression in the earliest gestational ages then a Ffold increase in the
Figure 4.1 RET 3' isofonn interactions with downstream effector molecules. The C-termini
of RET9 and RETS1 are shown. The amino acid sequence immediateiy upstream and
downstream of a phosphotyrosine (pY) can confer afbity for specific downstream
effectors. RET9 and W S 1 share amino acid sequence upstream of Y 1062 (LPN). The
presence of this amino acid sequence N-terminal to pY1062 suggests that the tyrosine is
capable of interacting with the PTB domain of Shc upon phosphorylation. However,
Y1062 in the sequence context of RET9 downstream sequence (YGRI) has greater affinity
for the SH2 domain of Shc. The YGRI sequence is bolded in RET9 to indicate a preference
Shc-SH2 domain interaction at Y 1062. RET51 stronger affsnity for Shc-PTB at Y 1062 and
has an additional Grb2-SH2 domain interaction site at Y1096 (YANW), one of the two Y
residues not present in RET9.
relative expression level of this transcript by 9 weeks gestation. Our data suggest that the
RET 3' variant encoding the RETS 1 isoform is not required for early kidney inductive
events. However, RETS 1 expression may be important for differentiation events
responsible for shaping the mature humao kidney.
Results
Expression of RET 3' AltemutiveIy Spliced Transcripts
We examined the expression of RET 3' alternatively spliced transcripts. which
differ with respect to the C-terminal amino acids they encode, in a panel of RNAs prepared
from human fetal kidneys ranging in gestational age from 7.5 through 24 weeks and human
adult kidney. RNA from a medullary thyroid carcinoma cell he , TT, known to express
RET at high levels, was used as a positive control T4. Given the Limited quantities of RNA
available for analysis, RT-PCR was used to investigate the expression of these transcripts.
For each analysis, primer pairs were selected to specifically amplify one of the RET 3'
alternatively spliced coding variants. A single fornard primer, CRT 148. that corresponds
to REl exon 19 sequence, was used in combination with reverse primer KRT14D.
KRT20A or KRT3B (Figure 4.2) to arnpliry transcripts corresponding to RED, RETS 1 or
RET43 C-terminal amino acids respectively 6. PCR products were electrophoresed on
ethiciium bromide-stained 2% agarose gels. We identified the (109 bp) and RET43
amplicons (177 bp) in a l l ages of human fetal kidney examined as well as in adult kidney
and the TI' cell line control (Figure 4.3). However, the ET" 1 amplicon (88 bp), which
corresponds to transcripts in which RET exon 19 is spliced to exon 20 (Figure 1.2), was
detected at much lower levels in the 7.5 week human fetal kidney, the earliest age available
to us, relative to the 12 week fetal kidney, the next gestational age analyzed (Figure 4.3).
This observation was independently confirmed by the reactions described above using
primers CRT14B (exon 19) and KRT3B (exon 21). In addition to the 177 bp product
representing the exon 191exon 21 splice which corresponds to RE143, a PCR product of
Figure 4.2 Schematic of RET 3' exons and primers used in RT-PCR analyses. The intmn
and exon organization of the RET 3' end is represented Coding sequence is indicated by
boxes. Non-coding sequence is indicated by lines. The approximate locations of primers
relative to the RET 3' exons are indicated with arrows.
Figure 4.3 Expression of RET 3' coding variants in human fetal and adult kidney. RT-PCR
analyses were used to detect expression of the tbree RET 3' coding variants in fetal kidney
ranging in gestational age from 8-24 weeks (wk). Primer pairs used in these analyses are
described in Chapter 2. The size of the predicted amplification product for each variant is
indicated. A] Expression of R E D , B] expression of RETS 1 and c} expression of RET43.
Positive (+ve) and negative (-ve) controls are indicated.
353 bp was also produced (Figure 4.3). We have shown previously that this product
results from splicing of exon 19 to exon 20 6 . This mRNA encodes a RETSL aanscript
with a 3' UTR extending through a non-coding exon 21. Although the 177 bp amphcon
corresponding to RET43 was detected in al l fetal kidney samples, the 353 bp product
corresponding to RET51 was present only in samples ranging in gestational age from 12
through 24 weeks. Our data suggested that RET51 was absent in early kidney
developmental stages and that the initiation of RETSl expression occuned after 7.5 and
before 12 'weeks gestation.
Qmtitation of RET 3' Alternatively Spliced Varirts
To investigate the ~ I a t i v e expression levels of the three RET 3' coding variants duriag
human kidney organogenesis and to characterize the early expression of REn 1, we used a
semiquantitative RT-PCR assay simiIar to that previously described in quantitation of RET
5' spliced variants 18. We compared the expression levels of RE73 1 and RET43 relative to
REIP, the most abundant of these transcripts, within a single RNA sample using multiplex
PCR A single fornard primer in exon 19 (CRT MB) was used in combination with reverse
primers in intron 19, exon 20 and exon 21 to amplify RE79, RETS1 and RET43 transcripts
respectively in a single reaction w~gure 4.2). Initial experiments were conducted to
determine the kinetics of amplification over a range of cycle numbers in order to select
conditions for which amplification was linear. End-labeled forward primers were included
in PCRs and the quantity of PCR product was represented by the amount of radioactive
incorporation. Template cDNAs were amplified for 16, 20, 24, 28, 32, 36 or 40 cycles.
PCR products were separated on 2% agamse gels, the appropriate bands excised and
incorporated counts measured by liquid scintillation. We found that amplification was Linear
for all products between 20 and 26 cycles of PCR (Figure 4.4). To ensure that
amplification proceeded with equal efficiency regardless of amount of starting template. we
performed PCR using a two-fold serial diIution of TT cDNA for 22. 24 and 26 cycles. A
Figure 4.4. Determination of conditions for semiquantitative RT-PCR analysis of RET 3'
coding variant expression. A] Kinetics of simultaneous ampiification of RED. RET5 1 and
RET43. Amounts of the three transcripts amplified in a single multipIex reaction were
quantitated by liquid scintiuation counting of radioactivity incorporated in PCR products
which had been resolved on 2% agarose gels and excised. Counts (measured in cpm) were
plotted relative to the number of amplification cycles. The exponential reaction phase was
hear between 20 and 26 cycles. Above 26 cycles, rates of ampLification for all RET 3 '
coding variant products decreased and approached plateau. B] Confirmation of
amplification efficiencies of RET primer pairs used in multiplex PCR. The results for 24
cycles are shown. Linear results were obtained when counts were plotted relative to
dilution factor for amplification of all RET 3' variant transcripts. Similar slopes for the
linear plots indicate comparable efficiencies for all primer pairs. Differences in slopes were
accounted for in final calculations using the formula (Mi/')(caIcuIated value) 131.
2 3 Two-Fold Serial Dilution Factor
linear relationship between input cDNA and amount of PCR product was identified for each
of RED, RElSl and RET43 when PCR proceeded for 24 cycles (Figure 4.4).
In our initial analyses, we chose to investigate relative expression levels of RET 3'
alternatively spliced transcripts in five human kidney RNA samples that spanned the range
of gestational ages available (75, 14, 18 and 24 weeks) as well as adult kidney.
Quantitation of RET5 1 relative to during human kidney development was performed
at 24 cycles of PCR. RET43 expression was not detected at quantifmble levels in the
human kidney samples (4% of expression levels). Thus, RET43 expression was
not considered huther in these analyses. For each of these kidney samples, the reliability of
PCR conditions for quantitation was confirmed by establishing a hear relationship
between input cDNA and PCR product. Two-fold serial dilutions of sample cDNA were
amplified for 24 cycles of PCR. The expression of RETS l relative to RED was assessed
by comparison of incorporated counts, where RET5 1 product was expressed as a fraction
of product flable 4.1). Semiquantitative assays were repeated five times for each of
7.5, 14, 18 and 24 week human fetal kidney samples as well as for human adult kidney
and mean expression with standard deviation calculated. No signiticant differences in the
relative expression level of RET5 1 to R E D were observed for the 14, 18 and 24 weeks
gestation samples and these did not vary greatly from the relative levels observed in adult
kidney (Table 4.1). In a l l cases, RET51 expression was approximately 114 to 1/3 that of
RE79 expression. Interestingly, our analyses did not detect appreciable expression of the
RE25 1 transcript in the 7.5 weeks gestation kidney sample (Table 4.1).
We next broadened these analyses to examine the expression of RETS 1 relative to
RED in fetal kidney samples spanning 7.5-14 weeks gestation using the same semi-
quantitative RT-PCR analysis. Expression of RET5 1 was found to be comparable in 7.5
and 8.5 week human fetal kidney samples at 5&3% and 6&5% that of RE29 respectively
(Table 4.1, Figure 4.5). However, by 9 weeks gestation, the expression level of REn 1
had increased seven-fold to 35&8% that of RE29 (Table 4.1, F i g w 4.5). Our &ta suggest
Table 4.1. RE151 expression relative to RE29 expression in human fetal kidney.
Quatitation of the RET 3' alternatively spliced coding variants during human kidney
development based on semiquantitative multiplex RT-PCR analyses. RETS 1 expression
levels are given as a fiaction of RElP expression levels. RE79 expmssion levels have been
normalized to 1.00 in all samples. Means and standard deviations of five repeats are given.
Sample RElP Meanksd
7.5 week 1.00 0.05+0.03 8.5 week L .OO 0.06&0.05 9 week 1.00 0.35&0.03
10.5 week 1.00 0.2m.04 12 week 1.00 0.3w.08
14 week 1.00 0.36+0.06 18 week 1 .OO 0.32+0.05
24 week 1.00 0.3 1+0.04
adult 1 .OO 0.2m.04
Figure 4.5 Developmental expression of RET 3' coding variants in human fetal kidney.
Expression levels of RETSl transcripts relative to RET9 transcripts amplified in the same
mulitplex RT-PCR reaction are given for each sample. Quantitation was performed as
described in text. Mean values and standard deviations shown in Table 4.1 are plotted.
Age of Fetal Kidney (weeks)
developmental regulation of expression of the RE15 1 M p t over the 7.5-24 week
period in the human fetal kidney. Further, we have shown that RE751 is expressed at very
low levels early in gestation but represents approximately 114 of RET transcripts by 10.5
weeks gestation in the human kidney.
Discussion
The human kidney is fairIy well-defined by 8 weeks gestation and begins to
function by 11 weeks gestation (reviewed in 37). We have shown that RET expression is
higher at earlier stages of kidney development (7.5 weeks gestation) relative to later stages
(14-24 weeks gestation). RET expression levels were shown to decrease with increasing
fetal age through to 24 weeks gestation 18. In this study, we have shown that the three RET
3' coding variants, R E D , RETSl and RET43, are expressed during human kidney
development in samples ranging in gestational age from 7.5 through 24 weeks as well as in
adult kidney. However, we observed that RETS1 expression is very low in the earliest
gestational ages (7.5-8.5 weeks) relative to R E D expression in the same samples. While
we did not detect significant RETS1 expression in the 7.5 and 8.5 week fetal kidney
samples, a considerable increase in RE75 1 expression was observed by 9 weeks gestation,
the next available age of human fetal kidney, in all later gestational ages examined (9
through 24 weeks) and in adult kidney (Tables 4.1 and 4. 2). The absence of R E T S 1
expression until approximately 9 weeks gestation in human kidney raises the possibility
that RETSl has a role in kidney development distinct from those of RET9 and RET43. By
8 weeks gestation, the permanent kidneys have taken on a recognizable form and 3-5
branchings of the ureteric bud have occurred (reviewed in 37). The renal pelvis and the
major and minor calyces, ail of which are products of the ureteric bud, begin to take shape
by 10 weeks gestation around the time we see initiation of RETSl expression. Our data
indicate that the absence of RETS 1 expression during the early inductive events in the
human kidney is followed by a notable increase in RET51 expression by the time early
differentia~g events begin.
There are considerable data in the Literature suggesting that the functions of the
RET9 and RETS1 isoforms are not totally redundant. Atti6 et al. lo* have identified a
missense mutation in exon 20 which is, thus, present in the RET51 isoform but not in the
other RET 3' coding variants in a patient with HSCR. As described in chapter 1, HSCR is
a congenital abnormality characterized by the absence of sympathetic neurons in the
hindgut Inac t i v a ~ g RET mutations are identified as the underlying cause of 1040% of al l
HSCR cases 97. Thus, RET51 appears to be required for the induction of the myenteric
nerve plexus but not for kidney induction. Consistent with this phenotype, Rossel et al.
identified more prominent neurite outgrowth in PC12 cells transfected with activated
RETSI compared to activated RET9 although both isoforms induced some degree of
neurite differentiation 55. Taken together, these data might suggest that RETS1 may
activate downstream differentiation pathways in addition to or perhaps in preference to
mitogenic pathways.
The RETS1 isoform contains two additional tyrosine residues not present in the
RET9 or RET43 isoform (Y1090 and Y1096) 9. Y1096 has been identified as an
autophosphorylation site in RET 136. Direct binding between the Grb2-SH2 interaction
domain and the at pY 10% of RET5 1 has now been demonstrated 56. W three isoforms
include the tyrosine residue at 1062 which can be autophosphorylated on RET activation.
Splicing and sequence divergence at amino acid residue 1063 places this tyrosine in three
different binding contexts in the 3' RET isoforms 9. AU three sites share a consensus
sequence for interaction with the Shc-PTB domain (Figure 4.1) 13'. PreIiminary studies
have identified differences in the abilities of RET9 and RETS1 to interact with the Shc-PTB
domain at Y1062 57 (M. Billaud, personal commUtLication). In comparison to RET9, the
stronger binding of RETSI to the Shc-PTB domain is probably due to a higher affinity of
Y1062 for Shc-PTB in the sequence context of RETSL. Y1062 has been found to be a
major Shc-SII2 domain interaction site in RET9 while RETSl has distinct Shc-SH2 and
PTB interaction sites 56.
The differences between RET9 and Rl3"SI affinities for Grb2-SH2 and Shc-SH2
and -PTB interaction domains suggest that these two RET isoforms may differ with respect
to their downstream signaling pathways. Thus, the expression of these two isoforms could
modulate the relative activation of these pathways. We have shown that the RET 5 '
alternatively spliced transcript, RERI6, has highest expression early in human kidney
development (8 weeks gestation) and decreases through to 24 weeks gestation 18. We
suggested that RET may have varying roles or significance at different stages of kidney
development affected by differences in expression of the various RET 5' altemativeiy
spliced forms. The data described in this chapter may also suggest that the RET 3'
alternatively spliced variants affect kidney morphogenic processes. The dramatic increase in
the relative expression of RETS 1 compared to RE19 and RET43 between 8.5 and 9 weeks
gestation in the human kidney implicates a role for RET51 in human kidney development
that is distinct from either that of RET9 or RET43 (Table 4.1, Figure 4.5).
Materials and Methods
Fetal Kidney. Adult Kidney and IT RNA Analyses
The RNA extraction methods used are described in Chapter 3. Primer sequences
used in these analyses are given in Chapter 2. One l g of total RNA was heated at 7 0 0 ~ for
5 minutes and briefly cooled on ice. First strand cDNA was synthesized by incubating
RNA templates and PCR amplification performed under conditions descriid in Chapter 3.
Initial amplification analyses to identify expression of the individual RET 3' altemativeiy
spliced variants were performed using 1 min at 950C I 1 min at 550Cll min at 72OC 1 min
for 40 cycles followed by a final extension of 72% for 10 minutes.
Semi-Quantitative RT-PCR
RT-PCR experiments were performed in LOW volumes using the RT-PCR
conditions described but including 0. lpM 32Pend-labeled sense strand primer. To amplify
the three RET 3' alternatively spliced coding variants in a single multiplex PCR reaction,
1p.M each of NT forward primer (CRT14B) and reverse primers (KRT14D, KRT2OA and
KRT3B) was used Analyses to determine the linear range of amplification were performed
using 1/10 of a cDNA reaction, described above, in PCR for 16, 20, 24, 28, 32, 36 or 40
cycles. PCR products were separated and visualized on ethidium bromide-stained 2%
agarose gels and appropriate bands were excised. Quantitation of PCR products was
performed by Liquid scintillation of incorporated radioactivity. Plots of incorporated counts
(cpm) versus cycle number were used to define the range of PCR cycle numbers for which
amplification was linear (Figure 4.4). Two-fold serial dilutions of cDNA were subjected to
cycles of PCR within the Linear range to co&m the number of cycles for which primers
would amplify with similar efficiencies regardless of amount of starting template (Figure
4.4). PCR products were quantitated as described above. If the relationship of cpm versus
dilution factor was hear, the conditions were considered reliable for quantitation purposes.
Based on the preliminary experiments, 24 cycles of PCR was selected for semiquantitative
RT-PCR analysis of RET 3' alternatively spliced transcript expression in human fetal and
adult kidney RNA samples.
Chapter 5
Expression of genes encoding the RET ligand complex components GDNF and GDNFR-a daring human kidney development
I performed all the analyses of GDNF and GDWR-a expression in human kidney.
Introduction
Mammalian kidney development quires a series of reciprocal inductive
interactions between two distinct cell types, the ureteric bud epithelium and rnetanephric
mesenchyme 35. Induction is followed by the development of tubular epithelium from the
mesenchyme and the proliferation and branching of the ureteric bud. Roles for glial cell
linederived neurotrophic factor (GDNF) and RET. its receptor. in them events are
suggested by the phenotypes of the knockout mice, both of which display renal
dysmorphology characterized by retarded growth and reduced branching of the ureteric bud
as well as large areas of undifferentiated mesenchyme (described in Chapter 1) 34* 46-48.
GDNF receptor-a (GDMR-a), a cell surface protein, is required to mediate high affinity
binding of GDNF to RET 21.22- 33.
