Histological evaluation of extracellular matrix profile ...
Transcript of Histological evaluation of extracellular matrix profile ...
Histological evaluation of extracellular matrix
profile during sciatic nerve regeneration
Tobias KRETSCHMER
Verhandeling ingediend tot
het verkrijgen van de graad van
Master in de Biomedische Wetenschappen
Promotor: Prof. Dr. M. Cornelissen
Begeleiders: Dr. Victor Carriel, Charlot Philips
Vakgroep: Medische basiswetenschappen
Academiejaar 2014-2015
Histological evaluation of extracellular matrix
profile during sciatic nerve regeneration
Tobias KRETSCHMER
Verhandeling ingediend tot
het verkrijgen van de graad van
Master in de Biomedische Wetenschappen
Promotor: Prof. Dr. M. Cornelissen
Begeleiders: Dr. Victor Carriel, Charlot Philips
Vakgroep: Medische basiswetenschappen
Academiejaar 2014-2015
“De auteur en de promotor geven de toelating deze masterproef voor consultatie
beschikbaar te stellen en delen ervan te kopiëren voor persoonlijk gebruik. Elk ander
gebruik valt onder de beperkingen van het auteursrecht, in het bijzonder met betrekking
tot de verplichting uitdrukkelijk de bron te vermelden bij het aanhalen van resultaten
uit deze masterproef.”
Datum: 08/05/2015
Tobias Kretschmer Prof. Dr. M. Cornelissen
Voorwoord
Alvorens deze masterproef aan te vangen, zou ik graag een woord van dank betuigen aan enkele
mensen in het bijzonder. Deze mensen hebben het op verschillende manieren mogelijk gemaakt
om deze masterproef te realiseren:
Mijn promotor, Professor Cornelissen voor het mogelijk maken van deze masterproef, haar
kennis die zij aan mij heeft doorgegeven, haar begeleiding tijdens het laatste anderhalf jaar en
het ter beschikking stellen van haar labo en materialen. Ik ben uiterst dankbaar voor de tijd die
zij nam om mijn thesis te lezen, haar feedback en bondige gesprekken waarvan ik veel heb
kunnen leren.
Mijn begeleider, Victor Carriel die mij een groot aantal vaardigheden in het labo heeft
aangeleerd, die mij veel materiaal en tijd ter beschikking stelde en mij steeds met zijn expertise
bijstond om mijn wetenschappelijk onderzoek op een correcte manier uit te voeren. Verder ben
ik hem zeer dankbaar voor zijn feedback en begeleiding tijdens het schrijven van deze
masterproef.
Leen Pieters, de persoon die mij tips kon geven over elk onderwerp betreffende het praktische
werk in het labo. Ondanks het feit dat ze het zelf druk had, kreeg ik op elk moment en elke
vraag steeds een antwoord dat mij hielp om mijn doelen te bereiken.
De doctoraatstudenten, in het bijzonder Charlot Philips, voor haar vele tips en feedback op de
schriftelijke delen die uiteindelijk in deze thesis werden opgenomen. Zij nam de tijd om mij
grondige feedback te geven en was zo voor mij een enorme hulp tijdens het schrijven.
Ten slotte ben ik uiterst tevreden over de vele interessante en vriendelijke mensen met wie ik
in het laatste anderhalf jaar gewerkt heb op het labo. Er was altijd een vriendelijke en
aangename sfeer die zeker ook heeft bijgedragen aan mijn enthousiaste manier om deze
masterproef te realiseren.
Table of contents
Samenvatting .......................................................................................................................... 1
Abstract .................................................................................................................................... 2
1. Introduction ........................................................................................................................ 3
1.1 THE NERVOUS SYSTEM. .................................................................................................... 3
1.2 THE PERIPHERAL NERVOUS SYSTEM. .............................................................................. 3
1.2.1 Morphology of the PNS. ...................................................................................................................... 3
1.2.2 Schwann cells and myelination. .......................................................................................................... 4
1.2.3 The extracellular matrix (ECM) of the PNS....................................................................................... 5
1.2.4 Collagens in the ECM. ........................................................................................................................ 6
1.2.5 Proteoglycans in the ECM. .................................................................................................................. 6
1.2.6 Histological assessment of the PNS. ................................................................................................... 8
1.3 DEGENERATION AND REGENERATION OF THE NERVOUS SYSTEM. ................................. 8
1.4 CLINICAL ASPECTS. ........................................................................................................ 11
1.5 HYPOTHESIS AND OBJECTIVES. ..................................................................................... 11
2. Material and methods .................................................................................................... 12
2.1 EXPERIMENTAL ANIMALS. ............................................................................................. 12
2.2 TISSUE PROCESSING FOR HISTOLOGICAL ANALYSIS. .................................................... 13
2.2.1 Fixation of the tissues. ....................................................................................................................... 13
2.2.2 Paraffin embedding, sectioning and mounting. ............................................................................... 13
2.3 ROUTINE STAINING AND HISTOCHEMISTRY. ................................................................. 14
2.3.1 Hematoxylin and eosin. ..................................................................................................................... 14
2.3.2 Histochemistry with MCOLL. ........................................................................................................... 15
2.4 IMMUNOHISTOCHEMICAL ANALYSES. ........................................................................... 16
2.4.1 Antigen retrieval. ............................................................................................................................... 17
2.4.2 IHC protocols. .................................................................................................................................... 18
3. Results ............................................................................................................................... 19
3.1 H&E STAINING............................................................................................................... 19
3.2 MCOLL HISTOCHEMICAL METHOD. ............................................................................ 21
3.2.1 Myelin and collagen in autograft repaired nerves. ........................................................................... 25
3.2.2 Myelin and collagen in conduit repaired nerves. .............................................................................. 27
3.3 COLLAGEN I IHC. .......................................................................................................... 29
3.4 COLLAGEN III IHC. ....................................................................................................... 33
3.5 DECORIN IHC ................................................................................................................ 37
3.6 VERSICAN, FIBROMODULIN AND BIGLYCAN IHC. ......................................................... 41
4. Discussion and conclusion .......................................................................................... 43
Acknowledgment ................................................................................................................. 48
5. Bibliography ..................................................................................................................... 48
6. Addendum
6.1 IMMUNOHISTOCHEMISTRY – COLLAGEN I
6.2 IMMUNOHISTOCHEMISTRY – COLLAGEN III
6.3 IMMUNOHISTOCHEMISTRY – DECORIN
6.4 IMMUNOHISTOCHEMISTRY – VERSICAN
6.5 IMMUNOHISTOCHEMISTRY – FIBROMODULIN
6.6 IMMUNOHISTOCHEMISTRY – BIGLYCAN
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Samenvatting
Achtergrond: Perifere zenuwen zijn in staat om over korte afstanden terug aan elkaar te
groeien en verschillende componenten uit de extracellulaire matrix spelen hierbij volgens recent
wetenschappelijk onderzoek een belangrijke rol. Tot nu toe zijn de samenstelling, verdeling en
herschikking van deze ECM componenten tijdens zenuwregeneratie nog niet goed gekend. Het
doel van deze studie is de evaluatie van het ECM profiel tijdens de regeneratie van de nervus
ischiadicus van de rat.
Methoden: De zenuwen werden doorgesneden om een 5 mm defect te introduceren dat
vervolgens werd verbonden via een autograft of een bio-artificiële conduit. Na 20, 30 en 50
dagen werden de zenuwen verzameld. De histologische analyses werden uitgevoerd door
gebruik te maken van hematoxylin en eosine (H&E), de MCOLL histochemische methode en
immuunhistochemie (IHC) kleuringen. Door deze laatste werden de expressie en herschikking
van collageen type I en III, decorin, versican, fibromodulin en biglycan geanalyseerd.
Resultaten: Aan de hand van de H&E kleuring werd de toestand van regenererende axonen in
autograft behandelde zenuwen en van nieuw gevormde axonen in conduit behandelde zenuwen
bepaald en de progressie van axon regeneratie geëvalueerd. Door middel van de MCOLL
kleuring kon de graad van myelinisatie en de collageen herschikking in proximale, centrale en
distale zenuwuiteinden bepaald worden. De IHC kleuringen toonden aan dat collageen I en III
in het perineurium en endoneurium tot expressie kwamen en een soort omhulsel voor de
regenererende axonen vormden. Decorin kwam in nauwe associatie met het collageen tot
expressie. Versican, fibromodulin en biglycan kwamen niet tot expressie.
Conclusies: Dit onderzoek heeft nieuw inzicht geleverd in de verdeling en herschikking van
verschillende componenten van de ECM in zenuwen die op twee verschillende manieren
gerepareerd werden. Tijdens de regeneratie is er een duidelijk verschil in de herschikking van
de ECM proteïnen en het gebruik van een conduit kon deze structurele herschikking
bevorderen.
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Abstract
Background: Peripheral nerves possess the ability to regenerate over short distances after
transection and recent studies suggest that various extracellular matrix (ECM) components
contribute to the regeneration of these nerves. However, the precise composition, distribution
and reorganization of different ECM components are still largely unknown. This study aims at
evaluating the ECM profile during sciatic nerve regeneration in rat sciatic nerve (SN).
Methods: The rats were implanted with an autograft or a bioartificial conduits after a 5 mm
gap was induced in one SN. Nerve samples were harvested at 20, 30 and 50 days after
implantation. The histological analyses were carried out using H&E staining, the MCOLL
histochemical method and immunohistochemistry (IHC). By immunohistochemical means, the
expression and organization of collagen type I and III, decorin, versican, fibromodulin and
biglycan were analyzed.
Results: Based on the H&E staining the presence of regenerating axons in autograft repaired
nerves and newly-formed axons in conduit repaired nerves were observed and the progression
of axonal regeneration was evaluated. MCOLL results provided information on the degree of
myelination and collagen organization in proximal, central and distal nerve ends. The IHC
revealed collagen I and III expression in the perineurial and endoneurial space forming sheaths
around regenerating axons. Decorin was found in close association with these collagens. There
was no expression found of versican, fibromodulin and biglycan.
Conclusions: New information was obtained on the distribution and organization of several
proteins in the ECM in both types of nerve repair at different time intervals. The regeneration
process showed different characteristics regarding the ECM components’ organization and
indicated advantages for structural SN regeneration when using the conduit repair.
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1. Introduction
1.1 The nervous system. The nervous system of mammals is extremely complex from
a structural and functional point of view. It can anatomically and functionally be divided into
two different parts, i.e. the central and the peripheral nervous system. The central nervous
system (CNS) is subdivided into the brain and the spinal cord where, among other processes,
motor stimuli arise and sensory information and stimuli are processed and integrated (1). On a
macroscopic view the CNS consists of white and grey matter. The grey matter comprises mainly
unmyelinated axons which transmit the nerve stimuli, nerve cell bodies and dendrites. The
white matter comprises mainly myelinated axons and only very few cell bodies.
The supportive cells of the CNS are the glial cells, further subdivided into microglia and
macroglia. The microglia represent the immune cells of the CNS, specialized monocyte-derived
and antigen-presenting cells, which constitute a minority of all CNS cells. The macroglia cells
are the astrocytes, oligodendrocytes, ependymal cells and radial glial cells. Astrocytes are
regulatory cells and important for the neuronal environment and probably also serve as
predominant compartment of the blood-brain barrier. Oligodendrocytes perform the task of
myelin sheath production around the axons in the CNS. Ependymal cells are associated with
the cerebrospinal fluid production and secretion while forming a connection between blood and
cerebrospinal fluid in the form of a blood-cerebrospinal fluid barrier. Lastly, radial glial cells
play a role in nerve development and in the cerebellum and retina of the mature brain (2).
1.2 The peripheral nervous system. In the peripheral nervous system (PNS),
structures and cells are different and the major task of the PNS is to link the communication
between organs, tissues and the CNS (1). Peripheral nerves (PN) are found throughout the entire
body, emerging from the CNS and reaching almost every organ and all tissues. They provide
sensory, motor and autonomic innervation which is necessary for the complex functions of each
organ. In general, sensory nerve fibers originate from pseudo-unipolar neurons which are
located in the sensory ganglia, except for cranial nerve VIII and the mesencephalic root of
cranial nerve V. Motor nerve fibers have their origin in somatic and autonomic motor neurons
which are found in the CNS. Additionally, mixed nerves are the third group of nerves in the
general classification (2) (3).
1.2.1 Morphology of the PNS. PN are subdivided into two components that can be
recognized, a parenchyma and stroma. The parenchyma comprises the nerve fibers with their
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axons and Schwann cells while the stroma is made up of various connective tissue elements.
Compound nerve trunks and nerve fibers contain many nerve fascicles which are bound
together by a connective tissue layer called epineurium (3). Figure 1 gives a general schematic
overview of the structures and morphology of a PN. The epineurium is the outermost layer of
PN and delineates the nerve from the surrounding tissue. Epineurium comprises mainly
collagen and some adipose tissue and within the epineurium blood vessels are present and
fibroblasts and mast cells can be found. Surrounding the individual nerve fascicles is the
perineurium which consists of thin but dense sheath of collagen layers organized in bundles
that separate concentric layers of flattened cells. Underneath the perineurium, nerve fiber axons,
their surrounding Schwann cells, collagen fibers, fibroblasts, capillaries and few mast cells are
present in a connective tissue compartment called the endoneurium. The space which is
surrounded by the perineurium is called the endoneurial space. Perineurial cells separate the
endoneurial space from the interstitium via tight junctions. In the endoneurial space, capillaries
are present whose endothelium functions as blood-nerve barrier (3) (4).
1.2.2 Schwann cells and myelination. Axons are associated with Schwann cells which
wrap around their respective axon and produce the myelin sheath in a spiral way around an
individual axon. The myelinated portions are termed internodes and they are separated by
unmyelinated regions which display ion-channels and are termed nodes of Ranvier (3) (5).
Schwann cells thus offer support for axons by insulating them with myelin sheaths which
Figure 1: Schematic structure and components
of a peripheral nerve (58).
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basically consist of layers of phospholipid membranes. An advantage of the myelin insulation
is that signal transduction is enhanced through saltatory conduction (6).
In contrast to oligodendrocytes in the CNS, which produce myelin sheaths for more than
one axon, Schwann cells only ensheath part of one axon. However, non-myelinated axons are
also associated with Schwann cells, usually several axons enveloped as a group by a single
Schwann cell. Non-myelinated axons are usually smaller than myelinated axons and action
potential velocity is lower in the non-myelinated axons due to the fact that saltatory conduction
over nodes of Ranvier cannot occur (4).
Schwann cells derive from the neural crest which yields pluripotent cells that
differentiate under the influence of specific transcription factors. The association of Schwann
cells to developing peripheral nerves leads to their maturation in the PNS. As they maturate a
morphogenetic process called radial sorting is initiated which aims at combining Schwann cells
with large diameter and small diameter axons. The association in a 1:1 relationship of large
axon with Schwann cells will lead to myelination of the axon while small axons are not
myelinated and combine in groups around a non-myelinating Schwann cell. One of the factors
that plays a role in myelinating and non-myelinating Schwann cell development is NRG1-III
which is involved in neuregulin signaling. Furthermore, laminin which is present in the basal
lamina and interacts with certain receptors also influences myelinating Schwann cell
development (7) (8).
The contact between axons and Schwann cells is particularly important for the Schwann
cell growth and survival. Although these cells hardly divide in adult nerve tissue, cell division
is induced following nerve injury. After nerve transection, Schwann cells undergo
dedifferentiation from their myelinating state when contact to the axon is lost and turn into a
proliferative state. Due to the proliferation, the Schwann cells can remove debris together with
macrophages during Wallerian degeneration. Also, they will start to line up to form the so-
called bands of Büngner and secrete factors, such as laminin and fibronectin, to guide the
regenerating axons or axonal sprouts towards the distal nerve stump. In the absence of axon
contact and regeneration, the Schwann cells do not proliferate and the cell population decreases
by apoptosis (4) (9).
1.2.3 The extracellular matrix (ECM) of the PNS. The ECM is produced by different
cell types and provides the physical and chemical properties of different tissues. ECM
molecules are important from a structural point of view and they are even more important
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guiding the process of regeneration of PN. The ECM molecules provide strength and structure
to tissues, have a supportive role and also have influence on cell behavior. The latter is probably
achieved through precise spatial and temporal expression of ECM molecules and
transmembrane receptor interactions (5).
1.2.4 Collagens in the ECM. In PN, the ECM is highly organized and surrounds each
nerve fiber. Furthermore, a fibrillar matrix comprising collagen-based fibrils forms part of the
ECM. Collagens are extracellular, structural proteins synthesized mostly by fibroblasts.
Schwann cells in PN also produce collagen of the types I, III, IV and V. Collagens are composed
of high amounts of hydroxyproline, proline and glycine. They typically display a triple α-helical
configuration. Collagens are found in the endoneurium as fibrils of interstitial collagen and in
the basal lamina surrounding the processes of Schwann cells and perineurial cells as non-
fibrillar elements (10) (11) (12).
Following traumatic nerve injury, fibroblasts increase their production of collagen
around the injury site and distal to it. As a result, the tensile strength of the injured nerve is
enhanced and a collagenous framework for axon orientation and sheath formation by Schwann
cells is provided. Collagen types I and III are most important in regenerating nerves since they
play a vital role in the self assembly process of fibril formation (12). In the ECM, these fibrils
form scaffolds which increase the stability of the ECM, influence cell differentiation and
migration and interact with cellular receptors (8) (13). In some cases, the production of collagen
in the regenerating nerve is excessive and can lead to scar formation. Scarring can then prohibit
axonal sprouting and a successful regeneration of the nerve (14).
1.2.5 Proteoglycans in the ECM. Several ECM macromolecules are produced by
Schwann cells and neurons including collagens, glycoproteins and proteoglycans. These ECM
molecules are involved in important cellular processes including cell proliferation, migration
and differentiation (11). Proteoglycans are heterogeneous poly-peptides existing of a core
protein coupled to one or more glycosaminoglycan (GAG) side chains. These GAG chains are
basically long, unbranched polymers of repeating disaccharide units. GAGs can be divided into
5 broad classes based on their disaccharide content, i.e. chondroitin sulphate (CS), dermatan
sulphate (DS), keratan sulphate, heparan sulphate and hyaluronan. Many proteoglycans are
secreted to become part of the extracellular matrix, or they are attached to the extracellular side
of the cell membrane (15). Chondroitin sulphate proteoglycans (CSPG) are particularly
interesting because they are expressed in both developing and mature nerves and have been
reported to inhibit neurite outgrowth (5). When enzymes that degrade CSPG were added to a
graft or the distal nerve stump, the inhibitory effects of the proteoglycans were reduced (16).