GDNF is a distant relative of the transforming growth factor (TGF)-P superfamily
based on the presence of seven conserved cysteine residues spaced identically in nerve
growth factor, plateletderived growth factor and TGF-f3 23. Human GDNF consists of
two exons and encodes a 211 amino acid pmtein precursor- Mature GDNF forms
glycosylated, disulfide-linked hornodimers to impart biological activity 24. The use of an
alternative splice site at nucleotide (nt) 69 of the human GDNF cDNA sequence results in
the deletion of 78 at corresponding to nt 70-148 (amino acids 24-50} and leads to a shorter
GDNF mRNA 239 26-27. The protein sequence deleted as a result of alternative splicing is
in the preprotein sequence and is not predicted to Sect the amino acid sequence of the
mature GDNF protein. GDNF is highly expressed in the gut prior to innervation by the
neural crestderived enteric neuroblasts and in the undifferentiated metanephric
mesenchymal cells in the nephrogenic zone of the developing kidney 20v 29. The phenotype
of GDNF -/- mice, which includes complete rend agenesis, characterized by lack of
ureteric bud or failure of the bud to grow and invade the rnetanephric mesenchyme,
suggests that GDNF plays a role in kidney induction 4&48. There are striking similarities
between the phenotypes of the GDW-/- and REW- mice. Not only do these mice have
similar degrees of renal dysplasia, they also both lack entenc neurons 34* 464%
The expression of RFT at the cell surface is not sufficient for high m t y binding
of GDNF 19-22. Binding assays have indicated a requirement for GDNFR-a in GDNF
binding to RET 21. 22. GDNFR-a, a novel GPI-linked protein, was originally isolated
from expression libraries prepared from mRNA isolated from retinal cell cultures enriched
for photoreceptors and rat embryonic midbrain enriched for GDNF-responsive
dopaminergic neurons 21- 22. Northern analyses have shown high levels of GDNFR-a
expression in embryonic kidney and intestine, sites of RET and GDNF expression 21- 227
33. Low levels of GDNFR-a expression have been detected in fetal brain, lung and other
components of the central and peripheral nervous systems.
We have shown that RET expression levels are highest during early human kidney
development then decrease with increasing embryonic age (described in Chapter 3) 18. In
this study, we examined expression of the genes encoding the RET ligand complex
components, GDNF and GDNFR-a, in developing human kidney using RT-PCR analyses
similar to those described in Chapters 3 and 4. In each of our fetal kidney samples. we
detected GDNF as well as GDNFR-a expression. Using a semiquantitative RT-PCR
analysis, we observed developmentally regulated expression of GDNFR-a in fetal kidney.
Our data is consistent with a role for REWGDNFI GDNFR-a signaling in human kidney
morphogenesis.
Results
Expression of GDNF in Human Fetal K idnq
We examined the expression of GDM; in a p a d of RNAs prepared from human
fetai kidneys ranging in gestational age b m 75 through 24 weeks as well as in adult
kidney. RNA from a Wi' tumour found to express GDNF at high levels (discussed in
Chapter 6) was used as a positive control. As described in Chapter 3, RT-PCR analyses
with a primer pair selected to amplify across the exodmtmn boundary were used to
investigate GDNF expression. A primer pair was selected that would amplify both full
length GDNF and the alternative splicing v&ant in a single reaction. PCR products were
electrophoresed on ethidium bromide-stained 2% agarose gels. We identified two predicted
products of 448 bp and 370 bp, corresponding to full length and alternatively spliced
GDNF, respectively, in all ages of human fetal kidney examined and in adult kidney
(Figure 5.1). Based on the intensities of the GDNF PCR products relative to one another,
expression appeared to be stronger between 8.5 and 12 weeks gestation compared to other
ages. RT-PCR was performed using GUSB-specific primers described in Chapter 2 to
determine if the differences we observed were due to variability in RNA integrity. The
intensities of the GUSB products were similar in all samples indicating minimal variability
in integrity across samples (Figure 5.1).
Erpression of GDNFR-a During Human Kidney Development
We used RT-PCR to investigate the expression of GDNFR-a in human kidney
development. PCR was performed using RAN0 and R A W primers, designed to amplify
products that crossed an exodintron boundary, to amplify a GDNFR-a product of 208 bp.
RT-PCR was performed on our panel of human fetal kidney RNAs ranging in age from 7.5
through 24 weeks as well as adult kidney. RNA extracted from a medullary thyroid
carcinoma cell line, TT, treated with retinoic acid (RA) for 24 hours was used as a positive
control (TT+RA). GRNFR-a expression was not detected in RNA samples fkom untreated
Figure 5.1. Expression of GDNF and GDNFR-a in human fetal and adult kidney. RT-
PCR analyses were used to detect GDNF and GDNFR-a expression in developing human
kidney. Similar analyses were used to detect GUSB expression in these samples as an
indicator of sample integrity. Rimer pairs used in these analyses are described in Chapter
2. The sizes of the predicted amplification products are indicated Gestational age of the
kidney sample is given in weeks (wk). A] GDNF expression, B] GDNFR-a expression
and C] GUSB expression. Positive (we) and negative control reactions are indicated (-ve).
'IT cells (data not shown). PCR products were electmphoresed and visualized on ethidium
bromide-stained 2% agarose gels. We identifled amplicons of the predicted size
comsponding to GDNFR-a throughout our panel of human fetal kidneys as well as in
adult kidney (Figure 5.1).
Quantitation of GDNFR-a in Hwnan Fetal Kidney
To investigate the reiative expression levels of GDATFR-a duriag the various stages
of human -kidney development, we used a semiquantitative RT-PCR assay to compare
expression levels of GDNFR-a to those of a housekeeping gene, P-glucuronidase
(GUSB). In order to avoid variations that might arise due to inter-sample differences in
RNA quality, we determined GDNFR-a expression relative to GUSB expression within a
sample. In addition to a 208 bp GDNFR-a product, a 195 bp GUSB product was
amplified in the reactions. A 5: 1 molar ratio of GDNFR-a primers to GUSB priwrs was
used to obtain similar amplitication of both products. To determine PCR conditions that
would be reliable for quantitation of products, preliminary experiments similar to those
described in Chapters 3 and 4 were conducted Template cDNAs were amplified over
increasing cycles of PCR, products were electrophoresed on 2% agarose gels and
appropriate bands excised. Incorporated counts (cpm), representative of the amount of
amplified product, were measured using liquid scintillation. After determiaing that
amplification proceeded Linearly between 20 and 26 cycles of PCR (Figure 5.2).
amplification efficiencies were confirmed using a two-fold serial dilution of TT+RA cDNA
for 22, 24 or 26 cycles as described previously in Chapters 3 and 4. At 24 cycles of
amplification. a linear relationship between input cDNA and amount of PCR product was
identified for each of GUSB and GDNFR-a (Figure 5.2).
We investigated GDNFR-a expression in RNA exuacted from human fetal kidneys
aged 7.5, 12.5, 14, 18 and 24 weeks, spanning the range of gestational ages available, as
well as in adult kidney. The reliability of conditions established for our control cell h e was
Figure 5.2. Determination of conditions for semiquantitative RT-PCR analysis of
GDNFR-a expression. A] Kinetics of simultaneous a~~~~lif?cation of GDNFR-a and
GUSB. Amounts of G M R a and GUSB product amplified in a singe muitiplex reaction
were quantitated by liquid scintillation counting of incorporated radioactivity. Counts
(measured in cpm) are plotted relative to the number of amplification cycles. The
exponential reaction was linear between 20 and 26 cycles. At 26 cycles, rates of
amplification for both GDNFR-a and GUSB decreased and approached piateau. B]
Confirmation of amplification efficiencies of G D N F R a and GUSB primers used in
multiplex PCR for semiquantitative analyses of GDNFR-a expression. A two-fold serial
dilution of rrtinoic acid-treated TI' (TT+RA) cDNA was subjected to 22,24 or 26 cycles of
PCR. The results for 24 cycles are shown. Linear results were obtained when counts were
plotted relative to dilution factor for amplification of both GDNFRa and GVSB transcripts
indicating comparable amplification efficiencies for these primer pairs.
GUSB GDNFR-a
Number of PCR Cycles
GDNFR-a GUSB
0 1 2 3 4 5 Two-Fold Serial Dilution Factor
confkmed for each human kidney sample by subjecting two-fold serial dilutions of cDNA
to 24 cycles of PCR A linear relationship between input cDNA and amount of PCR
product, determined by liquid scintillation of incorporated counts, coafirmed equivalent
amplification efficiencies for GDNFR-a and GUSB in each kidney sample.
Comparison of incorporated counts was used to assess GDNFR-a expression
levels relative to those of GUSB. The amount of GDNFR-a product was expressed as a
fraction of the amount of GUSB product. M e w of five repeats of the assay are given in
Table 5.1 with calculated standard deviations. We found that GDNFR-a expression levels
were relatively high in human fetal kidney aged 7.5 through 14 weeks compared to later
gestational ages. Expression leveis were approximately 2-fold lower in the 24 week feral
kidney sample compared to earlier ages (Table 5.1. Figure 5.3). Expression levels in adult
kidney were approximately 3-fold lower than those observed for early ages of fetal kidney
(Table 5.1, Figure 5.3). Our data suggest that GRNFR-a expression decreases during later
stages of human kidney development.
Discussion
In this study, RT-PCR analyses were used to investigate GDNF and GDNFR-a
expression in human kidney development. We observed expression of both mRNAs in the
earliest gestational ages available to us (7.5 weeks) through to 24 weeks gestation as well
as in adult kidney. GDNF expression appeared to be reduced in the adult kidney relative to
expression in the early gestational ages. Our data are consistent with reports of GDNF and
GDNFR-a expression in rodents 2 2 27-29. GDNF expression has been found to be lower
in the adult relative to embryonic and neonatal rodent kidneys 2*. In rodents, GDNFR-a
expression in the developing kidney has not yet been directly compared with expression in
the adult kidney. However, high levels of GDNFR-a in the adult kidney relative to
expression levels in other organs have been described 21.
Table 5.1. Expression of GDNFRa in developing human kidney. GUSB expression
levels have ken normalized to 1.00 for a l l samples. GDM;R-a expression levels are given
as fractions of GUSB expression levels amplified in the same reaction. Means of five
repeats and calculated standard deviations are given.
Sampie Meanksd
7.5 weeks 1.1 1a.02
12.5 weeks 0.9 lH.03
14 weeks 0.9 1H.20
18 weeks 0.82H.23
24 weeks 0.49M -04
adult 0.3&0.06
Figure 5.3 Developmental expression of GDNFR-a in human fetal and adult kidney. Semi-
quantitative RT-PCR was used to investigate GDNFR-a expression levels. Ratios of
GDNFR-a expression to GUSB expression within a sample are given for fetal kidney
samples ranging in gestational age fiom 7.5 through 24 weeks. Points plotted on the graph
are the means of five individual assays. Error bars for each sample represent calculated
standard deviations.
6 8 1-0 12 14 16 18 20 22 24 26 Gestational Age of Kidney (weeks)
In Chapter 3, we reported developmental regulation of RET expression in human
fetal kidney '8. Here, we show that GDNFR-a also undergoes developmental regulation
over the same period. Our data show that GDNFR-a expression levels are relatively higher
in the early gestational ages (7.5- 14 weeks) then decrease through to 24 weeks gestation in
human kidney. The Lowest levels of GDNFR-a expression were detected in adult kidney.
GDMR-a has been shown to mediate the association of GDNF with RET 21. 22. 33.
Tremor et al. 22 suggest that a disulfide-linked GDNF dirner bound to one or two
molecules of GDNFR-a forms a complex which subsequently binds to and activates RET
(Figure 1.4). In the absence of GDNFR-a expression, GDNF is unable to induce
autophosphorylation of RET 21- 22. In vino assays have shown that overexpression of
GDM;R-a greatly increases GDNF binding to RET and, hence, RET autophosphorylation
21- 22. Given that GDNFR-a expression levels modulate GDNF binding to RET, the
higher GDNFR-a expression in early ages of human fetal kidney relative to expression in
adult kidney which we observed is consistent with GDNFR-a expression as a means of
regulating RET activity during kidney development.
Another means of regulating RET activity would be through receptor binding to
alternative ligand components. The multiple GDNF and GDNFR-a family members
identified to date are potential modulators of RET activity. Recently, Sanicola et aL 33
reported the isolation of RETL2 from a rat embryonic kidney cDNA Library. The RETL.2
protein shares 4 9 1 homology to rat GDNFR-a but, unlike GDNFR-a, is capable of
binding GDNF only in the presence of RET. GDNFR-a and R E Z E are expressed in a
wide variety of embryonic and adult tissues including kidney. This raises the possibility
m y or all of these molecules affect RET activity. Sanicola et al. 33 have proposed that the
dissociation of the REWGDNF/RET complex would release GDNF from the cell surface
while dissociation of the GDNFR-or/GDNF/RET complex would retain GDNF bound to
GDNFR-a. In this scenario, RETL2-expressing cells might display greater sensitivity to
changing local concentrations of GDNF than those expressing only RETLZ. Neurmrin has
been identified as a relative of GDNF 31. The protein shares 42% homology with the
mature GDNF protein. Similar to GDNF. neurturin is expressed in a wide range of
neonatal and adult tissues including brain and kidney. The ability to promote survival in
neuronal populations, which neurturin shares with GDNF, suggests that the two proteins
are capable of acting through common signaling pathways 31. However, whether neurturin
is able to interact with RET has not yet been investigated.
High levels of GDNF expression have been observed in embryonic rat kidney 2'-
29. GDNF expression in the developing kidney decreases after embryonic day 16 and
significantly lower levels of GDNF expression are detected in the postnatal kidney 2'- 28.
No expression was detected in the adult kidney 27v 28. I . humans. we have shown that
GDNF expression occurs throughout the various stages of kidney development. Lower
levels of expression in the adult kidney are suggested by the intensity of the PCR product.
Thus, a similar developmental tread in GDNF expression in the developing kidneys of
rodents and humans is suggested, however, quantitative analysis of GDNF expression in
the developing human kidney is required.
The expression of genes encoding the fust two identified RET ligand complex
components. GDNF and GDNFR-a, in human kidney development is consistent with a
role for the RET signaling complex during kidney morphogenesis. We have identified a
downward trend in GDNFRa expression with increasing fetal age in the human kidney.
The developmental pattern of GDNFR-a expression in the kidney might act as a
mechanism for regulatory control of RET activation during development in this organ.
Materials and Methods
Reverse-Trc~nscnption- Polymerase Chain Reachon Analyses
RNA was extracted using the methods described in Chapter 3. Primers sequences
used in RT-PCR analyses are given in Chapter 2. One pg of total RNA was heated to 70oC
for 5 minutes and briefly cooled on ice. First strand cDNA was synthesized by incubating
RNA templates under conditions descn'bed in Chapter 3. PCR amplification of cDNA
templates was performed in lOmM Tris-HCl (pH 8.3), 50mM KCI, 0.01% gelatin, 2 0 w
d N T P s , lpM each primer, 1.5 units Taq DNA polymerase (Gibco-BRL Life Technolo@es)
and 0.75m.M MgC12 for ampiification of GDNF products or 1.5m.M MgC12 for
amplification of GDNFR-a products. The PCR cycling conditions used are described in
Chapter 3.
Semi-Quantitative RT-PCR
RT-PCR experiments were performed in 10p.L volumes using the RT-PCR
conditions described but including O.1p.M 32~end-labeled sense strand primer. Optimal
conditions for co-amplification of GDNFR-a and GUSB in a single multiplex PCR
reaction consisted of LpM of each GDNFR-a primer and 0.2pM of each GUSB primer.
The hear range of amplification was determined as described in Chapters 3 and 4. Two-
fold serial dilutions of cDNA were subjected to cycles within the linear range to confirm the
number of cycles for which primers would amplify with similar efficiencies regardless of
amount of starting template. PCR products were quantitated as described above. If the
relationship of cpm versus dilution factor was hear, the conditions were considered
reliable for quaatitation purposes. Based on the preliminary experiments, 24 cycles of PCR
was selected for semiquantitative RT-PCR analysis of G D N F R a expression in human
fetal and adult kidney RNA samples.
Chapter 6
Analyses of RPT, GDNF and GDNFR-a Expression in Human Disease
I performed all analyses of RET, GDNF and GDNFR-(x expression in Wilms' tumours and rend cell carcinomas. The d t s of G D W mutation screening in Hirschsprung disease appear in Human Molecular Genetics 5:2023-2026 (1996) and are the result of a collaborative effort with Ms. Shirley Myers. Sequencing analyses of GDNF were performed equally by Ms. Myers and myself.
Introduction
The E T proto-oncogene encodes a receptor tyrosine kinase required for enteric
neurogewsis and kidney development 9- 349 40. Expression of RET is restricted both
spatially and temporally in the developing nervous and excretory systems, suggesting a role
for this receptor in the regulation of proliferation and/or differentiation during development
11* 14-169 18. RET's involvement in tumourigenesis and in developmental anomalies has
been well documented. RET is rearranged and constitutively activated in a proportion of
papillary thyroid carcinomas 78-82. Germline point mutations of RET are associated with
the majority of multiple endocrine neoplasia types 2A and 2B and familial meduliary
thyroid carcinoma, all of which are dominantly inherited cancer syndromes characterized by
multiple tumours of neuroectodermal origin (reviewed in 88). These mutations convert
RET into an activated oncogene 87. Mutations in RET have also been described in 1040%
of cases of HSCR, a congenital abnormality characterized by aganglionosis of the lower
gut 989 102- 10% los- 106. It has been shown that RET mutations associated with HSCR are
inactivating and result in abrogation of biological activity of the receptor 9 9 ~ 1 3 ~ .
Recently, a ligand for RET has been identified as a multicomponent complex
consisting of GDNF and GDNFR-a 21- 22. 33. While GDM is a soluble molecule,
GDNFR-a is a GPI-Linked cell surface protein. GDNF is not sufficient for high affiaity
binding to RET aud has a requirement for GDNFR-a. The pattem of GDNF expression
during development of the nervous and excretory systems is similar to that of RET 14* 159
27.29. Further, the phenotypes of the GDNF -/-and RET-/- mice are similar including renal
dysplasia and lack of enteric neurons 349 46-48. These observations suggest that
disturbances in any pan of the RET activation complex may have similar consequences.
Phenotype associations have previously been reported for mutations in c-KTr and Steel
factor (SLF), genes encoding a complementary receptodgrowth fanor system (reviewed in
139).
Reciprmal inductive interactions between ureteric bud epithelia and metanepbric
mesenchyme are required to signal cell proliferation aud differentiation in the developing
kidney 3? It has bem suggested that defccts in mechanisms which halt cell proLiferatiou
and/or induce mesodefmal differentiation can result in Wilms' turnour m, the most
common paediatric solid -our of the kidney and one of the most common solid tumours
of childhood (reviewed in 140-143). The majority of WTs are sporadic although 1% of
cases are familial (reviewed in 143). Histological analysis of WTs have indicated a
resemblance to inappropriate development Turnours may be triphasic containing compact
areas of blastema, more differentiated epithelial components and/or saomal elements. One
of these elements often predominates '44. WTs are believed to be derived from cells of the
MM that normally differentiate into the epithelial components of the nephron (reviewed in
141-143).