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Biglycan belongs to the group of small proteoglycans and has 2 GAG side chains either
containing CS or DS or a combination of CS and DS side chains. It is found, for instance in
fetal or young bone as CSPG or in articular cartilage as DS containing form. The precise
functions of biglycan in different tissues remain to be elucidated, but it has been suggested that
it binds transforming growth factor-β (TGF-β) in vitro, influences bone mineralization and
binds to the growth factor BMP-4 which has effects on osteoblasts (13) (17). Biglycan is also
thought to interact with collagen type I, maybe in balance with decorin, and to help assembly
the ECM (18). However, in its purified form biglycan does not bind to collagen fibrils and it is
also not found in association with classic collagen bundles in tissues. The mRNA and protein
of biglycan are expressed in several types of cells in developing human tissues (13).
Decorin is a small proteoglycan containing a single CS or DS chain attached to the core
protein. The size of decorin can differ depending on the tissue where it is found and biglycan
in the same tissue is almost always bigger than decorin. It has been shown that decorin changes
the kinetics of collagen fibril formation and that it can bind to TGF-β and thereby neutralizes
its effect on certain cells (13). Recently, it has been reported that decorin plays an important
suppressive role in acute scar formation in the CNS through inhibition of inflammatory fibrosis
by contributing to the neutralization of TGF- β1/2. Further, decorin contributes to the induction
of tissue plasminogen activator and matrix metalloproteinase in chronic lesions which leads to
fibrolysis and reduction of grown scar tissue (19).
Fibromodulin belongs to the group of keratan sulphate proteoglycan which are
expressed in different connective tissues, e.g. cartilage, skin and tendon. The structure and
amino acid sequence of fibromodulin is related to those of the proteoglycans biglycan and
decorin (13). Additionally, decorin and fibromodulin seem to be involved in the assembly and
binding of collagen in the process of fibrillogenesis (20) (21). Fibromodulin is able to bind to
collagen type I and II, and also can impede collagen fibrillation in vitro which results in the
formation of thinner fibrils (13).
Versican is a relatively large CSPG of the ECM and is released by fibroblasts. There are
different isoforms of versican expressed in various tissues, including the CNS. All of these
isoforms contain regions to interact and bind with hyaluronic acid binding domain.
Furthermore, the V3 isoform possesses the ability to bind the EGF-receptor and isoform V2 can
cause the inhibition of neurite outgrowth in CNS and PNS neurons. Through the interaction
with the ECM via specific domains, versican has a regulatory effect on cell invasion and
metastasis. Versican, together with other proteoglycans, has been reported to have inhibitory
effects on axonal regeneration and neurogenesis in the CNS after injury (13) (22). Additionally,
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decorin and versican were found to be upregulated during mouse sciatic nerve regeneration and
it has been stated that these molecules decrease cell adhesion in different nerve cell lines (23)
(24).
1.2.6 Histological assessment of the PNS. Light microscopy is a frequently used
approach to observe and evaluate the morphological features of PN during pathophysiological
and regenerative processes. Observation of the multifarious histological appearance of cellular
and extracellular structures in PN is possible using light microscopy. However, depending on
the structure of interest and its presence and organization in the tissue, different methods of
staining can and should be applied.
Various histochemical methods allow for the identification of structures like myelin and
collagen. Toluidine blue and luxol fast blue (LFB) stain myelin with certain degree of accuracy
and specificity, but both methods also feature disadvantages. Applying toluidine blue on resin-
embedded, semi thin sections for example is more time-consuming and expensive than LFB
staining of 5 µm, paraffin-embedded sections. Furthermore, it was recently described that LFB
can be combined with the picrosirius method for simultaneous collagen staining to enhance
contrast and use less tissue sections compared to other approaches (25). Therefore, this new
method, called MCOLL method, provides a more comprehensive assessment for myelin and
collagen while being less time-consuming and less expensive.
On the other hand, several structures and molecules of the ECM are not recognized with
high accuracy or specificity through histochemical approaches. Regarding structures like ECM
proteoglycans, it seems to be more advantageous to use an immuno-histochemical approach.
Such approaches can be conducted on paraffin-embedded tissue sections of 5 µm which require
no specialized or expensive equipment (26). Immuno-histochemical protocols are usually
performed within one day, between 5 to 18 hours, depending on incubation times of the
antibodies. Furthermore, the antibodies display high potentials of specificity and accuracy
towards their respective target structure or molecule. Therefore, immunohistochemical
approaches are very useful in the assessment of histological structures which are relatively
difficult to stain using histochemical methods.
1.3 Degeneration and regeneration of the nervous system. In higher vertebrates, the
neuronal cell body can stay structurally intact for certain time and induce a regenerative
program if the neuron does not undergo cell death after transection of an axon in the CNS.
However, these regenerative efforts of the neuron are short-lived and rather unstable, ultimately
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resulting in atrophy or degeneration of the neuron (27). Furthermore, regeneration-inhibiting
properties of glial cells in the CNS are an essential reason for sprouting of axons over only
several millimeters in immediate surroundings of the neural lesion. Oligodendrocytes, for
instance, are cells which contribute to the axonal sprout inhibition by the production and
secretion of growth-inhibiting “Nogo” molecules which are part of the mature CNS (5) (27).
After transection of a PN, the processes occurring and the involved cellular structures
are different from those in the CNS. Figure 2 schematically summarizes several of the processes
and events taking place in PN during axonal degeneration and regeneration. Morphological
changes like chromatolysis, which entails nuclear and cell body swelling, occur several hours
after nerve injury. The neurons switch from producing neurotransmission-related substances to
a growing modus where syntheses of cytoskeletal and growth-associated proteins have priority.
In the proximal part of the transected nerve, axons degenerate over a short distance back from
the site of injury in a so-called retrograde degeneration. An axon of this proximal part then
starts producing a high number of collateral and terminal sprouts starting at the tip of the
remaining axon and advancing to a distal direction. The sprouts are orientated at the basal
lamina and occur within several hours after injury. A second wave of sprouts is observed within
the following two days and earlier sprouts can degenerate before the definitive sprouts are
formed. Schwann cells play an important role in guiding these sprouts physically over the nerve
injury gap. Schwann cells form processes that provide a rate-limiting step for axonal
regeneration, rather than axonal growth itself does. Nonetheless, the space between proximal
and distal nerve stump, the interstump zone, opposes the major barrier for nerve regeneration
and success of regeneration depends specifically on chemical and cellular events taking place
at this zone (9).
Distal from the nerve transection a highly regulated process called Wallerian
degeneration occurs at the injured site (28). This process is taking place 24 to 36 hours after
nerve transection. Macrophages are responsible for removal and breakdown of myelin debris
and therefore play a vital role in Wallerian degeneration. Furthermore, macrophages secrete
neurotrophins and interact with Schwann cells to promote axonal growth and nerve repair (29)
(30). After 5 to 20 days, regenerative changes in axons can easily be detected, for example by
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identification of the cytoskeletal proteins neurofilament, β-III tubulin and GAP-43 by
immunohistochemistry (IHC) (31).
Guiding axons during regeneration after PN damage is partly achieved by Schwann cell
basement membrane together with collagen fibers in the outer endoneurial sheath (32) (33).
Schwann cells can easily be identified in damaged nerves by the presence of an investing
basement membrane that is composed of laminin, fibronectin and other components (34).
Proliferation of Schwann cells in the endoneurial sheaths is a characteristic event which takes
place in the distal nerve stump after transection of a PN. It leads to the formation of so-called
bands of Büngner which resemble tightly packed columns of Schwann cells that aid in guiding
the regenerating axons to the periphery (35).
Regenerative changes and cellular events also take place in and are influenced by the
extracellular microenvironment (9) (10). Today, the general histological organizations of the
PN and several molecular aspects have been studied. However, there is still little known about
the expression, distribution and the role of the extracellular microenvironment in these complex
organs during regeneration.
Figure 2: Schematic representation of processes taking place during axonal degeneration and regeneration.
A. Normal peripheral nerve. B. Schwann cells comprise axon and myelin debris and have divided to form
bands of Büngner seven days after axonal injury. C. Axonal sprouts grow along the bands and proximal to
distal from the axon. D. Schwann cells are producing myelin around an axon. E. Reconnection of the axon
to its distal part with short regenerated internodes (57).
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1.4 Clinical aspects. The frequency of PN injuries is high and can cause different
degrees of structural damage and dysfunction of the PN (36). PN are long and delicate organs
and traumatic injuries occur frequently due to their vulnerability. When a PN is transected with
a short nerve gap, the direct repair, also called neurorrhaphy, is the surgeon’s method of choice.
In certain situations however, the direct repair is not possible, for instance when a direct repair
would set the repaired nerve under too much tension. In such cases, the surgeon can make use
of autologous grafts for reconstruction without tension on the injured nerve. Such autografts
can be obtained from a donor sensory nerve, e.g. sural nerve, or a combination of veins and
muscle tissue of the patient and therefore do not cause immunogenic reactions and provide a
favorable ECM with important factors for axon repair (36). Nonetheless, autografts also feature
some major disadvantages, for example donor site morbidity. This is the result of the fact that
the graft is taken from healthy tissue leaving behind a gap which is mostly not restored to its
original state and results in scar tissue formation. Further, autograft operations require more
time and are costly (36).
Under certain circumstances the use of a tubulization technique has more advantages
than direct or autograft repair of PN. Tubulization techniques with nerve conduits (NC) have
been established to guide the sectioned nerve fiber and to speed up and increase the number and
length of regenerating axons (37). After transection of a PN, the so-called nerve guidance
conduits are sutured to the proximal and distal ends of the nerve stumps that partially lie in the
conduit. Several phases comprising different cellular and extracellular events then take place in
the course of regeneration within the NC (38) (39). NCs are advantageous, because they spare
patients additional sutures and therefore reduce episodes of neuropathies which makes them
promising alternatives to classic direct repair. However, NCs are limited to nerve gaps of 30
mm and the incorporation of biomaterials, growth factors and ECM molecules to promote
regeneration still needs experimental analysis in terms of safety and efficiency (36). Knowledge
on ECM assembly may provide a better understanding of the complex process of nerve
regeneration. In addition, the knowledge of the role of these essential ECM molecules could
help us to develop better conduits used to support repair after PN injury (40) (41).
1.5 Hypothesis and objectives. We now know that the ECM influences and guides the
formation and elongation of nerve fibers. However, complex characteristics, properties and
promising features of the ECM are not fully described and demand further research. Additional
studies on regenerative changes at the axonal level could enhance a better understanding of the
events taking place during PN regeneration (9). From a clinical point of view, more knowledge
12
on regeneration-promoting NC can improve the treatment of many patients (36) (39). However,
manipulating the microcellular environment to enhance regeneration in PN is depending on a
better understanding of the factors and their interplay in the ECM (10) (42). The topographical
information obtained with histological techniques make it one of the most efficient methods to
elucidate the ECM profile during PN regeneration (3). Figure 3 shows a typical overview
staining of a PN to identify structures and the general morphology.
Due to the lack of information regarding the ECM profile in normal and regenerated
nerves, the aim of this study is to evaluate the ECM profile during sciatic nerve regeneration
by histochemical and immunohistochemical means. The goal is also to get a better insight into
the changes in composition, distribution and reorganization of the different components of the
ECM. It is hypothesized that the expression pattern of the different ECM molecules will display
similarities to what has already been described elsewhere for the process of PN regeneration
(3) (4) (43). However, the exact association of different cellular structures and ECM molecules
in the course of regeneration within several days to weeks remains to be determined as part of
this study.
2. Material and methods
2.1 Experimental animals. All animals used in this study were obtained from the
Service of Production and Animal Experimentation, University of Granada, with the approval
of the Ethics Committee of the University of Granada, Spain. The animals were kept in a
temperature controlled environment (21 +/- 1°C) which was maintained on a 12 hours light and
dark cycle and the animals were given free access to tap water and standard rat chow. Male
Wistar rats of 13 weeks old were used and subdivided into two groups. Under general
Figure 3: Hematoxylin and eosin staining of the rat sciatic nerve.
Important structures are highlighted and mentioned in the figure by
circles and arrows.
13
anesthesia, the first group of 8 animals was implanted with a collagen type I conduit
(NeuraGen®), 8 mm in length and 2 mm in diameter, after an incision was made to produce a
gap of 5 mm in the left sciatic nerve. The second group comprised another 8 animals which
underwent autograft repair of the left sciatic nerve after a similar incision as in the first group.
The right sciatic nerve in all animals was used as control tissue. 7/0 and 4/0 polypropylene
monofilament (Premilene®) sutures were used during surgery. Each animal was housed
individually after surgery and received metamizol in the drinking water. Euthanasia was
performed using an anesthetic overdose. Nerve tissues were harvested 20, 30 or 50 days after
conduit implantation or autograft repair.
2.2 Tissue processing for histological analysis. After the experimental animals were
euthanized, part of the regenerated sciatic nerve and control nerves were removed and had to
be treated in such a way that histological analysis could be conducted. To this end, tissues were
fixed, embedded and sectioned to obtain specimens for the analysis by different histochemical
and immunohistochemical techniques.
2.2.1 Fixation of the tissues. Formalin fixation is very common under pathologists and
the processes, advantages and disadvantages of formalin fixation are known. The general
structure of cellular organelles and peptide-protein bonds are primarily preserved with
formaldehyde fixation. Only little denaturation occurs and lipids and non-protein associated
carbohydrates are not fixed. Cross-links which mask epitopes and block antibody access can
occur (44) (45). In this work 10% formalin in 0,1M phosphate buffered saline (PBS) fixation
for 8 to 12 hours was selected for half of the control and experimental tissue samples.
The fixative methacarn was used for the other half of control and experimental tissue
samples. Methacarn is a modification of Carnoy’s fixative (10 ml acetic acid, 60 ml absolute
ethanol, 30 ml chloroform) where absolute ethanol is replaced with 100% methanol (44). In this
study, tissue sections were fixed in methacarn for 3,5 hours.
2.2.2 Paraffin embedding, sectioning and mounting. The goal of embedding the
tissues after fixation is to create a tissue block that can readily be cut in sections of varying
thicknesses. Embedding of the nerve samples was achieved by using paraffin wax as embedding
medium. Since paraffin is immiscible with water, the tissues have to be dehydrated using
increasing concentrations of ethanol and finally xylene or toluene which is ultimately replaced
by paraffin.
14
For sectioning, the paraffin blocks were put into a microtome (Cut 4060, SLEE Mainz,
Germany) to produce sections of a 5 µm thickness. The sections were transferred to a water
bath of 37 – 39°C and afterwards were transferred to microscope glass slides (Klinipath, Olen,
Belgium). Slides containing sections were then put into an oven at approximately 55°C for one
hour or alternatively at approximately 30°C overnight to dry. After drying, the slides can
theoretically be stored for months or years without the loss of tissues.
Before any staining could be carried out, the slides needed to be deparaffinated using
toluene (Chem-lab, Zedelgem, Belgium) first, decreasing concentrations of alcohol
(isopropanol, 99 vol.% and ethanol, 96 vol.%, Chem-lab) afterwards and finally, distilled water
(H2Od). In our study, an automated system (Microm HMS740, Walldorf, Germany) was used
to carry out deparaffination and dehydration at the beginning or end, respectively, of each
protocol. Table 1 shows the different steps of deparaffination and dehydration with the
respective solutions and rinse times. The last step after staining sections by means of
histochemical or immunohistochemical methods was mounting which was performed using
mounting medium (Richard-Allan Scientific).
Table 1: Deparaffination and dehydration as carried out by the automated system. The bath number in
chronological order, the solution and the time of rinse in the solutions are mentioned.
Deparaffination Dehydration
Bath Solution Time (minutes) Solution Time (minutes)
#1 Toluene 5’ Tap water 4’
#2 Toluene 5’ Ethanol 96% 2’
#3 Toluene 5’ Ethanol 96% 2’
#4 Isopropanol 2’ Isopropanol 2’
#5 Isopropanol 2’ Isopropanol 2’
#6 Ethanol 96% 2’ Toluene 2’
#7 Ethanol 96% 2’ Toluene 2’
#8 Tap water 2’ Toluene 1’
#9 Distilled water 1’ -
#10 Distilled water 1’ -
2.3 Routine staining and histochemistry. The goal of a routine stain is to highlight the
most important structures of a tissue and make it possible to differentiate these structures from
one another. The general reaction taking place is based on affinities of the dye for certain types
of molecules. Generally, two types of dyes are used for a routine staining, namely basic
(cationic) dyes and acidic (anionic) dyes.
2.3.1 Hematoxylin and eosin. One of the most famous routine stainings is hematoxylin
and eosin (H&E) staining which uses hematoxylin as basophilic and eosin as eosinophilic dye
15
(46). Eosin can be combined with phloxine to produce a cytoplasmic staining that is more
clearly demonstrating different tissue components than eosin solely. H&E stainings cause
nuclei to appear blue and cytoplasm and collagen fibers to appear red, thus providing a good
contrast between nucleus and cytoplasm of the cell (47). In this study, Hematoxylin (Mayer’s
hemalum solution, VWR®) and eosin + phloxine (Thermo Scientific) staining was used on all
tissue samples as routine staining. Hematoxylin alone was also used as counterstain following
histochemical and immunohistochemical stainings to provide a better overview and contrast in
the tissue samples.
2.3.2 Histochemistry with MCOLL. The recently described MCOLL histochemical
method is based on a combination of luxol fast blue (LFB) and picrosirius histochemical
methods and achieves simultaneous staining of myelin sheaths, collagen fibers in the stroma
and morphology pattern in CNS and PNS nerve tissues. LFB utilizes a copper phthalocyanine
dye which is attracted to basic groups in lipoproteins of the myelin sheath and is well-known
for myelin staining of formalin-fixed paraffin-embedded tissue sections (25) (48). A certain
peculiarity of the LFB protocol is the differentiation step where special attention is needed.
Differentiation aims at selectively withdrawing the dye in a solvent from the tissue and the dye
is usually first lost in structure with certain permeability, for example collagen. Therefore,
during differentiation slides can be placed under a light microscope to observe the loss of dye
in collagen structures and differentiation is stopped when this process is completed. Myelin
retains the dye significantly longer during differentiation and remains clearly visible and blue
colored (49). The subsequent use of picrosirius, i.e. Sirius red F3B in a saturated solution of
picric acid, aims at staining the collagen fibers. Sirius red, a strong anionic tetrakisazo dye,
interacts with cationic molecular groups, due to hydrogen bonding, present on collagen
molecules oriented in parallel and causes an intense red color of collagen fibers (50) (51).
In this study, 0,1% LFB (Color Index C.I. 74180, BDH Chemicals) in 95% ethanol
solution with 2,5 ml of 10% acetic acid (Chem-lab) was used and incubated overnight at 56°C.
Differentiation was performed in 0,05% lithium carbonate (E. Merck, Darmstadt, Germany).
Sections were also stained in 0,2% Sirius red F3B (C.I. 35780, Sigma-Aldrich) in a saturated
solution of picric acid, i.e. picrosirius solution, for 30 minutes at room temperature. Afterwards,
a counterstain was performed in hematoxylin (Mayer’s, VWR®). A protocol with the exact
steps, including rinse and washing after sections were stained, can be found in table 2.
16
Table 2: LFB staining and picrosirius staining together with other steps in the MCOLL histochemical method
protocol.
Step Procedure, solution and timing.