The molecular genetics of WT ae complex. however, three genes have been
implicated in tumourigenesis. 3040% of sporadic twnours are associated with loss of
heterorygosity (LOH) on chromosome 1 1 p 145. Mutations inactivating WT- 1, which has
been mapped to 1 lp 13, have been identified in a subset of cases with genetic susceptibility
to WT and in 1045% of sporadic tumows t46-148. One-third of WTs display LOH
restricted to 1 lpl5.5 14% 150. This same chromosomal region has been implicated in
Beckwith-Wiedemann syndrome (B WS), a congenital disorder characterized by generalized
overgrowth and an increased risk of childhood tumours including Wilms' tumour l49-151.
A BWS gene wodd be expected to impact on WT development Recently, mutations in
p57kip2, an imprinted gene that maps to chromosome 1 lp 15.5. have been identified in a
subset of BWS patients L52. Expression of pS7kip2 is reduced in WTs. however, p 5 7 W
has not been investigated for mutations in WT 152. A familial \KT predisposition gene,
FWTI, has been lccaiized to chromosome 17q12-21 153. Several candidate genes are
located in this interval including neurofibomatosis-l (IVF-I) and insulin-like growth factor
binding protein (IGFBP)-4, however, the gene associated with this phenotype has yet to be
defined 154.
Rend cell carcinoma (RCC) is the most commoa malignancy of adult kidney and
accounts for 2 8 of al l cancers (reviewed in 155). Most cases of RCC are sporadic,
however, rare familial forms are characterized by autosod dominant inheritance, young
age at diagnosis and bilateral and multifocal turnours. Von Hippel-Lindau (m) disease is
an inherited cancer syndrome charactexkd by high incidence of RCC (reviewed in 156).
The VHL gene lies at 3~25-26 157. Chromosome 3p a b n o d t i e s including
rearrangements and LOH are the most common occurrence and are amongst the earliest
abnormalities identitied in both sporadic RCC and MIL-associated renal turnours t58-160.
Frequent point mutations or transcriptional inactivation through hypermethylation of the
remaining VHL dele are found in RCC resulting in tumourigenesis l61- 162. Other
chromosomal abnormalities associated with RCC include LOH at chromosomes 6q, tip, 9,
LOq and 14q 158. 161-1% These are likely to represent secondary events in -our
progression 1%
Ultrasmcturd and cell surface protein expression studies suggest that RCC derives
from proximal tubule epithelium of the renal cortex (reviewed in 155). During
organogenesis, these cells, as well as giomerular and distal convoluted tubule epithelial
cells, originate from the MM, a cell mass that proliferates and differentiates in response to
signals h m the ureteric bud 35. Continued proliferation of the MM and its early derivatives
is dependent upon induction. This may suggest that disruption of genes with roles in the
promotion of proliferation or in induction could contribute to RCC.
Rcviously, we investigated the expression of RET during human kidney
morphogenesis l8 (described in Chapter 3). In this study, we examined RET expression as
well as expression of GDNF and GDNFR-a in a series of renal tumoun. RET expression
was detected in each WT but GDNF and GDNFR-a were not. In contrast, RET and
GDNFRa expression were detected in each RCC sample and GDNI; expression was
always absent.
We also investigated HSCR patients for mutations in GDNF. Our analysis revealed
a de novo mutation in one HSCR patient suggesting that GDNF mutations may conmbute
to the HSCR phenotype.
Results
Expression of RET, GDNF and GDNFR-a in Wilms' Tumour
We investigated RET' G D and GDNTRa expression in a panel of six WTs and
one WT cell line. DW2. Three tumour samples were obtained from primary tunours
(WT20, WT21, W 6 3 ) (Tabie 6.1). The remaining three tumour samples were obtained
from mouse xenografts of primary WTs (WT26, WT27A. WT19) flable 6.1) lu. AU
tumours in our panel were sporadic and had favourable histology according to Beckwith's
criteria 14'? Histological analyses identified the tumours in the panel as predominantly
blasternal. predominantly epithelial differentiated, predominantly smrnal differentiated or
epithelial mixed (Table 6.1). RT-PCR analyses were performed on RNA extracted from the
tumour samples and from DW2 cells using primer pain designed to cross an exodintron
boundary. Using RET-specific primers CRT4S and CRT4B, an amplicon of the predicted
size (187 bp) was detected in all six WTs and in the DW2 cell line (Figure 6.1). This result
was surprising given that the WT cell of origin is not predicted to express RET.
Investigation of GDNF and GDNFR-a expression in this WT panel was conducted
using RT-PCR analyses similar to those described in Chapter 5. The GDNF-specific
primers selected to amplify products that spanned an identified alternative splicing site were
GDXlF and GDN7R 26. 27. GDNF expression was not detected in one of six WTs
(WT27A) nor in the DW2 cell line (Figure 6.1). We detected two GDNF products of the
Table 6.1. Histology and RET, GDNF and GDNFR-a gene expression in Wilms' turnour.
AU tumours were classified as Wilms' tumours based on Beckwith criteria. Rimary
turnours and nude mouse xenografts are indicated Gene expression is indicated by + while
absence of gene expression is indicated by -. NA is used to denote lack of information.
WT Tumour Histol~gicai RET GDNF GDNFR-a Sam~le Source Classification Expression Expression Expression
WT20 primary stromal + + + differentiated
WT2 1 primary epithelial + + + differentiated
WT26 xenograft mixed + + + WT27A xenograft blasted + - + WT29 xenograft mixed + + + WT763 primary NA + + + DW2 cell line NA + - -
Figure 6.1 RET, GDNF and GDNFR-a expression in Wilms' turnour 0. PCR
amplification of cDNA templates was performed using primer pairs described in Chapter 2.
The predicted product size for each amplification is indicated A] RET expression.
B] GDNF expression and C] GDNFR-a expression. Positive (+ve) and negative (-ve)
controls are indicated.
RET
predicted sizes, 238 bp and 160 bp, in al l other samples including a 14 week human fetal
kidney RNA sample used as a positive control (Figure 6.1). There was no difference in the
level of expression of the two GDNF-specific PCR products nor in the ratio of expression
of the two products amongst samples.
RT-PCR analyses were also used to examine GDNFR-u expression in our panel of
tumours. Using GDNFR-a-specific primes, a product of the predicted size (208 bp) was
amplified in all six WTs and detected upon electrophoresis and visualization on agarose
gels (Figure 6.1). The intensities of detected PCR produfts appeared to be equivalent
across these samples. In comparison, a barely detectable GDNFR-a-specific PCR product
was amplified in the DW2 cell Line which was previously shown to express RET but not
GDNF (Table 6.1, Figure 6. L).
Expression of RET. GDNF and GDNFR-a in Renal Cell Carcinoma
In order to address the possibility of RET involvement in adult onset renal turnours,
we investigated the expression of genes encoding the RET/GDNF/GDNFR-a complex
components in 11 cases of renal cell carcinoma (RCC) and in the corresponding normal
kidney tissues. Tumour and matched normal kidney cortex tissue samples were obtained
following nephrectomies performed at the Kingston General Hospital. Tumow samples
were dissected from the surgically removed kidneys taking care to minimize contaminating
nonnal tissue. We used the same RT-PCR strategies described above for examination of
RET and GDNFR-a expression in WTs to investigate expression of these transcripts in
RCC and matched normal kidney. GDXlF and GDX3R primers were used for GDNF
expression analyses in RCC. For al l analyses, human fetal kidney aged 12 weeks was used
as a positive control. Using RlT-specific primea CRT4S and CRT4B in PCR, the
predicted 187 bp product was detected in each normal kidney sample and in each of the I 1
RCC tumour samples (Table 6.2). The results from a subset of these tunours and matched
normal kidney samples are shown in Figure 6.2. In each case, the intensity of the PCR
Table 6.2. RET, GDNF and GDNFR-a expression in renal ceU carcinoma. RT-PCR analyses
were used to investigate gene expression in a series of 11 RCCs (TK) and matched normal kidney
samples (NK). Expression of GLISB, a low-level house-keeping gene. was used to confirm
sample integrity. +, H, ttc and ++++ are arbitmy units used to denote expression levels where
+ represents low levels and cm represents high levels of expression baxd on the intensity of the
PCR product. I indicates absence of expression.
RET GDNF GDNFR-a GUSB
Sample NK TK NK TK NK TK NK TK
Figure 6.2 RET, GDNF and GDNFR-a expression in renal cell carcinoma (RCC). PCR
ampiification of cDNA templates prepared from RCC C I X ) and matched normal kidney
cortex (NK) samples was performed using primer pain described in Chapter 2. The
predicted product size for each amplification is indicated A] RET expression. B] GDNF
expression, C] GDNFR-a expression and D] GUSB expression. Positive (+ve) and
negative (-ve) controls are indicated.
product was greater in the normal kidney compared to the tumour sample which may
suggest differences in RET expression between the two. The ecpivalent intensities of
GUSB PCR products generated from these same samples suggested that the differences in
intensity of the RETPCR products was not due to differences in RNA quality (Figure 6.2).
GDNF and GDNFR-a expression was examined in our RCC samples. PCR
analyses failed to detect GDNF expression throughout our panel of RCCs while expression
was observed for each matched normal kidney cortex sample (Table 6.2, Figure 6.2). We
detected relatively high GDNFRa expression in 1111 1 RCC and comparable expression
levels in the matched normal kidney samples (Table 2 Figure 6.2).
GLlNF Mutation Analysis in Hirschspmg Patients
We used direct genomic sequencing to analyze DNA from 16 sporadic and 20
familial cases of HSCR. PCR was used to amplify GDNF exons 1 and 2 in separate
reactions and the products purified. Complete sequencing of GDNF exon 1 did not identify
any sequence variants amongst our samples. However, two sequence variants were
identified within exon 2 of GDNF in two different HSCR patient samples. The first
sequence variant was identified in a patient with totai colonic aganplionosis associated with
a cytogeneticdy detectable deletion of 10q 11.2-21 -2 which spanned the RET locus 101.
Both parents were healthy and had normal karyotypes suggesting that the disease
phenotype was associated with the deletion. The GDNF sequence variation involved a G-
>A substitution at base pair 429 (exon 2) (data not shown). The change was predicted to
destroy an RraI restriction site in the GDNF sequence. This was confirmed by restriction
enzyme digestion of the amplified patient DNA (Figure 6.3). The substitution was not
detected in 35 other HSCR patients nor in 301 normal controls 16* (R. Hofstra, personal
communication). Since neither an amino acid change nor an alteration in splicing resulted
from this substitution, it most likely represents a very rare polymorphism.
Figure 6.3 GDNF mutation in a Hirschsprung (HSCR) patient. a) Sequence from GDNF
exon 2 in patient HS4-3 and a n o d control (N). HS4-3 is heterorygous for the n o d
(ACA) and mutant (TCA) sequence at codon 154. b) Restriction e v e digest analysis of
GDNF exon 2 PCR products with Hinff and HincII in family HS4. Digestion of the 478
bp product with Hinfl produces bands of 36 and 115 bp in the absence of the T154S
mutation. In the presence of the mutation, novel bands of 195 and 168 bp are generated by
cleavage of the 363 bp hgment. The 478 bp fragment is not digested by H i n d in the
absence of the mutation. When T154S is present, novel bands of 303 and 175 bp are
generated. A 100 bp DNA marker is indicated (M).
A C G T A C G T
H i n f I H i n c I I
The second change was detected in a patient with sporadic long segment HSCR and
no detectable mutations of RET or odw HSCR disease susceptibility loci. The sequence
variation was a substitution of an A for a T at base pair 460 in exon 2 (Figure 6.3). This
resulted in an amino acid change from threonine to serine at codon 154. The change was
not detected in 35 other HSCR patients nor in 301 normal controls 165 (Hofstra, personal
communication). Novel Hinfl and HincII restriction sites were predicted to result from the
substitution. The presence of these sites was confirmed upon digestion of amplified GDNF
products from the patient (Figure 6.3). The restriction e n y m cut sites were not detected in
either parent suggesting a de novo mutation of GDNF in the patient. Paternity was
coofirmed using three microsatellite markers h m chromosome LO. These data may
indicate a causative relationship between the GDNF mutation and the HSCR disease
phenotype in this individual.
Discussion
RET/GDNF/GDNFR-a in Wilms' Turnour
In this study, we investigated the expression of RET and the genes encoding
GDW and GDNFR-a, RET's recently identified ligand complex components, in a panel
of six WTs and one WT cell line, DW2. We found that REZ was expressed throughout our
p d of WTs and in the DW2 cell line. This result was intriguing given that WTs are
believed to originate from r e d blastemal cells, mesenchymal cells that give rise to
nephrons when induced by the ureteric bud 144. Normally, RET is not expressed in this
cell type 14- 349 40. While unlikely, it is possible that a small amount of contaminating
normal cells was responsible for the strong RET expression we detected in the primary
tumour samples. However, this answer cannot suffice for the mouse xenografied samples
where the possibility of contaminating normal human tissue is eliminated. Our results show
that RET expression becomes deregulated in WT cells. Whether this is a direct effkct of
transformation or a secondary effect of deregulation of other molecules is not known. Other
genes such as T M have been shown to be deregulated, presumabiy as a secondary event,
in Wilm's tumourigenesis 166. Like RET, TrkC is normally expressed in the ureteric bud
epithelium 167. 168. While TrkC expression is not detected in the minduced ureteric bud
nor in the uninduced blastema and differentiated structures derived fiom MM, its
expression is associated with more advanced stages of collecting duct differentiation in cells
derived f?om the ureteric bud epithelium 16% 16% TrM= mRNA and protein expression
have, nonetheless, been detected in WTs where expression has been localized to the
epithelial tubule elements '66. In this study, we were not able to determine whether RET
expression occurs in a i l WT cell types or is localized to subsets of cells with specific
histological features. However, we have shown that RET and 5' splicing variants of RET
are a l l strongly expressed in a panel of WTs with histologies ranging from predominantly
blastemal to predominantly stmmal-differentiated.
Four of the five tumours in our panel for which we have histological data are
predominantly composed of a population of cells with a differentiated phenotype (Tabie
6.1). A f~ turnour, WT27A, is described as predominantly blastemal. Interestingly, this
tumcur expresses both RET and GDNFR-a but not GDNF. Given that WTs arise from
MM cells, GDNF expression would be predicted in a l l WTs. Absence of GDNF
expression in WT27A must represent a loss of gene expression in these tumour cells.
Neither GDNF nor GDNFR-a expression was detected in the DW2 cell line which
expressed RET. No clear pattern of expression of the three components could be discerned
for WT. The existence of three genes that predispose to WT has been described and at least
a fourth is predicted (reviewed in 143). Given that mutations in any one of these genes can
result in a similar phenotype, it is possible that the different mutated genes affect an
overlapping set of transcriptional regulatory pathways thus explaining RET expression in
all turnours investigated but the absence of GDNF and GDNFR-a expression in select
WTs Is** 153- 16% The variable expression of RET, GDNF and GDNFR-a in WTs
may represent different t u m o ~ etiologies which result in expression and/or repression of
unique subsets of mRNAs.
Kidney development proceeds via interaction between two different cell types, the
ureteric bud epithelium, where RET is expressed, and the metanephric mesenchyme, where
GDNI; is expressed 14- 2% 35. In contrast, tumours arise from a single cell type. The
expression of each of RET, GDNF and GDNFR-a in subsets of WT indicates that these
genes are all expressed in the tumour cell of origin unlike the localization of expression in
kidney development Differences in the pattern of gene transcription between differentiated
WT structures and the equivalent structures in fetal kidney are not uncommon. For
example, there is not a point during kidney development when WT- 1, PAX-2 and PAX-8
are a l l expressed at high levels in the same cell type although al l are expressed in the
condensed mesenchyme and/or its derivatives in normal developing kidney 44- 171-
PAX-2 and PAX-8 are also expressed at low levels in the ureteric bud epithelium where
W7'-1 expression is absent. Once differentiation of the MM commences, PAY-2 and PAX-
8 transcription attenuates while WT-1 expression is upregulated rapidly s4. l72. However,
many WTs display elevated expression of both PAX-2 and PAX-8 in highly differentiated
epithelial structures 172 173. This observation is consistent with deregulation of PAX-2 and
PAX-8 expression in Wilms' tumourigenesis compared to the tight control of expression
during kidney development. Similarly, RET, GDNF and/or GDNFR-a expression may be
deregulated in W s resulting in expression in a cell type where the gene(s) is not normally
expressed It is equally possible that disruptions in WT genes are not only capable of
activating but also of repressing transcription of genes such as GDNF which are normally
expressed in the cell thus explaining absence of GDNF expression in WT27A.
RET, GDNF and GDNFR-a Expression in K C
RET expression was identitied in 1111 1 RCC and corresponding matched normal
kidney cortex samples. The expression levels in the tumours appeared to be slightly lower
than in the normal samples. The results of RT-PCR amplification of GUSB, a low-level
house-keeping gene, confirmed that this observation was not just a reflection of differences
in RNA quality between normal and tumour samp1es 6.2). GDNF expression was
only detected in the matched normal controls at very low levels. GDNFRa expression was
detected in all tumours and matched normal samples at relatively high Levels compared to
GDNF expression in these same samples.
The presumed cell of origin of RCC, proximal tubule epithelium, is a derivative of
the metanephric mesenchyme and might not be predicted to express RET or GDNF
(reviewed in 155 and 174). Normally, RET is expressed in ureteric bud epithelium and
derivatives while GDNF is expressed early in uninduced MM and early derivatives but not
in the more differentiated cell types derived from MM 14- 29. Studies delineating cell type-
specific expression of GDNFRa in the normal kidney show that it is normally expressed
at least in some of the same cells as RET, adjacent to GDNF-expressing cells 22. The
absence of relatively high expression levels of REI or GDNF in RCCs may simply be a
reflection of the tumour cell of origin which might not be expected to express either
transcript. In fact, RET expression levels in RCC samples appeared to be similar to
expression levels in the matched normal kidney tissues. This observation raises the
possibility that the trace expression we observed in tunour samples was due to the
presence of residual normal tissue contaminating the huwur sample.