1 Deparaffinate sections in toluene twice, 99% ethanol 3 times, 95% ethanol 3 times, 70% ethanol twice,
á 2 minutes, and keep in distilled water afterwards.
2 Stain sections in 0,1% LFB at 56°C for 16–24 hours (overnight).
3 Rinse in 95% ethanol, then rinse and keep in distilled water.
4 Differentiate in 0,05% lithium carbonate until gray and white matter can be distinguished.
5 Rinse in 70% ethanol for 10 seconds, two changes. Then keep slides in distilled water to stop
differentiation.
6 Stain sections in picrosirius solution at room temperature for 30 minutes.
7 Rinse in distilled water for 3 minutes, two changes.
8 Counterstain with Mayer’s hematoxylin for 1 minute and 30 seconds. Wash under tap water afterwards
for 5 minutes.
9 Dehydrate sections in 96% ethanol twice, isopropanol twice and toluene 3 times, á 2 minutes.
10 Mount sections with mounting medium.
2.4 Immunohistochemical analyses. The basis of immunohistochemical methods is the
use of an antibody which binds to antigens in the target tissue. Figure 4 shows the concept and
structures involved in an IHC staining. The antigen is the structure of interest in the staining,
e.g. collagen type-I in a PN tissue section. The visualization of the primary antibody bound to
the antigen of interest is achieved by either direct or indirect means. For example, a fluorescent
dye molecule can be coupled to the primary antibody which therefore can directly be visualized.
However, this approach has less sensitivity compared to other methods and provides only little
signal amplification. Furthermore, a fluorescence microscope is required for the evaluation of
the stained sections. Using an indirect, histochemical approach where a secondary antibody
directed against the Fc-chain of the primary antibody is used, provides more sensitivity and
amplification of the signal. Even if this approach is more prone to errors, e.g. due to non-specific
binding of the secondary antibody, the amplification is very valuable for a clear and correct
analysis (46) (52). In this study, non-labelled primary antibodies and peroxidase-conjugated
secondary antibodies were used. Alternatively, biotinylated secondary antibodies and
streptavidin horse radish peroxidase (HRP) directed against the biotin-group were used. The
17
substrate for the peroxidase was 3,3’-diaminobenzidine (DAB) which is oxidized by peroxidase
resulting in a brown color at the site of reaction.
2.4.1 Antigen retrieval. One of the major disadvantages of formalin fixation and
paraffin embedding is the fact that these methods cause inter- and intramolecular cross-linking
of antigens of interest. These changes in three-dimensional structure can yield inappropriate
antigen-antibody interactions at the cost of unsatisfactory staining results. Therefore,
procedures and specific pretreatments have been tested and developed to increase
immunoreactivity of antigens in formalin-fixed tissues.
The first attempts to increase immunoreactivity utilized proteolytic enzymes which
digest molecules to re-expose hidden antibody binding-sites. Another approach used heat near
the boiling point of water with samples in citric acid buffer of pH 6 to further forward the
development of antigen “unmasking” or retrieval techniques. Important variables in these
techniques seem to be temperature, usually 95°C, and exposure time to this temperature varying
from 10 to 60 minutes. Cooling to room temperature after pretreatment is rather slow and might
take another 20 to 30 minutes. It is now clear that several cross-linkages can be reversed while
others stay intact and proteins thusly are not denatured by the heat which shows that antigen
retrieval indeed works (52).
In this study, several antigen retrieval treatments were used depending on the antigen of
interest for the IHC. For collagen I IHC staining of formalin-fixed sections pepsin (DAKO)
pretreatment was conducted. For collagen III IHC stainings of formalin-fixed sections
Figure 4: Simplified concept of an immunohistochemical staining. The primary antibody "1"
binds to a specific antigen "Ag" and a secondary antibody "2" binds the primary antibody. The
conjugated peroxidase "P" oxidizes DAB "D" to produce a brown reaction product.
18
pretreatment was conducted with citric acid buffer (E. Merck, Darmstadt, Germany) of pH 6,1
at 95°C in a steamer (Braun®) for 25 minutes. The proteoglycans were pretreated in
chondroitinase ABC 0,2 U/ml for one hour at 37°C. Chondroitinase ABC 0,2 U/ml was
prepared using 20 µl chondroitinase 5 U/ml (C3667, Sigma-Aldrich) in 0,01% bovine serum
albumin (BSA, Roche Diagnostics GmbH, Mannheim, Germany) combined with 480 ml
solution of 50 mM Tris (Promega Corporation, USA), 60 mM sodium acetate (Merck) and
0,02% BSA.
2.4.2 IHC protocols. The IHC protocols for the different ECM components were
conducted as follows. Slides were first deparaffinated using an automated system (Microm
HMS740, Walldorf, Germany) and kept in H2Od afterwards. The tissue on the slides was
outlined with a hydrophobic, delimiting pencil (DAKO). In the following step, formalin-fixed
tissues were pretreated with the respective pretreatment in citric acid buffer and others,
depending on the target of the immune stain. After pretreatments, a washing step was performed
in PBS + 0,3% Tween20 (1 L 0,01M PBS pH 7,2 – 7,4 plus 3 ml Tween20, DAKO) twice and
consequently in pure PBS (pH 7,2 – 7,4) once, each for 3 to 5 minutes. Endogenous peroxidase
block was performed in H2O2 (VWR) in PBS 1:9 for 10 minutes. Non-specific antibody binding
sites were blocked with casein solution (Vector Laboratories®, Burlingame, CA, USA) in
H2Od, or CAS-block (Vector®), and serum (Vector®). Afterwards, primary antibodies were
incubated for different times and under different temperature conditions depending on the target
of the immune stain. After incubation, the slides were washed in PBS + 0,3% Tween20 twice
and in pure PBS once, each for 5 minutes. In table 3, the antibodies and their concentrations
together with their targets can be found.
Table 3: Antibodies used in this study, their dilution and incubation time and product code. R/T=Room
temperature.
Antibody and target Dilution and incubation time Product information
Rabbit anti-collagen I 1:500, 2 hours at R/T Acris R1038
Rabbit anti-collagen III 1:500, 1 hour at R/T Abcam ab7778
Goat anti-decorin 1:500, 1 hour at R/T R&D System AF143
Rabbit anti-versican 1:100, 1 hour at R/T Abcam ab19345
Rabbit anti-fibromodulin 1:400, 1,5 hours at R/T Larry Fisher (NIH, Bethesda, MD), LF-150
Rabbit anti-biglycan 1:100, 1 hour at R/T Abcam ab49701
Rabbit anti-goat, biotinylated 1:200, 30 min. at R/T Dako, E0466
Anti-rabbit IgG Ready-to-use kit, 30 min. at R/T MP-7401, Vector Laboratories®
Anti-mouse IgG Ready-to-use kit, 30 min. at R/T MP-7402, Vector Laboratories®
Secondary antibodies of the ready-to-use solution kits (Vector®) were incubated for 30
minutes at room temperature. These antibodies carry a peroxidase (horse radish peroxidase)
19
enzyme-conjugate which is able to react with DAB. For decorin immune staining, a different
secondary antibody system was used consisting of biotinylated rabbit anti-goat (Dako, E0466)
2nd antibody 1:200 in PBS + 0,3% Tween20 and streptavidin horse radish peroxidase (HRP,
Dako, P0397) 1:200 in PBS + 0,3% Tween20. Both antibody and HRP were incubated 30
minutes at room temperature. Following incubation of the secondary antibodies, a washing step
is performed twice in PBS + 0,3% Tween20 and once in pure PBS. The histochemistry for the
detection of antibody reaction with the structure of interest was performed using DAB substrate
solution from DAB substrate kit (SK-4100, Vector®). The DAB substrate solution was
prepared with 1 ml H2Od, 17 µl buffer stock solution, 20 µl DAB stock solution and 16 µl H2O2
solution from the kit. The reaction of DAB with the peroxidase was observed under a light
microscope and stopped by transferring the slides to H2Od when a clear reaction was observed
without background. Usually, this was the case after 2 to 4 minutes. Counterstaining was
performed with Mayer’s hematoxylin for 10 seconds and slides were subsequently washed in
tap water for 5 minutes. Lastly, slides were dehydrated in the automated system and mounting
was performed using mounting medium (Richard-Allan Scientific). Detailed protocols of each
experiment can be found in the addendum (6.1 – 6.7).
3. Results
3.1 H&E staining. This method was applied to control (healthy) nerves, autograft
repaired nerves and conduit repaired nerves. Autograft and conduit repaired nerves were
obtained at 20, 30 and 50 days after implantation of the autograft or conduit. H&E staining
showed the general organization and morphology of the PN tissues. For example, dark blue
colored cell nuclei were observed based on the reaction with hematoxylin. However, the cell
type could not be determined based on this method. Further, several acidophilic structures, e.g.
collagens, were stained in red color based on the reaction with eosin.
Twenty days after implantation of autografts and conduits, cross-sections of proximal and distal
PN tissue of both groups showed characteristics of degeneration compared to control nerves. In
the center of sections of both groups the PN regeneration was observed. The degeneration
comprised degradation of axons and extracellular structures and an increase in the number of
cells of different types, e.g. macrophages, fibroblasts and Schwann cells. Further, blood vessels
inside both types of grafts and in the surrounding tissues were observed. The tissue inside the
graft was under progressive degeneration and after 20 days signs of regeneration were only
20
observed in the proximal nerve part. Cell infiltration had occurred outside of the perineurial
space of the autograft. Autograft repaired nerves displayed a homogeneous tissue organization
with macrophages, fibroblasts and Schwann cells. Novel neural tissue was formed and in the
proximal part of the nerve stump. Regeneration of endoneurium or axons was not observed
(figure 5, A and B).
Cross-sections of conduit repaired nerves at 20 days showed a marked degeneration in
distal nerve stumps and de novo formation of nerve tissue in the center of proximal nerve
stumps. The newly-formed nerve tissue comprised cells and the formation of a novel ECM.
This period was characterized by the presence of cellular clusters and newly-formed axons.
However, close to the conduit walls it was possible to identify a loose connective tissue and
several blood vessels. In contrast, the inner part of the conduits’ lumen was characterized by a
denser ECM and abundant cells (figure 5, C and D).
In autograft repaired nerves of 30 days after implantation, cluster organization of
regenerating axons started to appear in several sections and axons were surrounded by
endoneurium. An increase in the presence of extracellular components inside of the autograft
and in the number of fascicles filled with cells, e.g. fibroblasts, in the graft wall and outside the
graft was observed. The distribution of cells and extracellular components was more
homogeneous compared to conduit repaired nerves (figure 6, A and B). After 30 days, the
conduit repaired nerves showed clusters of nerve fibers, i.e. regenerating axons lying in close
proximity to each other forming a cluster, with restored endoneurium and groups of tiny axons
associated with cells. The presence of cells and extracellular components was mainly observed
in the center of the conduit lumen forming a circular area of regeneration. Curiously, in distal
nerve stumps this area was smaller (figure 6, C and D).
The histological analysis at 50 days after implantation revealed that the tissue pattern
and organization of both studied groups was similar to the observation at 30 days after
implantation. The autograft group showed a homogeneous distribution of cells and ECM. In
addition, it was possible to observe an increase of the density of these elements in the inner part
of the grafted nerve as compared to 30 days. Nerve fibers were found organized in clusters and
each nerve fiber was immersed in a newly-formed endoneurium connective tissue (figure 7, A
and B).
In the center of conduits, a slightly smaller regeneration area was present and separated
from the conduit wall by a space of loose connective tissue of several hundred micrometers.
21
This space between conduit wall and regeneration area was almost completely free of cells and
extracellular components. In the regeneration area, perineurium and endoneurium were
observed around groups of regenerating axons associated with cells in nerve fiber clusters
(figure 7, C and D).
3.2 MCOLL histochemical method. In this study, formalin and methacarn-fixed
tissues were used for the MCOLL method and only the tissues fixed in formalin showed an
appropriate histochemical reaction for myelin, collagen and cells. Methacarn is an alcoholic
fixative which preserves several tissue elements with optimal morphology and properties.
However, due to the alcoholic nature of this solution several lipids including myelin were
completely or partially dissolved. Most information about the degree of demyelination and
remyelination was derived from longitudinal nerve sections which displayed the degree of
myelination over up to several hundred micrometers of axon length. Additionally, the typical
parallel and undulated organization of nerve fibers was clearly visible in those sections. Cross-
sections of nerves therefore gave more information about the distribution and organization of
tissue elements, collagen fibers and changes related to myelin. Cells were stained for their
nucleus by the hematoxylin counterstain though identification of the specific cell type was not
possible based on this staining. Simultaneously with the evaluation of myelin, also collagen
organization and the process of axonal regeneration were evaluated with the MCOLL
histochemical method. The contrast between myelin and collagen and the specificity and
sensibility for both of these structures were markedly improved with MCOLL compared to
H&E staining.
22
Figure 5: H&E staining results of autograft (A and B) and conduit (C and D) repaired nerves after 20 days of
regeneration. In A1 – A3 (methacarn-fixed) and B1 – B3 (formalin-fixed) sections, the cellular and extracellular
density is low and clustered nerve fibers are not visible. Note the homogeneous appearance of the graft center in
A1 and B1. The sections C1 – C3 (methacarn-fixed) show the proximal nerve stump with more pronounced
regeneration in the center of the conduit forming the so-called regeneration area. D1 – D3 (methacarn-fixed)
sections display the distal nerve stump with less intense staining and smaller regeneration area compared to C
sections. Block arrows indicate clusters of regenerating axons, small arrows indicate blood vessels. Magnification:
A1, B1, C1, D1 = 4x. A2, B2, C2, D2 = 20x. A3 – D3 = 40x.
A3 A2 A1
B1 B2 B3
C1 C2 C3
D1 D2 D3
23
A3 A2 A1
B1 B2 B3
C1 C2 C3
D1 D2 D3
Figure 6: H&E staining results of autograft (A and B) and conduit (C and D) repaired nerves after 30 days of
regeneration. In A1 – A3 (methacarn-fixed) and B1 – B3 (formalin-fixed) sections, nerve fiber clusters and
endoneurium appear and the density of regeneration is markedly increased. Note the partial degradation of the
autograft wall in B. C1 – C3 (methacarn-fixed) display an increased regeneration area in the proximal part of the
conduit repaired nerve. Sections D1 – D3 (methacarn-fixed) show the distal nerve stump and a clearly smaller
regeneration area compared to the proximal nerve stump C. Block arrows indicate clusters of regenerating axons,
double-headed arrows indicate the autograft wall. Magnification: A1, B1, C1, D1 = 4x. A2, B2 = 20x. C2, D2,
A3 – D3 = 40x.
24
A1 A2 A3
B1
B2 B3
C1 C2 C3
D1 D2 D3
Figure 7: H&E staining results of autograft (A and B) and conduit (C and D) repaired nerves after 50 days of
regeneration. In A1 – A3 (methacarn-fixed) endoneurium and small axons are present, but the clustered
organization is hardly visible in A3. In B1 – B3 (formalin-fixed) sections, no cluster pattern of regenerated
axons are visible. C1 – C3 (methacarn-fixed) and D1 – D3 (methacarn-fixed) sections display clusters of
regenerating axons surrounded by endoneurium. C2 shows the space between conduit wall and regeneration
area which shows no regenerating axons and only few cells. Block arrows indicate clusters of regenerating
axons, double-headed arrows indicate the autograft wall which is partially disorganized. Magnification: A1,
B1, C1, D1 = 4x. A2 – D2 = 20x. A3 – D3 = 40x.
25
3.2.1 Myelin and collagen in autograft repaired nerves. Myelin was found to be
sparsely present in the proximal nerve stumps of autograft repaired nerves at 20 days after
implantation. Further, an important decrease of myelin accompanied by Wallerian degeneration
was observed. The histochemical reaction for myelin was weaker in longitudinal sections of
autograft repaired nerves at 20 days after implantation compared control nerves. Axons were
severely degenerated and unmyelinated at different degrees in the perineurial space over the
whole length of the axon (figure 8, A).
After 30 days of implantation, autograft repaired nerves were unmyelinated over the
whole length of the axons (figure 8, B). Autograft repaired nerves of 50 days after implantation
showed a weak reaction for myelin in longitudinal sections. At this point, myelination had
occurred over parts of the regenerated axons in the proximal part of the nerve (figure 8, C).
The reorganization of collagens in the regenerating peripheral nerves was assessed by
the picrosirius reaction as part of the MCOLL method. The typical undulated and parallel
organization of collagens and nerve fibers was observed in longitudinal sections. Collagens
were mainly found associated to the epineurium and perineurium of the grafted nerve. The
endoneurial compartment was less organized and composed of a loose collagen matrix with a
weak histochemical reaction. Additionally, it was possible to identify some blood vessels with
a positive reaction for collagen at the vessel wall (figure 8, A).
After 30 days of implantation, the autograft repaired nerves showed an increase of
collagen content in comparison to 20 days after implantation. Further, the extracellular space
displayed a dense network of collagens surrounding axonal sprouts in longitudinal and cross-
sections. Thin collagen sheaths, i.e. collagen fibers oriented longitudinally and
circumferentially around axonal sprouts, were observed, but nerve regeneration was not
organized into forming nerve clusters. In addition, it was possible to identify several axonal
sprouts with irregular organization near to the perineurial layer and surrounded by collagen
fibers (figure 8, B).
In sections of 50 days after implantation, the collagen fiber pattern showed no evident
alterations compared to autograft sections of 30 days after implantation. However, the density
of other extracellular components was slightly increased and led to a more homogeneous
appearance of the regenerating nerve tissue. Organization into clusters was not observed and
reestablishment of endoneurium was found in parts of the cross-sections. In longitudinal
26
sections, collagen sheaths around regenerating axons were present with a pattern and density
that was similar to control nerves (figure 8, C).
A1 A2 A3
B1 B2 B3
C1 C2 C3
D1 D2 D3
Figure 8: Evaluation of MCOLL histochemical results of autograft repaired nerves (A, B, C) and control (healthy)
nerves (D). A1 – A3 show the autograft repaired nerves 20 days after implantation and display degeneration and
demyelination of axons. Residual myelin (circle), collagen fibers (block arrows) and blood vessels with their typical
collagen-rich vessel wall (small arrows) are present. Scale bar = 40 µm. B1 – B3 show autograft repaired nerves
after 30 days of implantation with increased collagen expression (block arrows), but absence of myelin. Scale bars
= 80 µm (B1) and 40 µm (B2 & B3). C1 – C3 show autograft repaired nerve 50 days after implantation with a
dense, regenerated collagen network and partially remyelinated axons (circles). Collagen fibers (block arrows) and
blood vessels (small arrows) are also found. Scale bars = 80 µm (C1) and 40 µm (C2 & C3). D1 – D3 show the
healthy control nerves with plenty of myelin and ordered collagen fibers. Groups of myelinated axons (circles),
collagen fibers (block arrows) and blood vessels (small arrows) are observed. Scale bars = 100 µm (D1), 40 µm
(D2) and 30 µm (D3).