Expression of GDNFR-a has been shown to be relatively high in the normal
kidney 21- 2 2 33. Given that localization of GDNFRa expression in the kidney appears to
mimic that of RET, co-expression of RET and GDNFR-a in the same cells is not
surprising. Their co-expression in RCC is, however, surprising given that the tumour cell
of origin is not predicted to express RET. It is possible that transcription of these genes is
affected by mutations in a gene predisposing for RCC. Analyses of sporadic RCCs have
revealed loss of one VHL dele in 95-9796 of turnours with kquent point mutations or
hypermethylation of the remaining allele 175-17? VHL is involved in the inhibition of gene
transcription and is ubiquitously expressed in the rnetanephric, ureteric and stromal
components of the developing kidney 178. There appear to be several factors that contribute
to the initiating or regulating events of VHL in normal organogenesis as well as in
pathogenesis. It is possible that any of these might also affkct RET and GDNFR-a
expression in these same cells causing them to be expressed when they are not n o d y
expressed.
Reports of GDNFR-a expression in cells that do not express RET, such as
Schwann cells, suggest that GDNFR-a expression in RCC might not be unexpected 22. In
sinc hybridization and immunocytochemical analyses indicate that GDNFR-a expression is
more widespread than RET expression in the developing kidney 22. This provides an
alternative explanation for the relatively high GDNFR-a expression levels we detected in
both RCC and matched normal kidneys compared to low levels of RET. We cannot rule out
the possibility that GDNFR-a has the capacity to interact with molecules other than GDNF
and RET and hence stimulate different downstream pathways that are involved in RCC
tumourigenesis.
The absence of GDNF expression in RCC most Likely reflects the tumour cell of
origin which is not normally predicted to express GDNF. Similar low levels of RET
expression were detected in both RCCs and matched n o d kidney samples. GDNFR-a
expression was relatively higher in both turnour and normal kidney samples compared to
RET expression. RET and GDNFR-a expression in these tumours may be the result of
disruption of regulatory pathways during the course of tumourigenesis.
GDNF Mutation Analysis m Hirschpmng Disease
We screened a panel of 36 sporadic HSCR patients for mutations in GDNF, a gene
that encodes one of the RET ligand complex members. Within our panel, we identified one
patient with a very rare polymorphism, a conservative substitution of G->A at GDNF base
pair 429. HSCR disease in this patient was previously found to be associated with a
deletion of chromosome l0q 1 1.2-2 1.2 which spanned the RET locus lo I . This same
polymorphism has been reported by R Hofstra in a patient with a familial form of HSCR
(personal communication).
There are reports in the literatwe of polyrnotphisms in a gene modulating
susceptibility to disease. For example, Creutzfeld-Mob disease (UD) occurs in both
sporadic and f e d forms 179- 180. Familial CTD is associated with the presence of
mutations in the pnon protein gene (PRNP). In addition to pathologic mutations of PRNP,
homozygosity at the site of a common poIymorphism at codon 129 is implicated in the
development of sporadic and infectious CJD The disease phenotype of familial
CJD is also modulated by this same polymorphism 182. Mutations in codon 178 of PRNP
can either result in fatal familial insomnia (FFI), a dementing illness. or familial CTD 183-
l86. The genotypic basis for the difference between FFI and CJD associated with this
PRNP mutation Lies in the codon 129 polymorphism IB7. Individuals with a mutation in
PRNP at codon 178 and homozygous for valine at codon 129 develop CJD whereas
individuals with the same mutation in codon 178 and homozygous for methionine at codon
129 develop FFI. In light of the fact that polymorphisms can affect disease phenotype. it is
possible that GDNF sequence variations such as the one we detected have bearing on the
expression or severity of the HSCR phenotype in patients with RET or other HSCR
mutations without being causative for the disease. It is, however, difficult to predict what
the effects of a sequence variation that does not lead to an amino acid change could be on
the GDM: protein.
In a second patient with sporadic long segment HSCR, we found a de novo
mutation of GDNF at base pair 460 resulting in substitution of s e ~ e for threonine. The de
now occurrence of the mutation was c o n w e d using restriction enzyme digests which
identified a cut site generated by the mutation in the patient but not in either parent. The fact
that both RET-I- and GDNF-I- mice displayed absence of enteric ganglia suggested that
inactivation of GDNF could result in a similar phenotype as RET inactivation 34- 46-48.
Thus, any gene encoding a member of the RET multicompouent Ligand complex could
represent a candidate gene for HSCR disease. Similar phenotypes are attniutable to
mutations in genes encoding either the c-KlT receptor or its corresponding ligand SLF
188. Interactions between the products of these genes influence various developmental
processes including survival, proliferation andor differentiation of germ cells, pigment
cells and hematopoietic cells (reviewed in 139). In the mouse, mutations at either the white-
sponing/c-KIT 189 or SLF 190 locus result in almost identical defects including dominant
white-sponing, sterility and severe macmcytic anemia (reviewed in 139). Mutations in
either c-KFT or SLF control the human piebald phenotype by resulting in a reduction in
tyrosine kinase activity and failure of mlawcytes to thrive and reach the skin during
embryogenesis 191- 192- It is possible that mutations in GDNF affect the HSCR phenotype
similar to mutations in RET. Whether or not mutations and/or polymorphisms in GDNFU-
a can also contribute to the HSCR phenotype remains to be established.
We and others have shown that the occurrence of GDNF mutations in HSCR
patients is very infrequent 165. 193. Angrist et al. 193 identified one familial GDNF
mutation in a HSCR patient with a known de novo RET mutation while Salomon a al. 165
identified mutations in patients with either RET mutations or trisomy 21, a chromosomal
anomaly known to predispose to HSCR disease. Their results suggested that GDNF
mutations were neither necessary nor sufficient for the genesis of the disease phenotype.
The de novo case of HSCR we report here is associated with a de novo mutation of GDNF
in the absence of any RET mutations or nisomy 2 1. In addition, the patient does not have
any other associated HSCR disease phenotypes such as deafness or pigmentary
abnormalities which might suggest the involvement of another known HSCR locus such as
EDN3 or EDNRB 98.1949 195. While the GDNF mutation we have identified in this patient
could be purely coincidental with the occurrence of HSCR, it is equally possible that the
TIS4S mutation has functional significance for GDNF. A better understanding of this
awaits analysis of the functional domains of GDNF.
The ligand for RET consists of a multicomponent complex which includes GDNF
and GDNFR-CY. The possibility exists that mutations in GDNFR-a can contribute to or are
responsible for the HSCR disease phenotype. It is equally possible that other RT3 ligand
complex members exist but have not yet been elucidated or that GDNF and GDNFR-a
family members exist that are also capable of interacting with REX Any of these might also
contriiute to the genesis of HSCR disease.
Miterids and Methods
Reverse Trunscription and Polymerase Chain Reaction Conditions
Total RNA was extracted h m RCC and matching normal tissues and fiom Wilms'
tumour samples and first strand cDNA synthesis was performed as described Chapter 3.
Sequences of primers used in PCR amplification of cDNA templates are given in Chapter
2. PCR was essentially as described in Chapter 3 with the exception of the MgClz
concentrations included in reactions. 1 SmM, 0.75mM, and 1 SmM concentrations of
MgQ were included in PCRs to amplify RET, GDNF and GDNFR-a sequences
respectively. PCR proceeded for 40 cycles of 950C for 1 min/550C for 1 W 2 0 C for 1
min. Cycling concluded with a final extension of 72% for 10 minutes.
Genomic Sequencing
DNA was extracted fiom peripheral blood using standard protocols 122.
Sequencing analyses were as described in Ivanchuk et al. l21.
Chapter 7
Discussion
RET in Hwnan Kidney Development
Proliferation and differentiation events are both required for maturation of the
human kidney. Inductive stimuli from the ureteric bud cause the rnetanephric mesenchyme
to proliferate and differentiate into nephrogenic and stromagenic cells (reviewed in 38 and
39). Under the stimulus of the metanephric mesenchyme, the ureteric bud grows and
branches 35. Expression studies in rodents have shown high levels of RET expression
early in development and much lower levels or absent expression in adult animals 1416.
We have identified a similar pattern of RETexpression in the developing human kidney 18.
Overall, RET expression was found to be approximately 7-fold higher at the earliest stage
of human kidney development investigated (7.5 weeks) compared to RETexpression in the
adult kidney. Around 6 weeks gestation, the ureteric bud is predicted to invade the
metanephric mesenchyme, establishing contact between the two populations of cells and
facilitating reciprocal inductive interactions. Branching morphogenesis and mesenchymal
differentiation. the results of reciprocal inductive interactions, begin around 6 weeks
gestation in humans and continue through to 32-34 weeks gestation (reviewed in 37).
Ureteric bud branching is rapid between 8 and 14-15 weeks gestation. RET expression was
found to decrease 1.5-fold by 8.5 weeks gestation, which is close to the time at which
rapid ureteric bud bifurcation is initiated (8 weeks). RET expression was found to decrease
considerably around 14 weeks gestation, when the rate of bud branching slows, and
approach adult kidney expression levels. The relatively high level of RET expression
observed in human fetal kidney aged 7.5 weeks compared to expression in adult kidney is
consistent with a role for RET early in kiduey development.
In the embryonic murine kidney, RET expression is found in epithelial cells
throughout the uninduced ureteric bud l6l6. W~th increasing gestational age, RET
expression localizes to the branching tips of the ureteric bud within the nephrogenic zone,
the site of reciprocal inductive interactions between the ureteric bud and the metanephric
mesenchyme 14- 15. The observed expnssion pattern is consistent with the phenotype of
the RET4- mice and suggestive of a role for this receptor in kidney development. REI-I-
mice display variable degrees of kidney dysgenesis characterized by growth failure and
reduced branchings of the ureteric bud as well as large areas of undifferentiated
metanephric mesenchyme 34. Th majority of RET-/- mice (67%) develop ureteric buds
indicating that R E ? signaling is not the first step in metanephric kidney induction 34.
However, in approximately one-half of these cases, the bud fails to invade the metanephric
mesenchyme. In comparison, the ureteric bud fails to form altogether in 100% of WT-I -/-
mice 41. W e molecules such as WT-1 are involved in ureteric bud formation, others such
as RET are necessary for interadom between the ureteric bud and metanephric
mesenchyme (Figure 1 5 ) .
RET 5' Alternatively Splicing Variants
Alternative splicing variants of RET are generated when exon 2 is spliced to any of
exons 3, 4, 5 or 6 (Figure 1.3) 13. The resulting transcripts differ from transcripts
encoding full length RET in that they lack sequence encoding portions of the RET
extraceUular domain. In the case where exon 2 is spliced to exon 5, a soluble product is
predicted due to a premature stop codon that resuits from translation of exon 5 out of h e
13. The expression levels of these variant RET mRNAs were found to vary during the
different stages of human kidney development 18. The expression levels of the REZW4 and
REZ2/5 alternatively spliced variants were consistently one-third the level of FL RET
expression. These results suggest that levels of these transcripts vary proportionally with
changing levels of overall RET expression during kidney development. The expression
pattern of the third transcript, RER16, was markedly different from those of the others.
Expression of -6 was found to be highest in our earliest sample, 8 weeks gestation,
the point in kidney development when rapid division of the ureteric bud is initiated
(reviewed in 37). Exp~ssion levels remained relatively high through to 14 weeks gestation
after which RETu6 expression levels were found to decrease (Figure 3.3). Decreased
expression of RETU6 coiacides with a period in kidney morphogenesis when the rate of
ureteric bud division slows and bifiucation is infkquent (14-20 weeks) (reviewed in 37).
Around 24 weeks gestation, expression levels of R E N 6 were found to approach those of
adult kidney. The high levels of RETZ16 expression during a period of rapid branching of
the ureteric bud and the corresponding decrease in expression when bifurcation slows may
suggest that the RET isoform encoded by this transcript is significant to the branching
process.
The distinct expression profile of REW6 relative to the other RET 5' alternatively
spliced variants during human kidney morphogenesis suggests that it is capable of
modulating a different subset of RET activities. These activities could be mediated at the
level of ligand binding. The alterations in the extracellular domain that result fiom
alternative splicing at the 5' end of RET result in novel RET isoforms which may have
distinct speciticity or affiaity for a RET ligand. For example, RER16 encodes a product
which lacks the entire region of cadherin homology present in the full length RET protein
13. If this protein is capable of binding the GDNWGDNFR-a complex, it is likely that its
affiaity for the complex differs from that of full length RET. It is equally possible that
RET2/6 binds an alternate RET ligand. The identification of new GDNF and GDNFR-a
family members has raised the possibility that Ligand relatives are also capable of binding to
RET. Neurturin was identified as a relative of GDNF based on sequence homology and a
similar ability to support neuronal survival in 31. Although these results suggest that
neumuin may act through signaling pathways similar to those of GDNF, the ability of
neurturin to interact with RET has yet to be investigated. Human RETL2 has been
identified as a relative of GDNFR-a and displays 49.146 homology to human GDNFR-a
33. Human -2. l i k GDNFR-a, can facilitate GDNF-dependent phosphorylation of
RET. In the absence of RET, GDNF has been shown to bind to GDNFR-a expressing
cells but to bind poorly to RETL2 expressing cells 3'. The differences in GDNF binding
observed for GDNFR-a and RETU are due to different requirements for RET to faciltate
complex formation: RETL2 binding to GDNF appears to be dependent on the presence of
RET whereas GDMR-a binding to GDNF is RET-independent.
As GDNFR-a and REIZ2 an both expressed in the embryonic kidney, it is
possible that either or both of these molecules Narc capable of modulating RET activity
during human kidney development 33. It will be interesting to leam if the various GDNF
and GDNFR-a family members are capable of interacting not only with RET but also with
its distinct isoforms. Little is known about the functions of these RET isoforms. In vine
translation of proteins fiom the corresponding cDNAs has been described 13 (M. Billaud,
personal communication). When these constructs were transfated into a kidney cell Line,
proteins were generated and those isoforms predicted to retain the transmembrane domain
were found to localize at the cell surface (M. Billaud, personal communication). This
suggests that the mechanisms are in piace for translocation of these RET isoforms to the
cell surface at least in this cell type.
GDNF and GDNFR-a in Human Kidney Development
The renal agenesis observed in the RET-1- and G D W - mice indicates the
importance of both of these molecules in kidney development 3 4 v 4 6 4 . It has been shown
that GDNF requires GDNFR-a for high affinity binding to the RET receptor 21. 22, 33. In
the absence of GDNFR-a, GDNF binding to RET and RET autophospholylation is
minimal. Chapter 5 describes the expression of RET ligand complex components in the
developing human kidney. The data are consistent with GDNF and GDNFR-a expression
during kidney development in rodents suggesting that the pathway is conserved in humans
22, 29.
A developmental expression pattern for GDNFR-a in human kidney
morphogenesis has been observed. GDNFR-a expression was found to be higher in the
early fetal kidney ages then decrease with increasing gestational age. Comparison of the
downward trends in RET and GDNFR-a expression during the come of human kidney
development indicates they are dissimilar. GDNFR-a expression levels were found to be
~latively consistent through the early ages of fetal kidney (7.5-14 weeks) whereas RET
expression was found to decrease dramatically between 7.5 and 8.5 weeks. A significant
decrease in GDNFR-a expression was not noted until 18 weeks gestation. These results
indicate that RET and G D N F R a expression are not coordinately regulated in the
developing human kidney. In light of the f a that GDNFR-a is required for high affinity
binding of GDNF to RET, it is clear that the reguiation of GDNFR-a expression during
human kidney development may act as a mechanism for regulating RET activation. In v i m
experiments have shown that overexpression of GDNFR-a augments GDNF binding to
RET and, hence, RET autophosphorylation 21- 22. This suggests that RET activity can be
regulated at the level of GDNFR-a. At early stages of kidney development, where both
GDNFR-a and RETexpression levels are high and GDNF is present, one might expect to
see increased levels of RET activation. When REI expression decreases, GDNFR-a
expression levels are maintained During this period of reduced RET expression, the high
levels of GDNFR-a could, in the presence of GDNF, be important for the maintenance of
RET activation. Regulation of RET activity at the level of GDNFR-a could be important in
tissues such as the kidney which co-express GDNFR-a family members such as EETL2
which is also capable of interacting with RET and GDNF. Sanicola et aL 33 suggest that
dissociation of the RETt2/GDNF/RET complex would release GDNF from the surface
while dissociation of the GDNFR-WGDNFIRET complex would leave GDNF bound to
GDNFRu on the cell surface and thus free to reassociate with RET. In the absence of the
ability to retain GDNF at the cell surface, RETL2 expressing cells would be more sensitive
to fluctuations in the local concentration of free GDNF.
RET 3' Alternatively Sjdiced Variants
RET appears to have roles in both protiferation and differentiation. A role for RET
in proliferation is suggested at both the in vim0 and in vivo levels. In vivo evidence for
RET's role in proliferation comes from MEN 2 patients. In these individuals, hyperplasia
of the calcitonin-producing C-cells of the thyroid is associated with activating mutations in
RET 8% 196. At the in vitro level, transfections of chimeric constructs resulting in
constitutive RET activation or of constructs with activating RET mutations both result in
tyrosine phosphorylation correlated with potent transformation and mitogenic activities 8'-
133. 197- 198. Conversely, the expression of constitutively activated RET in PC12 cells
results in morphological changes such as neurite outgrowth and induction of nemfilament
mRNA expression both of which are associated with differentiation in this cell type 5% 134-
198. The RET 3' isoforms appear to have varying effects on proliferation and
differentiation. While there are no functional data to suggest the role of the RET43 isoform,
there are data to suggest different roles for RET9 and RET5 1. Interestingly, we observed
RETSI was expressed at very low levels during the early stages of human kidney
development (7.5-8.5 weeks) and expression was upregulated around 9 weeks gestation
(Figure 4.5). Compared to RET5 1 expression. expression was relatively constant in
all ages of human fetal kidney examined There is an absolute requirement for RET early in
kidney development and our expression data suggest that RET9 possibly in conjunction
with RET43. satisfies this requirement. RElSl expression is upregulated at a later stage
when ureteric bud bifurcation is rapid which may indicate an important role for this isoform
in branching morphogenesis. Interestingly, the situation is different in the development of
the ENS. The identification of a R.1-specific mutation in a HSCR patient shows that
RETSI is absolutely required for the development of neurons in the lower gut 105. It is
possible that requirements for REn 1 expression during embryogenesis are tissue-specific.
Further studies are required to examine the details of RET9 and RET5 1 functions in kidney
development However, our data indicate that the two proteins have distinct roles in the
process.