27
3.2.2 Myelin and collagen in conduit repaired nerves. MCOLL staining of this group
of nerves revealed a progressive nerve regeneration but no myelination of the newly-formed
axons at 20 days after implantation. Complete absence of myelin was observed and small axonal
sprouts were found only in the central, circular regeneration area of the conduit where new
nerve tissue was formed (figure 9, A). In contrast, a proximal longitudinal sections of conduit
repaired nerves of 30 days after implantation displayed axons with a weak residual reaction for
myelin in one section. Further, axons were thicker than 20 days after implantation. The degree
of myelination in these sections was comparable to the degree of myelination in autograft
repaired nerves of 50 days after implantation, but not comparable to the control nerves (compare
figure 8 C & D to figure 9 B). Cross-sections of conduit repaired nerves showed absence of
myelin in the newly-formed nerve fibers. The same was observed in longitudinal and cross-
sections after 50 days of implantation where regenerating axons also showed an increase in
diameter compared to 20 and 30 days after implantation (figure 9).
Collagen was found in conduit repaired nerves forming fibers which appeared properly
oriented along the newly-formed axons. Further, in longitudinal sections the typical undulated
and parallel organization of collagen fibers and axons was observed. In sections of 20 days after
implantation, collagen fibers were found in the newly formed endoneurium around the axonal
sprouts. In the center of the conduits, a regeneration area was formed which showed a higher
collagen density than the space between regeneration area and the conduit wall. In this space
between regeneration area and conduit wall, collagen was present as long and thin fibers and
accompanied by cells, however without axons. Furthermore, the regeneration area showed a
denser extracellular space compared to the extracellular space found in autograft after 20 days
of implantation. A certain degree of fibrosis was observed in the regeneration area and its
surrounding. This fibrosis was characterized by an intensely stained collagen fiber deposition
(figure 9, A).
The regeneration area inside the proximal part of the conduit showed an increase in size
at 30 days after implantation. The density and organization of collagen and other extracellular
structure in the perineurial regeneration area was comparable to 20 days after implantation.
Collagen was present in endoneurium of newly-formed axons. Fibrosis was observed in the
peripheral parts of the perineurial area at a similar degree as in sections of 20 days after
implantation. Longitudinal sections at 30 days after implantation showed stronger collagen
presence around axons compared to sections after 20 days of implantation (figure 9, B).
28
After 50 days of implantation, longitudinal sections of conduit repaired nerves showed
improved organization and more collagen compared to 20 and 30 days after implantation (figure
9). The collagen fibers, endoneurium and extracellular components appeared less dense in
cross-sections after 50 days than after 30 days of implantation. However, the organization of
collagen, endoneurium and extracellular components was still comparable. Fibrosis was
observed in several sections (figure 9, C).
A1 A2 A3
B1 B2 B3
C1 C2 C3
Figure 9: Evaluation of MCOLL histochemical results of conduit repaired nerves. A1 – A3 show conduit repaired
nerves 20 days after implantation and display degeneration and demyelination of axons. Collagen fibers (block
arrows) were intensely stained and formed endoneurium and axonal sheaths. Blood vessels (small arrows) with
their typical collagen rich vessel wall were also observed. Fibrosis can be seen in A2 between block and small
arrow as red collagen stacks (squares). Scale bar = 80 µm (A1) and 40 µm (A2 & A3). B1 – B3 show conduit
repaired nerve after 30 days of implantation with increased collagen expression (block arrows) and residual myelin
(circle) in longitudinal section. Scale bars = 80 µm (B1) and 40 µm (B2 & B3). C1 – C3 show conduit repaired
nerve 50 days after implantation. Collagen fibers (block arrows), blood vessels (small arrows) and fibrosis (squares)
are observed. Scale bars = 80 µm (C1) and 40 µm (C2 & C3).
29
3.3 Collagen I IHC. Results of the collagen type I IHC staining indicated the expression
and distribution of this protein in the regenerating nerve at 20, 30 and 50 days after implantation
of autograft or conduit. In control nerves, collagen type I was observed in the endoneurium
around each nerve fiber, in the perineurium and epineurium (figure 10, A).
After 20 days of regeneration, a strong reaction for collagen I was observed in the
autograft epineurium and blood vessels. This reaction was positive with a homogeneous and
clear extracellular pattern. However, collagen type I was absent in the endoneurium layer
(figure 10, B1 & B2). In longitudinal sections, a positive reaction in the perineurium was visible
and also in endoneurial space around axons which were associated with Schwann cells and
surrounded by collagen I sheath (figure 10, B3).
After 30 days of regeneration, the reaction intensified for collagen I in the ECM inside
of the autograft. Newly-formed axons in a network of collagen I were observed, without clear
endoneurium formation or clustered organization in the distal part and with collagen I positive
endoneurium in the proximal part of the nerve. In the graft-surrounding connective tissue,
fascicular structures which comprised cells and collagen I were visible (figure 10, C).
In the autograft repaired nerves of 50 days of regeneration, regenerating axons of the
distal nerve showed no ensheathment by collagen I fibers, no clustered organization or restored
endoneurium and unorganized collagen I expression in the ECM in the graft (figure 10, D1).
However, a dense network of small axons surrounded by collagen I sheaths with an organized
collagen I expression in the ECM was observed in the proximal nerve (figure 10, D2 & D3).
Also, collagen I was abundant in the proximal longitudinal section around regenerating axons
and this section showed the typical undulated orientation of collagen I fibers and axons (figure
10, D3).
In conduit repaired nerves after 20 days of regeneration, a small regeneration area
located in the center of the conduit was observed based on the reaction for collagen I in the
perineurial space. Very few and newly-formed axons were visible which were surrounded by
collagen I fibers and organized into nerve fiber clusters. Collagen I density in the ECM was
high towards the center of the regeneration area (figure 11, A1). In longitudinal sections, the
reaction was less intense and axons surrounded by collagen I were observed in the proximal
section showing advanced axonal regeneration. In the distal section, the expression of collagen
I was lower and axonal regeneration was less advanced showing small axonal sprouts (figure
11, A3 & A4). Outside of the perineurial regeneration area and towards the conduit wall,
30
collagen I was found in longitudinally cut blood vessels and small groups of regenerating axons
(figure 11, A2). In the proximal section, a bigger perineurial space was observed and showed
axon ensheathment by collagen I fibers and organization into clusters of regenerating nerve
fibers (figure 11, A1).
In conduit repaired nerves of 30 days after implantation, the perineurial space increased
in size, filling up almost the entire lumen of the conduit. In several sections, the endoneurial
sheath around small axons was stained but hardly visible in the center of the perineurial space
and more clearly visible in the periphery of the perineurial space. However, other sections
displayed bigger axons with collagen I sheath also forming a new endoneurium (figure 11, B1
& B2). Longitudinal sections showed the undulated organization of collagen I around axonal
sprouts, but these sprouts were not visible in all of the sections. Nonetheless, collagen I was
found in the ECM forming bands to support the axonal sprouts by a network of collagens.
In conduit repaired nerves, the expression of collagen I after 50 days was homogeneous
in the regeneration area. In the distal part, axons were small and endoneurium which stained
positive for collagen I appeared weakly around those axons. However, the proximal part
showed the reaction in the endoneurium more clearly where axons were also organized into
clusters (figure 11, C1 & C2). The collagen I expression in the ECM appeared thinner and less
organized compared with sections of 30 days after implantation. In the proximal part of the
longitudinal sections, the collagen fibers around regenerating axons were organized in an
undulated orientation forming a dense ECM of collagen I. In the distal part however, this
organization of collagen I in the ECM was present to a far less extent and only small axonal
sprouts were observed. A positive reaction in the wall of the NeuraGen® collagen conduits was
also observed.
31
Figure 10: Results of immunohistochemistry for collagen type I in control (healthy) and autograft repaired nerves.
In control nerves (A1 – A3) the normal collagen I organization and ensheathment of axons in a longitudinal section
can be seen. In autograft repaired nerves after 20 days of implantation, the graft epineurium is strongly reactive for
collagen I (B1) and in the perineurial space the ECM is less reactive for collagen I (B1 & B2). Collagen I is mostly
seen around blood vessels (small arrows). The proximal longitudinal section shows collagen I around regenerating
axons forming sheaths in the endoneurial space and in the perineurium (B3, block arrow). After 30 days, the distal
section (C1) shows no clear endoneurial sheaths while the proximal part of the same nerve displays thin endoneurial
sheaths around regenerating axons (C2). In the epineurium, fascicles comprising cells and positivity for collagen I
are found (C3). Blood vessels are indicated by small arrows and perineurium positive for collagen I by block arrow.
After 50 days of implantation, in the distal section D1 no endoneurial sheath formation or axonal clusters are found
while the proximal section D2 displays individual ensheathment by collagen I of regenerating axons. Also, the
proximal longitudinal section D3 displays big, regenerated axons with individual ensheathment and collagen I
positive perineurium (block arrow). Scale bars = 80 µm (A1, B1), 40 µm (A2, B2 & B3, C1 – C3, D1 – D3) and
20 µm (A3).