RET9, RET51 and RET43 have in common the first 1062 amino acids but differ
with respect to their C-termini beginning at residue 1063. As a result of sequence
divergence at Y1062, RETSl contains an additional two tyrosine residues (Y 1090,
Y1096), not found in either of RET9 or RET43, one of which can be autophosphorylated
(Y lO96) lo- 12,136. While both RET9 and RETS1 isofonns display certain similarities with
respect to -interactions with downstream effector molecules, differences between the two
isoforms in their interactions have also been observed 5 6 s7 (M. Billaud, personal
communication). RET9 and RETS 1 differ with respect to their relative binding affinities for
the SH2 and PTB domains of the Shc adapter protein 57. Although Y1062 is the last
common amino acid shared by both RJ39 and RETS1. as a result of alternative splicing
after sequence encoding Y1062, this tyrosine residue is placed in different amino r i d
contexts in the translated products. M o u s l y , it was shown that the amino acid sequence
immediately upstream or downstream of pY residues confers preference for downstream
effector interactions (reviewed in 199). While Y 1062 has a greater affinity for Shc-SH2 in
the sequence context of RET9, in the sequence context of RETS I it has a greater affinity for
Shc-PTB interaction domain 56- 57 (M. Biilaud, personal communication). As a result of
the additional two tyrosine residues present in RET51, only RETSl contains a Grb2
interaction site (Y 106) and, hence, is capable of binding Grb2 directly via the SH2
interaction domain 56.57- In addition to binding to activated receptors. Grb2 is capable of
simultaneously binding to phosphorylated Shc in vivo (reviewed in 199). This enables
Grb2 to form multiple activated complexes with other SH2-containing proteins as well as
with activated receptors.
Upon phosphorylation of the receptor, both RET9 and RET5 1 have been shown to
associate with downstream molecules that interact with effectors of the RAS activation
pathway 56.57~ 200. The S hc and Grb2 adapter proteins are two such molecules. Both S hc
and Grb2 interact with phosphorylated RET via SH2 interaction domains while Shc is
additionally capable of interacting with RET via its PTB domain 56. Thus, RET 3' isoforms
differ in their downstream interaction and, potentially, these differences contribute to
distinct abilities of REIP and RETS1 to elicit downstxeam signaling responses. As
descn id above, our data show that RET5 1 expression is considerably lower in early fetal
kidney relative to expression at 9 weeks gestation and beyond. These results indicate that
RET51 is not required during the earliest stages of human kidney development d i k e
RET9 which is consistently expressed at relatively higher levels throughout kidney
organogenesis. The EZET5 1 isofom-specific mutation associated with HSCR supports the
theoxy of distinct roles for the RET 3' isoforms during development 105. The mutation in
this patient affects an amino acid residue immediately downstream of Y 1062 (M1064T). in
vitro, the mutation disrupts the interaction of N X 5 1 with the ITB domain of Shc 57.
Given that Shc phosphorylation is Linked to the RAS pathway, disruptions in Shc
phosphorylation are likely to disrupt activation of signaling through the RAS pathway.
Differences in expression of the RET 3' alternatively spliced variants such as those
identitied in the developing human kidney could be an important modulator of activation of
these pathways in these tissues.
The extremely low levels of REnl expression in the earlier stages of kidney
development investigated compared to 9 weeks gestation is interesting. RET9 and RETSl
isoforms appear to use distinct interactions to modulate downstream signaling pathways.
RAS activation can result in either proliferation or differentiation effects and it is not clear
which results from RET activation during the various stages of human kidney development
(reviewed in 201). The regulated expression of the EtET 3' isoforms in the developing
kidney could be an important determinant in proliferation versus differentiation both of
which are precisely timed events during development. The unique expression of REnl
relative to RE19 during human kidney development suggests non-compiementary roles for
these proteins. The RET51 isofom-specific HSCR mutation suggests that functional
RETS1 is required at a specifk time during development to ensure proper development.
The upregulation of RE151 expression we Qtected in a 9 week fetal kidney sample
coincides with a period of rapid ureteric bud bifurcation. Potentially, RE15 1 contributes to
the control of this process by affecting key downstream pathways responsible for
transcription of molecules involved in differentiation events. The relatively high levels of
RE19 expression throughout human kidney development suggest that RET9 has a role in
kidney morphogenesis that is distinct from that of RET5 1.
RET, GDNF and GDFNR-a in Human Disease
The mature human kidney consists of a number of different cell types each of which
is derived h r n either ureteric bud epithelium or metanephric mesenchyme 35. During the
early formative stages, the cells that give rise to the mature kidney express any of RET,
GDNF andlor GDNFR-a 14- 21. "- 29. RET is expressed in the ureteric bud epithelium
and its derivatives that give rise to the collecting duct system 14. While GDNFR-a
expression overlaps with RET expression in cells of the nephrogenic zone based on
irnmunocytochemistry, similar studies indicate that GDNFR-a may be expressed in a
broader range of cells 22. GDNF expression in metanephric mesenchyme is restricted to
undifferentiated cells which give rise to progeny with the potential to become either
nephrogenic or stromagenic cells (Figure 1.5) 29- 34. Given the cell typespecific
expression of these genes, some of the results of our investigation of RET, GDNF and
GDNFR-a expression in renal tumom are surprising. Renal cell carcinoma is thought to
arise from proximal tubule epithelial cells, highly specialized cells derived from
metanephric mesenchyme (reviewed in 174). We found Low Levels of GDNF expression in
adult kidney cortex samples but not in any of the I1 RCC samples dissected from the same
kidneys. Absence of GDNF expression in RCC is consistent with the tumour cell of origin.
The lack of expression in cells derived from metanephric mesenchyme following epithelial
conversion is predicted to be required to limit ureteric bud branching to the more distal
regions of the organ, preserving the radial patterning *02. Sanchez et al. 48 have shown
very Little GDNF is expressed in the tubular epithelium of the developing kidney suggesting
that GDAF expression is downregulated after epithelial differentiation.
RET expression appeared to be higher in n o d kidney samples relative to RCC
samples based on the intensities of the corresponding PCR products. Low levels of RET
expression are normally maintained in the adult kidney. The RET expression detected in
RCC might reflect the presence of contaminating normal cells which had been dissected
with the tumour sample. Alternatively, RETexpression in these tumours may be the result
of deregulated expression in this cell type. Mutations in genes responsible for RCC may
affect pathways involved in control of RET expression resulting in RET expression in a cell
type where it is normally absent.
GDNFR-a expression levels appeared similar in the RCC and matched normal
adult kidney cortex samples based on the intensities of the PCR products. GDNFR-a
expression in these tumours is not necessarily surprising. GDNFR-cx is expressed in cell
types which do not express RET. For example, GDNFR-a is expressed in Schwann cells
whereas RET is not 22. In situ hybridization has been used to show that GDNFR-a is
expressed between the inner and outer smooth muscle layers adjacent to and possibly
within the ENS; RET is only present in the ENS 22. Thus, GDNFR-a expression in RCC
may reflect the normal pattern of expression in the cell of origin and, thus, may not be
unusual whereas Rmexpression in RCC is unexpected.
Unlike RCC, expression of each of RET, GDNF and G D F N R a was detected in
the majority of WTs investigated. RET expression was consistent amongst tumour
samples. Single nunours expressed one of either GDNF or GDNFR-a in addition to RET
indicating that the collective expression of RET and the genes encoding its Iigmd
components is a common but not a consistent feature of WT. Expression studies have
shown that GDNFR-a and RET are both expressed in developing nephrons adjacent to
sites of GDNF expression 22. This indicates that the three components are not normally
expressed together in the same cell during kidney development. The WT cell of origin is
thought to be a derivative of the MM (reviewed in 140, 142 and 143). Given the tunour
cell of origin, GDNF expression in these tumours is not unexpected. GDNF is normally
expressed in both uninduced metanephric mesenchyme and its early derivatives 22.29. Both
cell types can be elements of WT 144 As with RCC, however, RET expression in WTs is
unexpected given the tumow cell of origin. There are no data to suggest that RET
represents one of the predicted genes responsible for WT. As mutations in s e v e d different
genes can result in an identical WT phenotype, it is Uely that several pathways may be
responsible for this phenotype. In this sense, RET expression in WT may be the result of
mutations in genes which, while not directly involved in RET expression, deregulate
pathways that are. G D N F M expression in WTs may be explained similarly.
RET mutations are found in 1040% of HSCR patients (reviewed in 88). Mutations
at other known HSCR loci account for an additional 3 4 % of cases indicating that a
significant proportion of HSCR disease is due to mutations in unidentified genes 98. 194.
195*203- 204. We identified a mutation in GDNF in a patient with HSCR that did not have
any mutations in other HSCR genes. The phenotype of GDNF-/- mice has suggested
GDNF is a HSCR candidate gene. Mice that lack functional GDNF are devoid of neurons
of the myenteric plexus which is derived from the vagal neural crest 4648. The absence of
the ENS in GDNF-I- mice was previously noted in RET-1- mice 34. Our data suggest that
mutations in either the receptor, RET, or its cognate ligand, GDNF, can result in a similar
phenotype. It has been found that mutations in either c-KIT or SLF, a complementary
receptor and ligand, result in similar phenotypes in mice and humans (reviewed in 139). It
is interesting that we have identified a GDNF mutation in only one of 36 HSCR patients
121. Similar studies have identified GDM:mutations in only four of 279 individual HSCR
patients 165. 193. Givea the low kquency of GDNF mutations in HSCR patients, it
appears that GDNF is not a major HSCR susceptibility locus.
In addition to a GDNF mutation associated with HSCR, we have identified a rare
GDNF polymorphism in a case of HSCR associated with deletion of a single copy of the
RET gene. The possibility exists that the polymorphism has a modulating effect on the
disease phenotype in this individual, however, any genotype-phenotype correlation has yet
to be proven. A situation where a polymorphism can affect disease phenotype is the prion
protein gene (PRNP). Whether individuals are homo- or heterozygous for a polymorphism
at codon 129 of PRNP affects susceptibility to sporadic or infectious CJD 179- 1%
Additionally, individuals bearing mutations at codon 178 of PRNP can present with either
f d a l CID or familial fatal insomnia depending on the nature of the polymorphism at
codon 129 182. It is unclear if the GDNF polymorphism we detected contributes to disease
phenotype in this individual, however, the possibility does exist that polymorphisms
contribute to the expression and/or severity of the HSCR disease phenotype.
Summary
The mature kidney arises from a series of reciprocal inductive interactions between
the ureteric bud epithelium and the MM. The RET proto-oncogene encodes an EUK
required for kidney development. We have identified developmental regulation of RET in
human kidney development. The datively high levels of RET expression in early
gestational ages compared to later in development indicate a role for RET in the early
inductive processes. In addition, we have identified variation in the expression levels of
alternatively spliced RETcoding variants over the course of kidney development Although
the functions of the isoforms these transcripts encode have not yet been fully characterized,
the developmental regulation of expression indicates roles for these proteins during specific
phases of kidney development.
GDNF and GDNFR-cx were recently identified as components of a ligand for RET.
GDNF is required for branching of the ureteric bud and differentiation of the MM in kidney
development similar to RET. We have identified expression of both GDM; and GDNFR-a
in the developing human kidney. In addition, we have shown that GDNTR-a expression is
developmentally regulated in this organ. Relatively high levels of GDNFR-a expression
are maintained when RET expression levels are downregulated. Given that GDNFR-a is
required for high affinity binding of GDNF to RET, our data suggest that regulation of
GDNFRa expression may be a means for regulating RET activity.
Abrogation of RET function contniutes to developmental anomalies. Inactivating
mutations in RET account for 104% of HSCR. We have identified a de n o w mutation in
GDNF suggesting that mutations in either the Iigand (GDNF) or the receptor (RET) can
result in a similar disease phenotype.
The expression of each of RET, GDNT and GDNFR-a in subsets of WTs is
interesting. Given that the WT cell of origin is believed to be derived fkom the MM, RET is
not predicted to be expressed in these tumours. Deregulation of transcriptional control
pathways during the course of tumourigenesis may result in RET expression as well as in
GDNFR-a expression in these tumours. The same can be said of RET and GDNFR-a
expression in RCC. Whether or not the expression of these genes has any tunour-specific
significance has not been investigated.
References
1. Takahashi, M., J. Ria , and G. M. Cooper. 1985. Activation of a novel human
transforming gene, ret, by DNA rearrangement. Cell. 4258 L -588.
2. Kuneida, T., M. Matsui, N. Nomura, and R. Ishizaki. 199 1. Cloning of an activated
human ref gene with a novel 5' sequence fused by DNA remgement . Gene. 107:323-
328.
3. Takahashi, M., and G. Cooper. 1987. ret transforming gene encodes a fusion protein
homologous to tyrosine kinases. Mol Cell Biol. 7: 1378-1385-
4. Itoh, F., Y. Ishizaka, T. Tahira, M. Yamamoto, A. Miya, K. Imai, A. Yachi, S. Takai,
T. Sugimwa, and M. Nagao. 1992. Identification and analysis of the ref proto-oncogene
promoter region in neuroblastoma cell lines and medullary thyroid carcinomas from
MENZA patients. Oncogene. 7: 120 1- 1206.
5. Kwok, J. B. J., E. Gardner, J. P. Warner, B. A. I. Ponder, and L. M. Mulligan. 1993.
Structural analysis of the human ref protmncogene using exon trapping. Oncogene.
8~2575-2582.
6. Myers, S., C. Eng, B. Ponder, and L. Mulligan. 1995. Characterization of RET proto-
oncogene 3' splicing variants and polyadenylation sites: a novel C terminus for RET.
Oncogene. 1 1:2039-2045.
7. Pasini, B., R. M. W. Hofstra, L. Yin, R. Bocciardi, G. Santanaria, P. M.
Grootscholten, I. Ceccherini, G. Patrone, M. Priolo, C. H. C. M. Buys, and G. Romeo.
1995. A physical map of the human RETproto-oncogene. Oncogene. 1 1: 1737-1743.
8. Ishizaka, Y., F. Itoh, T. Tahira, I. Jkeda, T. Sugimura, J. Tucker, and A. Fertitta.
1989. Human ret proto-oncogene mapped to 1Oq 1 1.2. Oncogene. 4: 15 19- 152 1.
9- Takahashi, M., Y. Buma, T. Iwamoto, Y. Inaguma, H. Ikeda, and H. Hiai. 1988.
Cloning and expression of the ret protooncogene encoding a tyrosine kinase with two
potential transmembrane domains. Oncogene. 357 1-578.
LO. Takahashi. M., Y. Buma, and H. Hi& 1989. Isolation of ref protooncogene cDNA
with an amino-terminal signal sequence. Oncogene. 4:805-806.
1 1. Tahira, T., Y. IshiAa, T. Sugimura, and M. Nagao. 1988. Expression of proto-ret
mRNA in embryonic and adult rat tissues. Biochem Biophys Res Cornmun. 153: l29O-
1295.
12. Tahira, T., Y. Ishizaka, F. Itoh, T. Sugimura, and M. Nagao. 1990. Characterization
of ret protooncogene mRNAs encoding two isoforms of the protein product in a human
neuroblastoma cell line. Oncogene. 5:97-102.
13. Lorenzo, M. J., C. Eng, L. M. MulIigan, T. J. Stonehouse, C. S. Healey, B. A. J .
Ponder, and D. P. Smith. 1995. Multiple mRNA isoforms of the human RET proto-
oncogene generated by alternative splicing. Oncogene. 10: 137701383.
14. Pachnis, V., B. Mankoo, and F. Costantini. 1993. Expression of the c-ref proto-
oncogene during mouse embryogenesis. Development. 1 19: 1005- 10 17.
15. Avantaggiato, V., N. Dathan, M. Grieco, N. Fabien. D. Lanaro, A. Fusco, A.
Simeone, and M. Santoro. 1994. Developmental expression of the RET protooncogene.
Cell Growth and Differentiation. 5:305-3 1 1.
16. Tsuzuki, T., M. Takahashi, N. Asai, T. lwashita, M. Matsuyama, and J. Asai. 1995.
Spatial and temporal expression of the ret protooncogene product in embryonic, infant and
adult rat tissues. Oncogene. 10: 19 1- 198.
17. Nakamura, T., Y. Ishizaka, M. Nagao, M. Ham, and T. Ishikawa. 1994. Expression
of the ret proto-oncogene product in human normal and neoplastic tissues of neural crest
origin. J Pathol. l72:255-260.
IS. Ivanchuk, S. M., C. Eng, W. K. Cavenee, and L. M. MuIligan. 1997. The expression
of RET and its multiple splice forms in developing human kidney. Oncogene. In press.
19. Trupp, M., E. Arenas, M. Fainzilber, A.-S. Nilsson, B.-A. Sieber, M. Grigoriou, C.
Kilkenny, E. Salazar-Grueso, V. Pachnis, U. Arum&, H. Sariola, M. Saarma, and C. F .
Ibiiiez. 1996. Functional receptor for GDNF encoded by the c-ref proto-oncogene. Nature.
38 1 :785-789.
20. Durbec, P., C. V. Marcos-Gutierrez, C. Kllkenny, M. Grigoriou K. Wartiowaara. P.
Suvanto, D. Smith, B. Ponder, F. Costaathi, M. Saarma, H. Sariola, and V. Pachnis.
1996. GDNF signalling through the Ret receptor tyrosine kinase. Nature. 38 1 :789-793.
21. ling, S., D. Wen, Y. Yu, P. L. Hol~t, Y. Luo, M. Faag, R. Tamir, L. Antonio, 2.
Hu, R. Cupples, J.-C. Louis, S. Hu, B. W. Mtrock, and G. M. Fox. 1996. GDNF-
induced activation of the Ret protein tyrosine kinase is mediated by GDNFR-a, a novel
receptor for GDNF. Cell. 85: 1 1 13- 1 124.
22. Tremor, I. J. S., L. Goodman, F. de Sauvage, D. M. Stone, K. T. Podsen, C. D.
Beck, C. Gray, M. P. Armanini, R. A. Pollock, F. Hefii, H. S. Phillips, A. Goddad M.
W. Moore, A. Buj-BeLIo, A. M. Davies, N. Asai, IM. Takahashi, R- Vanden, C. E.
Henderson, and A. Rosenthal. 1996. Characterization of a multicomponent receptor for
GDNF. Nature. 382:80-83.
23. Lin. L.-F. H., D. H. Doherty, J. D. Lile, S. Bektesh, and F. Collins. 1993. GDm a
&a1 cell hederived neurotmphic factor for midbrain dopaminergic neurons. Science.
260: 1130-1 132,
24. Lin, L., T. Zhang, F. Collins, and L. Armes. 1994. Purification and initial
characterization of rat B49 glial cell line-derived neurotrophic factor. J Neurochem. 633758-
768.
25. Schindelhauer, D., S. Schaenhauer, T. Gasser, A. Steinkasserer, and T. Meitinger.
1995. The gene coding for glial cell line-derived neurotrophic factor (GDNF) maps to
chromosome Sp 12- 13.1. Genornics. 28:605-607.
26. Suter-Crazzolara, C., and K. Unsicker. 1994. GDNF is expressed in two forms in
many tissues outside the CNS. NeuroRepon. 5:2486-2488.
27. Choi-Lundberg, D. L., and M. C. Bohn. 1995. Ontogeny and distribution of glial cell
line-derived neurotmphic factor (GDNF) mRNA in rat. Devel Brain Res. 85230-88.
28. Trupp, M., M. Ryden, H. Jornvall, H. Funakoshi, T. Timmush E. Arenas, and C.
Ibfiez. 1995. Peripheral expression and biological activities of GDNF, a new neurotrophic
factor for avian and mammalian peripheral neurons. J Cell Biol. 130: 137- 148.
29. HeUmich, H. L., L. Kos, E. S. Cho, K A. Mahon, and A. Zimmer. 1996. Embryonic
expression of glial cell-he derived neurotrophic factor (GDNF) suggests multiple
developmental roles in neural differentiation and epithelial-mesenchymal interactions. Mech
Devel. 54:95- 105.
30. Unsicker, K. 1996. GDW. a cytokioe at the interface of TGF-Bs and neurotrophins.
Cell Tissue Res. 286: 175- 178.
31. Kotzbauer. P. T., P. A. Lampe, R. 0. Heuckeroth. J. P. Golden, D. J. Creedon, E.
M. Johnson, and I. Milbrandt. 1996. Neurnuin, a relative of glial-cell-line derived
neurotrophic factor. Nature. 384:467-470.
32. Wnfriend, S ., and K. Kodulrula. 1995. How glycosyIphosphatidylinositol-anchored
membrane proteins are made. Ann Rev Biochem. 64563-59 1.
33. Sanicola, M., C. Hession, D. Worley, L. Walus. P. Carmillo, C. Ehrenfels, S .
Robinson, G. larworski, H. Wei, R. Tizard, A. Whitty, R. B. Pepinsky, and R. Cate.
submitted. Two accessory proteins mediate glialcell-line derived neurotrophic factor
(GDNFJ-dependent RET signalling via distinct mechanism. Pruc Nut1 Acad Sci, USA.
submitted.
34. Schuchardt, A., V. D'Agati, L. Larsson-Blomberg, F. Costantini, and V. Pachnis.
1994. Defects in the kidney and enteric nervous system of mice lacking the tyrosine kinase
receptor Ret. Nature. 3673380-383.
35. Saxen, L. 1987. Organogenesis of the kidney. Vol. 19. P. W. Barlow, P. B. Green,
and C. C. White, editors. Cambridge University Ress, Cambridge. 1-87.
36. Durbec, P. L., L. B. Larsson-Blomberg, A. Schuchardt, F. Costantini, and V.
Pachnis. 1996. Common origin and developmental dependence on c-ret of subsets of
enteric and sympathetic neuroblasts. Development. 122349-358.
37. Potter, E. L. 1972. Normal and A b n o d Development of the Kidney. Year Book
Medical Publishers Inc., Chicago. 305 pp.
38. Bard, I., J. Davies, I. Karavanova, E. Lehtonen, H. Sariola, and S. Vainio. 1996.
Kidney development: the inductive interactions. Cell Devel Bid. 7: 195-202.
39. Bard, J. A., J. E. McCo~eu, and l. A. Davies. 1994. Towards a genetic basis for
kidney development. Mech Devel. 48:3- 1 1.
40. Schuchardt, A., V. D'Agati, V. Pachnis, and F. Costanthi. 1996. Remi agenesis and
hypodysplasia in ret-k- mutant mice result from defects in ureteric bud development.
Development. 122: 19 19- 1929.
41. Kreidberg, J. A., H. Sariola, I. M. Loring, M. Maeda, J. PeUetier, D. Housmm, and
R. Jaenisch. 1993. WT- 1 is required for early kidney development. Cefi. 74:67969 1.
42. Mendelsohn, C., D. Lohnes, D. Decimo, T. Lutkin, M. Lemeur. P. Chambon and M.
Mark. 1994. Function of the retinoic acid receptors (RARs) during development.
Development. 120:2749-277 1.
43. Armstrong, J. F., P.-J. K, W. A. Bickmore, N. D. Hastie, m d J. B. L. Bard. 1992.
The expression of the Wilms' turnour gene WT-1 in the developing mammalian kidney.
Mech Devel 40: 85-97.
44. Pritchard-Jones, K.. S. Heming, D. Davidson, W. Bickmore, D. Porteous, C.
Gosden, J. Bard, A. Buckler, J. Pelletier, D. Housman, V. van Heyningen, and N.
Hastie. 1990. The candidate Wilms' tumor gene is involved in genitourinary development.
Nature. 346: 194-197.
45. D a m , K., R. Heyman, K. Umesono, and R. Evans. 1993. Functional inhibition of
retinoic acid response by dominant negative retinoic acid receptor mutants. Proc Narl Acad
Sci. 90:2989-2993.
46. Moore, M. W., R. D. Klein, I. Faciiias. H. Sauer, M. Annanini, H. Phillips, L. F.
Reichardt, A. M. Ryan, K. Carver-Moore, and A. Rosenthaf. 1996. Renal and neuronal
abnormalities in mice lacking GDNF. Nature. 382:76-79.
47. Pichel, I. G., L. Shea, H. 2- Sheng, A*-C. Gcanhoh, J. Drago, A. Grinberg, E- I.
Lee, S. P. Huang, M. Saarma, B. J. Hoffer, H. Sariola, and H. Westphal. 1996. Defects
in enteric innervation and kidney development in mice lacking GDNF. Nature. 382:73-76.
48. Shchez, M. P., I. Silos-Santiago, J. Frisen, S. A. Lira, and M. Barbacid 1996.
Renal agenesis and the absence ofenteric neurons in mice lacking GDNF. Nutzwe. 382:70-
73.
49. Maas, R., R. Zeller, R. Woychik, T. Vogt, and P. Leder. 1990. Disruption of formin-
encoding transcripts in two limb dflormity alleles. Nature. 346:853-855.
50. Dudley, A., K. Lyons, and E. Robertson. 1995. A requirement for bone
morphogewtic protein-7 during development of the mammalian kidney and eye. Genes d
Devel. 9:2795-2807.
5 L. Dressler, G.. J. Wilkinson, U. Rothenpieler, L. Patterson. L. Wiams-Simons, and
H. Westphal. 1993. Deregulation of Pax-2 expression in transgenic mice generates severe
kidney abnormalities. Nature. 362:65-67.
52. Stark, K., S. Vainio, G. Vassileva, and A. P. McMahon. 1994. Epithelial
transformation of metanephric mesenchyme in the developing kidney regdated by Wnt-4.
Nature. 372:679-683.
53. Dressler, GOT U. Deutsch, K. Chowdhury, H. Homes, and P. Gruss. 1990. Pax2, a
new murine paired-box containing gene and its expression in the developing excretory
system. Deve[opment. 109:787-795.
54. Ryan, G., V. Steele-Perkins, J. F. Morris, F. J. Rauscher, and G. R Dressler. 1995.
Repression of Pax-2 by WTl during normal kidney development. Development. 12 13367-
875.
55. Rossel, M., A. Pasini, S. Chappuis, 0. Geneste, L. Fournier, I. Schuffenecker, M.
Takahashi, L. A. van Grunsven, J. L. Urdiales, B. B. Rudkin. G. M. Lenoir, and M.
Billaud. 1997. Distinct biological properties of two RET isoforms activated by MEN
2A/FMTC and MEN 2B mutations. Oncogene. 14:265-275.
56. Bod lo , M. G., G. Pelicci, E. Arighi, L. DeFilippis, A. GECO, I. Bongarzone, M.
G. Rinetti, P. G. Pelicci, and M. A. Pierotti. 1994. The oncogenic versions of the ret and
trk tyrosine kinases bind Shc and Grb2 adaptor proteins. Oncogene. 9: 166 1- 1668.
57. Lorenzo, M., G. Gish, C. Houghton, T. Stonehouse, T. Pawson, B. Ponder, and D.
Smith. 1997. RET alternative splicing influences the interaction of activated RET with the
SH2 and PTB domains of Shc, and the SH2 domain of Grb2. Oncogene. 14:763-77 1.
58. van der Geer, P., and T. Hunter. 1994. Receptor protein-tyrosine kinases and their
signal transduction pathways. Ann Rev Cell Biol. l O : Z 1-337.
59. Klein, R., D. Conway, L. F. Parada, and M. Barbacid. 1990. The trkB tyrosine
kinase gene codes for a second neurogenic receptor that lacks the catalytic kinase domain.
Cell. 6 1 3647-656.
60. Lambde, F., R Klein, and M. Barbacid 1991. trlcC, a new member of the trk family
of tyrosine protein kinases, is a receptor for neurotrophin-3. Cell. 66:967-979.
61. Tsoulfas, P., D. Soppet, E. Escandon, L. Tessarollo, J. Mendoza-Ramirez, A.
Rosenthal, K. Nikolics, and L. Parada. 1993. The rat trkC locus encodes multiple
neurogenic receptors that exhibit differential response to neurotrophin-3 in PC 12 cells.
Neuron. 10:975-990.
62. Valemela, D., P. Maisonpierre, D. Glass, E. Rojas, L. Nunez, Y. Kong, D. Gies, T.
Stin. N. Ip, and G. Yancopoulos. 1993. Alternative forms of rat TrkC with different
functional capabilities. Neuron. 10:963-974.
63. Partanen, J., S. Vainikka, J. Korhonen, E. Armstrong, and K. Alitalo. 1992. Diverse
receptors for fibroblast growth factors. Prog Growth Factor Res. 4:69-83.
64. McDonald, F. J. 1994. Developmentally Regulated Expression of Fibroblast Growth
Factor Receptor Genes and Splice Variants by Murine Embryonic Stem and Embryonal
Carcinoma Cells, Devel Genet. 15: 148- 154.
65. Johnson, D., I. Lu, H. Chen, S. Werner, and L. Williams. 1991. The human
fibroblast growth factor receptor genes: A common structural arcangemem underlies the
mechanism for generating receptor forms that differ in their third immunoglobulin domain.
Mol Cell Biol. 1 1 :4627-4634.
66. Werner, S., D. Duan, d. V. C, K, Peters, D. Johnson, and L. Williams. 1992.
Differential splicing in the extracellular region of £%roblast growth f ~ o r receptor 1
generates receptor variants with different Ligand-binding specificities. Mol Cell Biol. 1282-
88.
67. Avivi, A., A. Yayon, and D. Givol. 1993. A novel form of FGF receptor 3 using an
alternative exon in the immunoglobulin domain III. FEBS Letfers. 330:249-252.
68. Miki. T., D. P. Bottaro, T. P. Fleming, C. L. Smith, W. L. Burgess. A. M.-L. Chan,
and S. A. Aaronson. 1992. Determination of ligand-binding specificity by alternative
splicing: Two distinct growth fictor receptors encoded by a single gene. Proc Nati Acod
Sci USA. 89:246-250.
69. Yayon, A., Y. Zimrner, G. Guo-Hong, A. Avivi, Y. Yarden, and D. Givol. 1992. A
confined region confers ligand binding specificity on fibroblast growth factor receptors:
Implications for the origin of the immunoglobulin fold. EMBO J. 1 1 : 1885- l89O.
70. On-Urtreger, A., M. T. Bedford, T. Burakova, E. Arman, Y. Zimmer, A. Yayon. D.
Givol. and P. Lonai. 1993. Developmental localization of the splicing alternatives of
fibroblast growth faftor receptor-;? (FGFR2). Devel Biol. 158:475-486.
71. Shi, D.-L., C. Lauoay, V. Fromentoux, J.-J. Feige, and I.-C. Boucaut. 1994.
Expression of fibroblast growh factor receptor-2 splice variants is developmentally and
tissue specifically regulated in the amphiiian embryo. Devel B i d 164: 173-182.
72. Jackson-Grusby, L., A. Kuo. and P. Leder. 1992. A variant Limb deformity transcript
expressed in the embryonic mouse limb defiws a novel formin. Genes and Devel. 6:29-37.
73. Chan, D., A. Wynshaw-Boris, and P. Leder. 1995. Formin isofom are differentially
expressed in the mouse embryo and are required for nonnai expression of fgf4 and shh in
the limb bud. Development. 121:3 15 1-3 162.
74. Santoro, M., R. Rosiui, M. Grieco, M. T. Berlingieri, G. L. C. D'Amato, V.
deFranciscis, and A. Fusco. 1990. The RET protooncogene is consistently expressed in
human pheochromocytomas and thyroid medullary carcinomas. Oncogene. 5: 1595-1 598.
75. Tahira, T., Y. Ishizaka, F. Itoh, M. Nakayasu, T. Sugimura and M. Nagao. 1 99 1.
Expression of the ret proto-oncogene in human neurob1astoma cell lines and its increase
during neuronal differentiation induced by retinoic acid. Oncogene. 6:2333-2338.
76. Nagao, M., Y. Isbaka, A. Nakagawara, K Kobo, M. Kuwano, T. Tahim F. Itoh,
I. Ikeda, and T. Sugimara. 1990. Expression of ref proto-oncogene in human
neuroblastomas. Jup J Canc Res. 8 1 :309-3 12.
77. Hofstra, R. M. W., N. C. Cheng, C. Hansen, R. P. Stulp, T. Stelwagen, N. Clausen,
N. Tommerup, H. Caron, A. Westerveld, R. Versteeg, and C. H. C. M. Buys. 1996. No
mutations found by RM mutation scanning in sporadic and hereditary neurobiastoma
Hum Genet. 97:362-364.
78. Ishizaka, Y., H. Shima, T. Sugimura, and M. Nagao. 1992. Detection of
phosphorylated r e t m oncogene product in cytoplasm. Oncogene. 7: 144 1- 1444.
79. Bonganone, I., N. Montini, M. G. Borrello, C. Carcano, G. Ferraresi, E. Arighi. P.
Mondellini, G. Della Porta, and M. A. Pierotti. 1993. Molecular characterization of a
thyroid tumor-specific transforming sequence formed by the fusion of ref tyrosine kinase
and regulatory subunit RIa of cyclic AMP-dependent protein kinase A. Mol Cell Biol.
13:358-366.
80. Santoro, M., N. Dathan, M. Berlingieri, I. Bongarzow, C. Paulin, M. Grieco, M.
Pierotti, G. Vecchio, and A. Fusco. 1994. Molecular characterization of RET/PTC3; a
novel rearranged version of the RET proto-oncogene in a human thyroid papillary
carcinoma. Oncogene. 9:509-5 16.
81. Grieco, M., M. Santoro, M. T. Berlingieri, R. M. Meiillo, R. Donghi, I. Bongmone,
M. A. Pierotti, G. Della Porta, A. Fusco, and G. Vecchio. 1990. PTC is a novel
rearranged form of the ret protooncogene and is frequently detected in vivo in human
thyroid papillary carcinomas. Cell. 60:557-563.
82. Bonganone, I., M. Butti, S. Coronelli, M. BorrelIo, M. Santoro, P. Mondellini, S.
Pilotti, A. Fusco, G. Della Porta, and M. Pierotti. 1994. Frequent activation of ret
protooncogene by fusion with a new activating gene in papillary thyroid carcinomas. Cimc
Res. 542979-298s.
83. Pierotti, M. A., M. Santoro, M. B. Jenkins, G. Sozzi, I. Boagarzone, M. Grieco, M.
Monzini, M. Miono, M. A. Kemnann, A. Fusco, I. D. Hay, G. DeUa Porta, and G .
Vecchio. 1992. Characterization of an inversion on the long arm of chromosome 10
juxtaposing Diosizo and Ret and creating the oncogenic sequence RetlPTC. P roc Natl Acod
Sci USA. 89: 16 16 - 1620.
84. Mulligan, L. M., I. B. I. Kwok, C. S. Healey, M. I. Elsdon, C. Eng, E. Gardner, D.
R. Love, S. E. Mole, I. K. Moore, L. Papi, M. A. Ponder, H. Telenius, A. Tunnacliffe,
and 8. A. J. Ponder. 1993. Germ-line mutations of the RET proto-oncogene in multiple
endocrine neoplasia type 2A. Namre. 363:458-460.
85. Mulligan, L. M., C. Eng, C. S. Healey, D. Clayton, J. B. I. Kwok, E. Gardner, M.
A. Ponder, A. Frilling, C. E. Jackson, H. Lehnert, H. P. H. Neumann, S. N. Thibodeau,
and B. A. J. Ponder. 1994. Specific mutations of the RET protwncogene are related to
disease phenotype in MEN 2A and FMTC. Nature Genet. 6:70-74.
86. Donis-Keller, H., S. Dou, D. Chi, K. M. Carlson, K. Toshima, T. C. Lairmore, J. R.
Howe, I- F. Moley, P. Goodfellow, and S. A. Wells. 1993. Mutations in the RET proto-
oncogene are associated with MEN 2A and FMTC. Hum MoL Genet. 2 :MI-856.
87. Santoro. M., F. Carlomagno, A. Romano, D. P. Bottaro, N. A. Dathaa, M. Grieco,
A. Fusco, G. Vecchio, B. Matoskova, M. H. Kraus, and P. P. Di Fiore. 1995. Activation
of RETas a dominant transforming gene by germline mutations of MEN2A and MEN2B.
Science. 267:38 1-383.
88. Eng, C., and L. M. Mulligan. 1997. Mutations of the RET protooncogene in the
multiple endocrine neoplasia type 2 syndromes, related sporadic nunours and Hirschspruag
disease. H m Mutat. 9:97- 109.
89. Eng, C.. D. Clayton. I. Schuffenecker, G. Lenoir, G. Cote, R. F. Gagel, H.-K Ploos
van Amstel, C. J. M. Lips, I. Nishisho, S.4. Takai, D. J. Marsh, B. G. Robinson, K.
Frank-Raue, F. Raue, F. Xu, W. W. No& C. Romei, F. Pacini, M. Fink, B. Niederie, J .
Zedeaius, M. Nordenskjold, P. Komminoth, G. Hendy, H. Gharib, S. T h l i e a u , A.
Lacroix, A: Frilling, B. A. J. Ponder, and L. M. Mulligan. 1996. The relationship between
specific RET pmto-oncogene mutations and disease phenotype in multiple endocrine
neoplasia type 2: International REl Mutation Consortium. J M . 276: 1575- 1579.
90. Mulligan, L. M., D. I. Marsh, B. G. Robinson, I. Schuffenecker, J. Zedenius, C. J .
M. Lips, R. F. Gagel, S.4. Takai. W. W. NOH. M. Fink, F. Raue, A. Lacroix, S. N.
Thibodeau. A. Frilling, B. A. J. Ponder, C. Eng, and International RET Mutation
Consortium. 1995. Genotype-phenotype cordation in multiple endocrine neoplasia type 2:
report of the International RET Mutation Consortium. J Intern Med. 238:343-346.
91. Bolino, A., I. Schuffenecker, Y. Luo, M. Seri, M. Silengo, T. Tocco, G. Chabrier,
C. Houdent, A. Murat, M. Schlumberger, J. Toumiaire, G. M. Lenoir, and G. Romeo.
1995. RET mutations in exons 13 and 14 of M C patients. Oncogene. 10:2415-2419.
92. Boccia, L. M., J. S. Green, C. Joyce, C. Eng, S. A. M. Taylor, and L. M. Mulligan.
in press. Mutation of RET codon 768 is associated with the M C phenotype. Clin Genet.
in press.
93. Eng, C., D. P. Smith, L. M. Mulligan, C. S. Healey, M. J. Zvelebil, T. J.
Stonehouse, M. A. Ponder, C. E. Jackson, M. Waterfield, and B. A. J. Ponder. 1995. A
novel point mutation in the tyrosine kinase domain of the RET proto-oncogene in sporadic
medullary thyroid carcinoma and in a family with FMTC. Oncogene. lO:509-5 13.
94. Hofsaa, R. M. W., R. M. Landsvater, I. Ceccherini, R. P. Stulp. T. Stelwagen, Y.
Luo. B. Pasini, J. W. M. Hoppener, H. K. Ploos van Amstel, G. Romeo, C. L M. Lips,
and C. & C. M. Buys. 1994. A mutation in the RET proto-oncogene associated with
multiple endocrine neoplasia type 2B and sporadic medullary thyroid carcinoma. Nature.
367:375- 376.
95. Eng, C.. D. P. Smith, L. M. Mulligan, M. A Nagai, C. S. Healey, M. A. Ponder, E.
Gardner, G. F. W. Scheumaan, C. E. Jackson, A. Tunnacliffe, and B. A. J. Ponder.
1994. Point mutation within the tyrosine kinase domain of the RET protooncogene in
multiple endocrine neoplasia type 2B and related sporadic ttunours. Hum Mol Genet.
3 :237-24 1 ;
96. Carlson, K, M., S. Dou, D. Chi, N. Scavarda, K. Toshirna, C. E. Jackson, S. A.
Wells, P. J. Goodfellow, and H. Donis-Keller. 1994. Single missense mutation in the
tyrosine kinase catalytic domain of the ret proto-oncogene is associated with multiple
endocrine neoplasia type 2B. Proc Noll Acad Sci USA. 9 L : 1579- 1583.
97. Passarge. E. 1967. The genetics of Hirschsprung's disease. Evidence for
heterogeneous etiology and a study of sixty-three families. AL Engl. I. Med. 276: 138- 143.
98. Chakravarti, A. 1996. Endothelin receptor-mediated signaling in Hirschsprung disease.
Hum Mol Genet. 5303-307.
99. Pasini, B-, M. G. BorreUo, A. Greco, I. Bonganone, Y. Luo, P. Mondek, L.
Alberti, C. Mirancia, E. Arighi. R. Bocciardi, M. Seri, V. Baroae, M. T. Radice. G.
Romeo, and M. A Pierotti. 1995. Loss of function effkct of RET mutations causing
Hirschspmg disease. Nature Genet. 10:35-40.
100. Luo, Y., I. Ceccherini, B. Pasini, I. Matera, M. P. Bicocchi, V. Baroae, R.
Bocciardi, H. KMriiiinen, D. Weber, M. Devoto, and G. Romeo. 1993. Close Linkage
with the RET proto-oncogene and boundaries of deletion mutations in autosomal dominant
Hirschsprung disease. Hum Mol Genet. 2: 18034808.
101. Fewtrell, M. S., P. K. H. Tam, A. H. Thornson, M. Fitchett, J. Currie, S. M.
Huson, and L. M. Mulligan. 1994. Hinchsprung's disease associated with a deletion of
chromosome 10(q 1 1.2): a further Iink with the neurocristopathies? J Med Genet.
3 1:325-327.
102. Edery, P., S. Lyomet, L. M. Mulligan, A. Pelet, E. Dow, L. Abel, S. Holder, C.
Nihoul-F6k&6, B. A. I. Ponder, and A. Munnich. 1994. Mutations of the RET proto-
oncogene in Hirschsprung's disease. Nature. 367:378-380.
103. Romeo. G., P. Ronchetto. Y. Luo, V. Barme, M. Seri. I. Ceccherini, B. Pasini, R.
Bocciardi, M. Lerone, H. Kiiiiriiiinen, and G. Martucciello. 1994. Point mutations
affecting the tyrosine kinase domain of the RET proto-oncogene in Hirrchsprung's disease.
Nature. 367:377- 378.
104. Luo. Y., V. Barone, M. Seri, A. Bolino. R. Bocciardi, I. Ceccherini, B. Pasini, T.
Toco, M. Lerone, S. Cywes, S. Moore, I. M. Vanderwinden. M. J. Abramowicz, U.
Kristofferson, L. T. Lanson, M. Silengo, G. Martuciello, and G. Romeo. 1994.
Heterogeneity and low detection rate of RET mutations in Hirschsprung disease. Eur J
Hum Genet. 2:272-280.
105. Attie, T., A. Pelet, P. Edery, C. Eng, L. M. Mulligan. I. Arniel, L. Boutran, C.
Beldjord, C. Nioul-Feltit& A. Munnich, B. A. J. Ponder, and S. Lyomet 1995.
Diversity of RET proto-oncogene mutations in f d a l and sporadic Hirschsprung disease.
Hum Mol Genet. 4: 138 1- 1386.
L06. Angrist. MOT S. Bok, B. Thiel. E. G. Puffenberger, R. M. Hofstra, C. H. C. M.
Buys, D. T. Cass, and A. Chakravarti. 1995. Mutation analysis of the RET receptor
tyrosine kinase in Hirschsprung disease. Hwn Mol Genet. 4:82 1-830.
107. Yin, L. 1994. Heterogeneity and low detection rate of RET mutations in
Hirschsprung disease. Eur J Hum Genet. 2:272-280.
108. Blaugrund. J. E., M. M. Johns, Y. J. Eby, D. W. Bd, S. B. Baylin. R. H. Hruban,
and D. Sidransky. 1994. RET proto-oncogene mutations in inherited and sporadic
medullary thyroid cancer. Hum Mol Genet. 3: 1895- 1897.
109. Eng, C., L. M. Mulligan, D. P. Smith, C. S. Healey, A. Frilling, F. Raue, H. P. H.
Neumam, R. Pfragner, A. Behmel. M. I. Lonnzo, T. I. Stonehouse. M. A. Ponder. and
B. A. 3. Ponder. 1995. Mutation of the RET protooncogene in sporadic medullary thyroid
carcinoma. Genes Chrom Cane. l2:209-2 12-
1 10. Zedeaius, J., G. WaIlin, B. Hamberger, M. Nordenskjold, G. Weber, and C.
Larsson. 1994. Somatic and MEN 2A de novo mutations identified in the RET proto-
oncogene by screening of sporadic ma. Hum Mol Genet. 3:1259-1262.
1 1 1 . Zedenius, I., C. Larsson, U. Bergholm, I. BovCe, A. Svensson, B. Hallengren, L.
Grimelius, M. Backdahl, G. Weber, and G. Wallin. 1995. Mutations of codon 9 18 in the
RET proto-oncogene correlate to poor prognosis in sporadic medullary thyroid carcinomas.
J Clin Endacrinol Metab. 80:3088-3090.
112. Komminoth, P., E. K. Kunz, X. Matias-Guiu, 0. Hion, G- Christiansen, A.
Colomer, I. Roth, and P. U. Heitz. 1995. Analysis of the RET protooncogene point
mutations distinguishes heritable from nonheritable medullary thyroid carcinomas. Cmcer.
76:479-489.
113. Marsh, D. J., D. L. Learoyd, S. D. Andrew, L. Krishnan, R. Pojer, A.-L.
Richardson, L. Delbridge, C. Eng, and B. G. Robinson. 1996. Somatic mutations in the
RET proto-oncogene in sporadic medullary thyroid carcinoma Clin Endocrinol. 44249-
257.
114. Dou, S., D. Chi, K. M. Carlson, I. A. Moley, S. A. Wells, and H. Donis-Keller.
1994. RET protooncogene mutations associated with sporadic cases of medullary thyroid
carcinoma. F@h International Workshop on Multiple Endocrine Neoplasia:73.
115. Donis-Keller, H. 1995. The RlT proto-oncogene and cancer. J Intent Med. 238:3 19-
325.
116. Romei, C., R. Elisei, A. Pinchera, I. Ceccherhi, E. Molinaro, F. Mancusi, E.
Martino, G. Romeo, and F. Pacini. 1996. Somatic mutations of the RET proto-oncogene
in sporadic medullary thyroid carcinoma are not to exon 16 and are associated
with tumor recurrence. J CZin Endocrinul Metab. 8 1 : 16 19- 1622.
117. Lindor, N. M,, R- Honchel, S. Khosla, and S. N. Thrideau. 1995. Mutations of
the RET protwncogene in sporadic pheochromocytomas. J CIin Endocri1101 Metab.
80:627-629.
118. Kornminoth, P., E. Kunz, 0. Hiort, S. SchrWer, X. Matias-Guiu, G. Christiansen,
J. Roth, and P. U. Heitz. 1994. Detection of RET protooncogene point mutations in
paraffin-embedded pheochmmocytoma specimens by nonradioactive single-strand
conformation polymorphism analysis and direct sequencing. Am J Path. 145922-929.
1 19. Beldjord, C., F. Desclaux-Arramond, M. Raffiin-Sanson, J. C. Corvol, Y. De
Keyser, J. P. Luton, P. F. Plouin, and X. Bertagaa 1995. The RE;T protooncogene in
sporadic pheochromocyt~mas: fkquent Multiple Endocrine Neoplasias 2-Like mutations
and new molecular defects. J Clin Endo Metab- 80:2063-2068.
120. Rychlik, W., and R. E. Rhoads. 1989. A computer program for choosing optimal
oligonucleotides for filter hybridization, sequencing and in vino amplification of DNA.
Nucleic Acids Research. 17 (2 1):8543-855 1.
121. Ivanchuk, S. M., S. M. Myers, C. Eng, and L. M. Mulligan. 1996. De novo
mutation of GDNF, ligand of the REWGDNFR-a receptor complex in Hirschsprung
disease. Hum Mol Genet. 52023-2026.
122. Mulligan, L. M., G. J. Matlashewski, H. J. Scrable, and W. K. Cavenee. 1990.
Mechanisms of p53 loss in human sarcomas. Pruc. Natl. Acad Sci. USA. 87:5863-5867.
123. Koufos, A., M. F. Hansen, B. C. Lampkin, M. L. Workman, N. G. Copeland, N.
A. Jenkins, and W. K. Cavenee. 1984. Loss of alleles at loci on human chromosome 11
during genesis of Wilms' turnour. Nature. 309: 170- 172.
124. Chomczynski, P., and N. Sacchi. 1987. Single-step method of RNA isolation by
guanidiniium thiocyanate-phenol-chlom fom extraction. Analytical Biochemistry. 162: 156-
159.
L25. Sambrwk, I., E. F. Fritsch, and T. Maniatis. 1989. Molecular Cloning: A laboratory
manual. Cold Spring Harbor Laboratories, Cold Spring Harbor, New York
126. Rothenpieler, U. W., and G. R Dressier. 1993. P a - 2 is required for mesenchyme-
to-epithelium conversion during early kidney development Development. 1 l9:7 11-720.
127. Nakamura, T., Y. Ishizaka, M. Nagao, M. Hara, and T. Ishikawa. 1993. Expression
of the ret protwncogene in normal and neoplastic tissues. . Submitted,
128. Leong, S. S., I. S. Horoszewicz, K. Shimaoka, M. Friedman, E. Kawinski, M. I.
Song, R. Zeigel, T. M. Chu, S. B. Baylin, and E. A. Mirand. 1983. In Advances in
Thyroid Neoplasia M. Andreoli, F. Monaco, and I. Robbins, editors. Educational Italia,
Rome. 95-108.
129. Bracey, L. T., and IS. Paigen. 1987. Changes in translational yield regulate tissue-
specific expression of fbglucuronidase. Proc Natl Acad Sci USA. 84:9020-9024.
130. Bevilacqua, A., R. P. Erickson, and V. Hieber. 1988. Antisense RNA inhiiits
endogenous gene expression in mouse preimplantation embryos: lack of double-stranded
RNA "melting" activity. Proc Natl Acad Sci USA. 8583 1-835.
131. Morrison, C.. and F. Gannon. 1994. The impact of the PCR plateau phase on
quantitative PCR Biochim Biophys Acta. 12 l9:493-498.
132. Bunone, G., M. G. Borrello, R. Picetti, I. Bonganone, F. A. Peverali, V. de
Franciscis, G. Della Valle, and M. A. Pierotti. 1995. Induction of RET protwncogene
expression in neuroblastoma cells preceded neuronal differentiation and is not mediated by
protein synthesis. E*p CeN Res. 2 l7:92-99.
133. Asai, NOT T. Iwashita, M. Matsuyama, and M. Takahashi. 1995. Mechanism of
activation of the ref proto-oncogene by multiple endocrine neoplasia 2A mutations. Mol
Cell BioL 15:1613-1619.
134. Califano, D., C. Monaco, G. De Vita, A. DIAlessio, N. A. Dathan, R. Possenti, G.
Vecchio, A, Fusco, MI Santoro, and V. de Franciscis. 1995. Activated RETmC
oncogene elicits immediate early and delayed response genes in PC12 cells. Oncogene.
1 l:lO7-L 12.
135. Santoro. M., R. U Melillo, M. Grieco, M. T. Bcrlingieri, G. Vecchio, and A.
Fusco. 1993. The TRK and RET tyrosine k i n a oncogenes cooperate with ras in the
neoplastic transformation of a rat thyroid epithelial cell line. CeN Growth Di# 4:77-84.
136. Liu X., Q. C. Vega, R A. Decker, A. Pandey, C. A. Worby, and J. E. Dixon.
1996. Oncogenic RE' receptors display different autophosphorylation sites and substrate
binding specificities. J Biol Chem. 27 1 5309-53 12.
137. Songyang, Z., K. L. Carraway, M. J. Eck, S. C. Harrison, R. A. Feldman, M.
Moharnmadi, I. Schlessinger, S. R Hubbard, D. P. Smith. C. Eng, B. A. J. Ponder, B.
I. Mayer, and L. C. Cantley. 1995. Cataytic specificity of protein-tyrosine kinases is
critical for selective signalling. Nature. 373 :S36-539.
138. Iwashita, T., H. Murakami, N. Asai, and M. Takahashi. 1996. Mechanisms of Ret
dysfunction by Hirschsprung mutations affecting its extracellular domain. Hum Mol Genet.
5: 1577- 1580.
139. Momson-Graham, K., and Y. Takahashi. 1993. Steel Factor and c-Kit Receptor.
From Mutants to a Growth Factor System. BioEssays. 1577-83.
140. Huff, V., and G. Saunders. 1993. Wilms tumor genes. Biochim Biophys Acta.
1 155:295-306.
141. Re, G. G., D. I. Hazen-Martin, D. A. Sens, and A. I. Gamin. 1994.
Nephroblastoma (Wilms' Tumor): a Model System of Aberrant Renal Development. Sem
Diag Pathol. 1 1 : 126-1 35.
142. Junien, C., and I. Henry. 1994. Genetics of Wilms' tumor: A blend of aberrant
development and genomic imprinting. Kidney International. 46: 1264- 1279.
143. Tay, J. 1995. Molecular genetics of Wilms' tumor. J Paediatr Child Health. 3 1 :379-
383.
144. Beckwith, I. B. 1986. W i ' tumor and other renal tumors of childhood. In
Pathology of Neoplasia in Children and Adolescents. M. Fiegold, editor. I B Lippincott,
Philadelphia. 3 13-332.
145. Wadey, R., N. Pal, B. Buckle. E. Yeomans, I. Pritchard, and J. Cowell. 1990. Loss
of heterozygosity in W i i ' tumor involves two distinct regions of chromosome 11.
Oncogene. 5 9 1-907.
146. Call, K. M., T. Glaser, C. Ito, A. I. Buckler, I. Pelletier, D. A. Haber, E. A. Rose.
A. Kral, H. Yeger, W. H. Lewis, C. Jones, and D. E. Housman. 1990. Isolation and
characterization of a zinc finger poiypeptide gene at the human chromosome 11 Wilms'
tumor locus. Celt. 60509-520.
147. Gessler, M., A. Poustka, W. K. Cavenee, R L. Neve, S. H. Orkin, and G. A. P.
Bruns. 1990. Homozygous deletion in W i turnours of a zinc-finger gene identified by
chromosome jumping. Nature. 343:774-778.
148. Haber, D. A., and D. E. Houseman. 1992. Role of the WT I gene in Wilms' turnour.
Cancer Surveys. 12: 105- 1 17.
149. Koufos, A., P. Grundy, K. Morgan, K. A. Aleck, T. Hadro, B. C. Lampkin, A.
Kalbakji, and W. K. Cavenee. 1989. Familial Wiedemann-Beckwith syndrome and a
second Wilrns tumor locus both map to 1 lp15.5. Am JHum Genet. 4471 1-719.
150. Ping, A. I., A. E. Reeve, D. I. Law, M. R. Young, M. Boehnke, and A. P.
Feinberg. 1989. Genetic linkage of Beckwith-Wiedemam syndrome to 1 lp 15. Am J Hum
Genet. U:720-723.
151. Wiedemann, H. R. 1983. Turnours and hemihypertrophy associated with
Wiedemann-Beckwith syudrome. Eur J Ped. 141: 129.
152. Hatada, I., H, Ohashi, Y. Fukushima, Y. Kaneko, M. Inoue, Y. Komoto, A. Okada,
S. Ohishi, A. Nabetani, H. Morisaki, M. Nakayama, N. Niikawa, and T. Mukai. 1996.
An imprinted gene ~ 5 7 ~ ~ ~ 2 is mutated in Beckwith-Wiedemann syndrome. Nature Genet.
14: 171-173.
153 Rahman, N., L. Arbour, P. Tonin, J. Renshaw, J. Pelletier, S. Baruchel, K.
Pritchard-Jones, M. R. Stratton, and S. A. Narod. 1996. Evidence for a familial WiIms'
tumour gene ( M I ) on chromosome 17q 12-2 1. Nature Genet. l3:46 1-463.
154. Tonin, P., E. Ehrenborg, G. Lenoir, J. Feunteun. H. Lynch, K. Morgan. H. Zazzi,
A. Vivier, M. Pollak, and H. Huynh. 1993. The human insulin-like growth factor-binding
protein 4 gene maps to chromosome region 17q12q21.1 and is close to the gene for
hereditary breast-ovarian cancer. Genomics. 1 8 :4 14-4 17.
155. Motzer, R. J., N. H. Bander, and D. M. Nanus. 1996. Renal Cell Carcinoma New
Engl J Med* 335:865-875.
156. Maher, E. R 1994. Von Hippel-Lindau Disease. Eur J Canc. 30: 1987- l9W.
157. Latif, F., K Tory, I. Gnarra, M. Yao, F.-M. Duh, M. L. Orcutt, T. Stackhouse, I.
Kuunin, W. Modi, L. Geil, L. Schmidt, F. Zhou, H. Li, M. H. Wei, F. Chen, G. Glenn,
P. Choyke, M. M. Walther, Y. Weng, D.4. R. &an, M. Dean, D. Glavac, F. M.
Richards, P. A. Crossey, M. A. Ferguson-Smith. D. LePaslier, I. Chumakov. D. Coben.
A. C. Cbinault, E. R. Maber, W. M. Linehan, B. Zbar, and M. I. Lerman. 1993.
Identification of the von Hippel-Lindau disease tumor suppressor gene. Science. 160 13 17-
1320.
158. Anglad, P., K. tory, H. Brauch, G. H. Weiss, F. Latif, M. J. Merino, M. I.
Lerman, B. Zbar, and W. M. Lineban. 1991. Molecular analysis of genetic changes in the
origin and development of renal cell carcinoma Canc Res. 5 1 : 107 1 - 107%
159. Tory, K., H. Brauch, M. Linehan, D. Barba, E. Oldfield, M. Filling-Katz, B . Seizinger, Y. Nakamura, R. White, F. Marshall, M. Lerman, and 8. Zbar. 1989. Specific
genetic change in tumors associated with von Hippel-Lindau disease. J Natl Cmtc Inst.
8l:lO97-llOl.
160. Kovacs, G., and S. Frisch. 1989. Clonal chromosome abnormaIities in tumor cells
from patients with sporadic renal cell carcinomas. Canc Res. 49:6S 1-659.
161. Seizinger, B. R., G. A. Rouieau, L. J. Ozelius, A. H. Lane, G. E. Farmer, I. M.
Lamiel, J. Haines, J. W. Ywns, D. Collins, and J. Majoor-Krakauer. 1988. Von Hippel-
Lindau disease maps to the region of chromosome 3 associated with renal cell carcinoma.
Nature. 3 32:268-269.
162. Crossey, P. A., E. R. Maher. M. H. Jones, F. M. Richards, F. Latif, M. E. Phipps,
M. Lush, K Foster, K. Tory, I. S. Green, B. Oostra, J. R. W. Yates, W. M. Linehan,
N. A. Affara, M. Lerman, B. Zbar, Y. Nakamura, and M. A. Ferguson-Smith. 1993.
Genetic Linkage between Von Hippel-Lindau disease and three microsatellite
polymorphism refmes the localization of the VHL locus. Hum Mol Genet. 2 (3):279-282.
163. Mocha, R., J. Ishikawa, M. Tsutsumi, K. Hikiji, Y. Tsukada, S. Kamidono, S.
Maeda, and Y. Nakamura. 1991. Melotype of renal cell carcinoma Cmu: Res. 51:820-
823.
164. Morita, R., S. Saito, J. Ishikawa, 0. Ogawa, 0. Yoshida, K. Yamakawa, and Y.
Nakamura. 1991. Common regions of deletion on chromosomes Sq, 6q and 10q in renal
cell carcinoma. Canc Res. 5 158 17-5820.
165. Salomon, R., T. Attie, A- Pelet, C. Bidaud. C. Eng, J. Amiel, S. Samacki, 0.
Godet, C. Ricour, C. Nioul-Fekktti, A. Munnich, and S. Lyomet. 1996. Germline
mutations of the RET ligand, GDNF, are not sufficient to cause Hirschsprung disease.
Nature Genet. 14:345-347.
166. Donovan, M. J., B. Hempstead, L. I. Huber, D. Kaplan, P. Tsoulfas, M. Chao, L.
Parada, and D. Schofield. 1994. Identification of the newotrophin receptors p75 and trk in
a series of Wilms' tumors. Am J Pathol. 145:792-80 1.
167. Durbeej, M., S. Soderstrom, T. Ebendal, T. Birchmeier, and P. Ekblom. 1993.
Differential expression of neurotmphin receptors during renal development. Development.
119:977-989.
168. Tessarollo, L., P. Tsoulfas, D. Martin-Zanca, D. Gilbert, N. Jenkins, N. Copeland,
and L. Paracia, 1993. ukC, a receptor for neurotrophin-3, is widely expressed in the
developing nervous system and in non-neural tissues. Development. 1 18:463-475.
169. Huff, V., H. Miwa, D. A. Haber, K. M. call, D. Housman, L. C. Strong, and G. F.
Saunders. 199 1. Evidence for WT1 as Wlms tumor (WT) gene: -genic germinal
deletion in bilaterd WT. Am J Hum Genet. 48:997-1003.
170. Maw, M., P. E. Grundy, L. J. Millow, M. R. Eccles, R. S. Dunn, P. I. smith, A. P.
Feinberg, D. J. Law, M. C. Paterson, P. E. Telzerow, D. F. Callen, A. D. Thompson, R.
I. Richards, and A. E. Reeve. 1992. A third Wilms' tumor locus on chromosome 16q.
Cane Res:3094-3098.
171. Eccles, M. R., L. J. Wallis, A. E. Fidler, N. K. Spurr, P. I. Goodfellow, and A. E.
Reeve. 1992. Expression of the PAX2 gene in human fetal kidney and Wilms tumor. Ceil
Growth Diff. 3~279-289.
172. Poleev, A., H. Fickenscher, S. Mundlos, A. Winterpacht, B. Zabel, A. Fidler, P.
Gruss, and D. Plachov. 1992. PAX8, a human paired box gene: isolation and expression
in developing thyroid kidney and Wi' tumor. Development. 1 l6:6 1 1-623.
173. Eccles, M. R., K. Yun, A. E. Reeve, and A. E. Fidler. 1995. Comparative in siru
hybridization analysis of PAX2, PAX8 and WTI gene transcription in human fetal kidney
and Wilms' tumors. Am J Puthol. 146:40-45.
174. Weiss, L. M., A. B. Gelb, and L. J. Medeiros. 1995. Adult renal epithelial
neoplasms. Am J Clin Pathol. 103:624-635.
175. Gnarra, I. R., K. Tory, Y. Weng, L. Schmidt, M. & Wei, H. Li, F. Latif, S. Liu,
F. Chen, F.-M. Duh, I. Lubensky, D. R. Duao, C. Florence, R. Pouatti, M. M. Walther,
N. H. Bander, H. D. Grossman, H. Brauch, S. Pomer, J. D. Brooks, W. B. Isaacs, M. I.
Lerman, B. Zbar, and W. M. Linehan. 1994. Mutations of the VHL tumour suppressor
gene in renal carcinoma. Nature Genet. 7:85-90.
L76. Foster, K., A. Prowse, A. van den Berg, S. Fleming, M. M. Hulsbeek, P. A.
Crossley, F. M. Richards, P. Cairns, N. A. Affrara and M. A. Ferguson-Smith. 1994.
Somatic mutations of the von Hippel-Lindau disease tumour suppressor gene in non-
farnilid clear cell rend carcinoma, Hum Mol Genet. 3:2l69-2 173.
177. Heman, J. G., F. Latif. Y. Weng, M. I. Lennan, B. Bar, S. Liu. D. Samid, D . 4 .
R. Duan, I. R. Gnarra, W. M. Linehan, and S. B. Baylin. 1994. Silencing of the VHL
tumor-suppressor gene by DNA methylation in rend carcinoma Pruc Nut1 Acad Sci USA.
9 139700-9704.
178. Kessier. P. M., S. P. Vasavada, R. R. Rackley, T- Stackhouse, F.-M. Dub, F. Latif,
M. I. Lerman, B. Zbar, and 8. R. G. Wfiams. 1995. Expression of the Von Hippel-
Lindau Tumor Suppressor Gene, VHL, in Human Fetal Kidney and During Mouse
Embryogenesis. Mol Med. 1 :457-466.
179. Palmer, M., A. Dryden, I. Hughes, and J. Collinge. 1991. Homozygous prion
protein genotype predisposes to sporadic Creuafeldt-Jakob disease. Nature. 3S2:3480-34 1.
180. Brown, P.. L. G. Goldfarb, C. I. Gibbs, and D. C. Gajdusek. 1991. The phenotypic
expression of different mutations in transmissible familial Creutzfeldt-Jakob disease. Eur J
Epidemiol. 7:469-476.
181. Brown, P., L. Cemenkova, L. G. G~ldfarb~ W. R. McCombie, R. Rubinstein, R.
G. Will, and M. Pocchiari. 1994. Iatrogenic Creuafeldt-Jakob disease: an example of the
interplay between ancient genes and modem medicine. Neurology. W 2 9 1-293.
182. Windl, 0.. M. Dempster, I. P. Estibeiro, R Lathe, R. de Silva, T. Esmonde, R.
Will. A. Springbett, T. A. Campbell, K C. L. Sidle. M. S. Palmer, and J. Collinge.
1996. Genetic basis of Creutzfddt-Jakob disease in the United Kingdom: a systematic
analysis of predisposing mutation and aUelic variation in the PRNP gene. Him Genet.
98:259-264.
183. Medori. EL, H. J. Tritschler, A. LeBIanc, F. Villare, V. Manetto, H. Y. Chen, R.
Xue, S. Leal, P. Montagna, and P. Cortelli. 1992. F a d familial insomnia, a prion disease
with a mutation at codon 178 of the prion protein gene. New Engl J Med. 326:444-449.
184. Medori, R., P. Montagna, H. I. Tritschler, A. LeBlanc, P. Cortelli, P. Tinuper, E.
Lugaresi, and P. Gambetti. 1992. Fatal familial insomnia: a second kindred with mutation
of prion protein gene at codon 178. Neurology. 42:669-670.
185. Petersen, R. B., M. Tabaton, L. Berg, S. Schrank, R. M. Torack, S. Leal, I. Mien,
C. Vital, B: Deleplanque, and W. W. Pendiebury. 1992. Analysis of the prion protein gene
in thdatuic dementia. Neurology. 42: 1859- 1863.
186. Goldfarb, L. G.. M. Haltia, P. Brown, A. Nieto, I. Kovanen, W. R. McCombie, S.
Trapp, and D. C. Gajdusek. 1991. New mutation in scrapie amyloid precursor gene (at
codon 178) in F i s h Creutzfeldt-lakob kindred. Luncet. 337:425.
187. Petersen, R. B., L. G. Goldfarb, M. Tabaton, P. Brown, L. Monari, P. Cortelli, P .
Montagna, L. Autilio-Gambetti, D. C. Gajdusek, E. Lugaresi, and P. Gambetti. 1994. A
Novel Mechanism of Phenotypic Heterogeneity Demonstrated by the Effect of a
Polymorphism on a Pathogenic Mutation in the PRNP (Rion Protein Gene). Mol
Neurobiol. 8:99- 103.
188. Williams, D. E., J. Eisenmann, A. Baird, C. Rauch, K. Van Ness, C. J. March, L .
S. Park, U. Martin, D. Y. M~~hizuki , H. S. Bosweil, G. S. Burgess, D. Cosman, and S .
D. Lyman. 1990. Identification of a ligand for the c-kit proto-oncogene. Cell. 63: 167474.
189. Chabot, B., D. A. Stephenson, V. M. Chapman. P. Besmer, and A. Bernstein.
1988. The proto-oncogene c-kit encoding a transmembrane tyrosine kinase receptor maps
to the mouse W locus. Nature. 335%-89.
190. Zsebo, K. M., D. A. Williams, E. N. Geissler, V. C. Broudy, F. H. Martin, H. L.
Atkins, E2.X Hsu, N. C. Birkett, K H. Okino, D. C. Murdock, F. W. Jacobsen, K. E.
Langley, K. A. Smith, T. Takeishi, B. M. Cattanach, S. I. Galli, and S. V. Suggs. 1990.
Stem cell fa~tor is encoded at the Sl locus of the mouse and is the Ligand for the c-kit
tyrosiw kinase receptor. Cell. 63 :2 13-224.
19 1. Geibel, L. B ., and R. A. Spritz. 199 1. Mutation of the KIT (mastktem cell growth
factor receptor) protwncogene in human piebaldism, Proc Natl Acod Sci USA. 88:8696-
8699.
192. FIeischma~l~l, R. A., D. L. Saltman, V. Stastny, and S. Zneimer. 199 1. Deletion of
the c-kit proto-oncogene in the human developmental defect piebald trait. Pruc Nati A c d
Sci USA. 88: 10885-10889.
193. Angrist, M., S. Bolk, M. Halushka, P. A. Lapchak, and A. Chakravarti. 1996.
Germline mutations in glid cell line-derived neurotrophic factor (GDNF) and RET in a
Hirschspmg disease patient. Nature Genet. l M 4 1-343.
194. Edery, P., T. Attie, J. Amiel, A. Pelet, C. Eng, R. M. W. Hofstra, H. MarteIli, C.
Bidaud, A. Munnich, and S. Lyonnet. 1996. Mutation of the endothelin-3 gene in the
Waardea burg-Hirschsprung (Shah- Wwden burg syndrome). Nature Genet. L 2:442-444.
195. Hofstra, R. M. W., J. Osinga, G. Tan-Sindhunata, Y. WU, E.4. Karnsteeg, R. P.
Stulp, C. van Ravenswaaij-Arts, D. Majwr-Krakauer, M. Angrist. A. Chakravarti. C.
Meijers, and C. H. C. M. Buys. 1996. A homozygous mutation in the endothelin-3 gene
associated with a combined Waardenburg type 2 and Hirschsprung phenotype (Shah-
Waardenburg syndrome). Nature Genet. 12:445-447.
196. Mulligan, L. M.. E. GXdne~, B. A. Smith, C. G. P. Mathew, and B. A. J. Ponder.
1993. Genetic events in tumour initiation and progression in multiple endocrine aeopiasia
type 2. Genes Chrum Cane. 6: 166-177.
L97. Romano. A*, W. T. Wong, M. Santoro, P. J. Winh, S. S. Thorgeirsson, and P. P.
DiFiore. 1994. The high transforming potency of erbB-2 and ret is associated with
phosphorylation of paxiilin and a 23 kDa protein. Oncogene. 9:2923-2933.
198. Borrello, M. G., D. P. Smith, B. Pasini. I. Bonganone. A. Greco, M. I. Lorenzo,
E. Arighi, C. Mirancia, C. Eng, L. Alberti, R. Bocciardi, P. Mondellini, L. Scopsi, G.
Romeo, B. A. i. Ponder, and M. A. Pierotti. 1995. RET activation by germline MEN2A
and MEN28 mutations. Oncogene. 11:2419-2427.
199. Pawson, T. 1995. Protein modules and signalling networks. Nature. 373573-580.
200. Pandey, A., D. F. Lazar, A. R. Sdtiel, and V. M. Dixit. 1994. Activation of the Eck
receptor protein tyrosine kinase stimulates phosphatidylinositol 3-kinase activity. J Bioi
Chem. 269330 154-30157.
201. Mama, H., and A. Burgess. 1994. Regulation of the Ras signalling network.
BiuEssuys. 16:489-496.
202. Vega, Q., C. Worby, M. Lechner, J. Dixon, and G. Dressier. 1996. Glial cell Iine-
derived neurotrophic factor activates the receptor tyrosine base REX and promotes kidney
morphogenesis. Proc Natl Acad Sci USA. 93: 10657- LO66 1.
203. Puffenberger, E., E. buffman, S. Bok, T. Matise, S. Washington, M. Angrist, I.
Weissenbach, K. Garver, M. Mascari, R. Ladda, S. Slaugenhaupt and A. Chakravarti.
1994. Identity-by-descent and association mapping of a recessive gene for Hirschsprung
disease on chromosome 13q22. Hum Mol Genet. 3: 12 17- 1225.
204. Puffenberger, E. G., K. Hosoda, S. S. Washington, K. Nakao, D. de Wit, M.
Yanagisawa, and A. Chakravarti. 1995. A missense mutation of the endothelin B receptor
gene in multigenic Hirschsprung's disease. Cell. 79: 1257- 1266.
Appendix 1
Solutions
LOOX Denhardt's
2SX SSC
LOX TBE
LOX TPE
sequencing gel mix
2% bovine serum albumin 2% (wh) Ficoll400 2% (w/v) po~yvinylpyro~do~
3.7M sodium chloride 0.4M uisodium citrate-2H20 *pH 7.4
0.9M Tris 0.9M boric acid 2- EDTA
0.9M Tris 0.0 1% orthophosphoric acid 2OmMEDTA
7M urea 5% acrylamide 0.25% (w/v) NN methyl bis acrylamide 1X TBE
denaturing GLB 95% deionized formamide 20mM EDTA 0.05% bromophenol blue 0.05% xylene cyan01
lOX Sigma GLB 40% sucrose O.1M EDTA 0.5% sodium dodecyl sulphate 0.0556 bromophenol blue
Rehybridization Buffed 6X SSC Hybridization Buffer 0.1% SDS
5X Denhardt's solution 100pg/mL sheared, denatured heterologous DNA
10X PNK Buffer ~OIIIM Tris-HC1 (pH 7.6) MgQ
5mM IYIT lOOmM spermidhe-HCl L O W EDTA (pH 8 -0)
10X RT Buffer
10X PCR Buffer lOmM Tris-HCl (pH 8.3) SOmM KCI 0.0 1 % gelatin 0.75- 1 .75mM MgClz