A1 A2 A3
B1 B2 B3
C1
D1
C2
D2
C3
D3
32
Figure 11: Results of immunohistochemistry for collagen type I in conduit repaired nerves after 20 (A), 30 (B) and
50 (C) days of implantation. After 20 days the density of collagen I in the ECM and around axons is highest in the
center of the perineurial regeneration area (A1) and gets progressively lower towards the conduit wall (A2). Small
axons, cell nuclei and blood vessels (small arrows) are visible. In distal (A3) and proximal (A4) longitudinal
sections, the regeneration was differently advanced and shows differently sized axons and collagen I sheaths around
the axonal sprouts. Blood vessels (small arrows) in the perineurium are also found. After 30 days, the ensheathment
of axons by collagen I in the endoneurial space, axon size and collagen I organization in the ECM are more
advanced in the proximal sections B2 compared to the distal section B1. In longitudinal sections the collagen I
density varies and B4 shows restored endoneurium more clearly than B3, but regenerating axons are embedded in
a collagen I rich ECM in both sections. Blood vessels (small arrows) are also stained. 50 days after implantation,
the collagen I density in the ECM seems to decrease and it is more difficult to observe endoneurium around
regenerating axons in C1 and C2. The distal longitudinal section C3 shows less organized collagen I expression in
the ECM and around axonal sprouts while the proximal section C4 has a more dense collagen I network and
advanced regeneration of axons. The walls of the NeuraGen® collagen conduits were also positive for collagen I.
Scale bars = 40 µm.
A1
A2
A3
A4
B1
B2
B3
B4
C1
C2
C3
C4
33
3.4 Collagen III IHC. Results of this IHC staining indicated the expression and
distribution of collagen type III in the regenerating nerve at 20, 30 and 50 days after
implantation of autograft or conduit. In control nerves, collagen III was present in endoneurial
sheaths surrounding individual axons and in the wall of blood vessels. Its expression pattern
was comparable to collagen I expression in control nerves, but it appeared to be less abundant
(figure 12, D). The positive reaction in blood vessels was also observed in both groups of
repaired nerves.
Collagen III expression and distribution after 20 days of regeneration in autograft
repaired nerves was different from collagen I in several ways. There was no network of collagen
III in the ECM, but circular organized sheaths of collagen III around individual axonal sprouts
were present. In the autograft epineurium, collagen III was found in fascicles which comprised
many cells. Further, collagen III was found in the walls of blood vessels (figure 12, A). In
longitudinal nerve sections, its expression and distribution was located around axons forming
the endoneurial sheath in a similar way as collagen I (figure 12, A).
After 30 days of regeneration, an increased density and network of collagen III was
observed in autograft repaired nerves. Collagen III was found in the ECM forming a dense
network and ensheathment of individual axons was difficult to observe due to the high density
and homogeneous distribution of collagen III (figure 12, B2). However, the proximal nerve
stump displayed the ensheathment of axons by collagen III in the perineurial space. In this
section, the ECM showed lower collagen III expression and a less disperse network in the
perineurial space (figure 12, B3). The longitudinal section displayed big regenerating axons
surrounded by collagen III positive endoneurial sheath and perineurium (figure 12, B1).
In autograft repaired nerves after 50 days of regeneration, the density of collagen III was
lower in the ECM of the distal nerve section than in the distal sections of 30 days. In the
autograft of the distal section, the nerve fiber clustered orientation disappeared and also
collagen III sheaths around axons were hardly visible. In the epineurium and connective tissue,
collagen III was found in fascicles comprising cells (figure 12, C2). In the proximal sections,
collagen III was found in endoneurial sheaths around regenerating axons. Collagen III was also
found in perineurium of those sections and in blood vessel walls and fascicle in the epineurium
(figure 12, C3). In the longitudinal sections, the expression was lower in the proximal section
which also comprised axons of bigger size compared to the distal sections that comprised axons
at an earlier stage of regeneration. In proximal and distal sections collagen III was found in the
34
perineurium and perineurial space forming sheaths around regenerating axons and in the ECM
of the endoneurial space (figure 12, C1, C4 & C5).
In conduit repaired nerves at 20 days after implantation, the reaction was weaker for
collagen III than for collagen I in the perineurial space, but the expression pattern was
comparable. Collagen III was found in the endoneurial space, in several axons forming
clustered nerve fibers and in the ECM. In the distal section, the expression of collagen III in the
ECM was lower than in the proximal sections. In all sections, multiple blood vessels were
identified based on collagen III reaction in the vessel walls (figure 13, A1-A4). Collagen III
expression was lower in distal longitudinal sections of nerves, but was organized in sheaths
around regenerating axons and less abundant in the ECM surrounding these axons. Distal nerve
stump showed marked degeneration of axons and low collagen expression while the proximal
stump consisted of thicker newly-formed axons and properly oriented collagen sheaths (figure
13, A3 & A4).
Thirty days after implantation, the perineurial regeneration area in the center of the
conduit increased in size, but the expression pattern of collagen III was comparable to 20 days
after implantation. Collagen III was clearly visible in endoneurium of regenerating axons and
in the ECM (figure 13, B1 & B2), but it was less abundant in the ECM compared to collagen I.
Further, regenerating axons were packed into clusters which were positive for collagen III. In
longitudinal sections, regenerating axons were surrounded by collagen III sheaths and again in
distal and proximal sections the degree of regeneration of axons was different, i.e. more advance
in the proximal part (figure 13, B3 & B4).
In conduit repaired nerves of 50 days after implantation, the reaction for collagen III
was weak in the ECM of the perineurial space of proximal and distal sections. Collagen III was
found almost exclusively in endoneurial sheaths of axons packed in clusters (figure 13, C1 &
C2). The reaction was very weak in longitudinal sections compared to collagen I, and collagen
III was almost absent in the ECM of distal and proximal sections. However, it was still observed
around regenerating axons and the organization of the collagen III was slightly more
homogeneous than in sections of 30 days after implantation (figure 13, C3 & C4).
35
A1 A2 A3
B1 B2 B3
C1 C2 C3
C4 C5 D1
Figure 12: Results of immunohistochemistry for collagen type III in control (healthy) (D1) and autograft repaired
nerves after 20 (A), 30 (B) and 50 (C) days of implantation. After 20 days the expression of collagen III in the
perineurial ECM is low and endoneurial sheaths around axons are formed in proximal sections (A1 & A2). Collagen
III is also present in the wall of blood vessels (small arrows) and in fascicles in the autograft epineurium. In
longitudinal sections, it is found in sheaths around regenerating axons. After 30 days, the ensheathment of axons
by collagen III is more difficult to observe and collagen III is more densely present in the ECM of the perineurial
space (B2 & B3). In longitudinal sections, collagen III is found in endoneurial sheaths around axons and in the
perineurium (B1). Blood vessels (small arrows) are also stained. 50 days after implantation, endoneurial sheaths of
collagen III and nerve fiber clusters are difficult to observe in the distal section (C2), but are more clearly visible
in the proximal section (C3). The longitudinal sections show different stages of axonal regeneration and collagen
III expression and organization. The proximal C1 shows the most advanced regeneration of axons and endoneurial
sheaths of collagen III while in distal sections C4 and C5 the axons are less advanced in the regeneration process
and collagen expression is higher but less organized. Perineurium is indicated by block arrows. Scale bars = 40 µm.
36
A1
A2
A3
A4
B1
B2
B3
B4
C1
C2
C3
C4
Figure 13: Results of immunohistochemistry for collagen type III in conduit repaired nerves after 20 (A), 30 (B)
and 50 (C) days of implantation. After 20 days, the expression is low in the perineurial ECM and more pronounced
in endoneurial sheaths, blood vessel walls (small arrows) and clusters of newly-formed axons (A1 & A2). In
longitudinal sections, collagen III is found sparsely around early regenerating axons in the distal part (A3) and more
advanced regenerating axons in the proximal part (A4) forming endoneurial sheaths. In sections of 30 days after
implantation, clusters of axons surrounded by endoneurial sheaths are present and the density of collagen III
increases in the ECM (B1 & B2). Axonal regeneration and endoneurial ensheathment is also found to be more
advanced in longitudinal sections (B3 & B4). After 50 days, collagen III density in the perineurial ECM appears to
decline but nerve fiber clusters and endoneurium are still positive and visible in both cross-sections and longitudinal
sections. Scale bar = 40 µm.
37
3.5 Decorin IHC. The IHC reaction for decorin resulted in a staining pattern in healthy
control nerves, autograft and conduit repaired nerves fixed in methacarn. The expression pattern
of decorin in the ECM was analyzed in those sections of repaired nerves after 20, 30 and 50
days of implantation of autografts or conduits. In control nerves, decorin was found to be
sporadically expressed in the perineurial ECM surrounding several axons in cross-sections of
nerve and in the connective tissue surrounding the nerve (figure 14, A1).
In autograft repaired nerves of 20 days after implantation, decorin was found to be
expressed in the autograft epineurium of two sections. In the proximal section, decorin was
homogeneously expressed in the perineurial ECM around regenerating axons of various sizes
and in the wall of blood vessels. In the distal section, the ECM in the regenerating nerve tissue
was negative for decorin (figure 14, B1 & B2). In the longitudinal section of this nerve, decorin
was weakly expressed in the endoneurial ECM surrounding axons and in blood vessel walls.
Due to the reaction of decorin the typical undulated pattern of the nerve was observed (figure
14, B3).
After 30 days of regeneration, the proximal section of autograft repaired nerve showed
a positive reaction in the epineurium and in the perineurial space of the graft in the ECM.
Further, blood vessels were stained positive for decorin and the distribution of decorin was
homogeneous among the ECM (figure 14, C1, C2 & C3). In the proximal part of the nerve
section, tiny regenerating axons surrounded by sheaths and decorin in the ECM were visible
which were not observed in the distal part of this nerve sections (figure 14, C2). The distal
section of autograft repaired nerve displayed no positive reaction for decorin in the ECM of the
perineurial space (figure 14, C3). However, the epineurium and surrounding connective tissue
were positive for decorin and a small proximal part of a longitudinal section also showed
positivity around several regenerating axons (figure 14, C4).
Longitudinal sections showed positivity for decorin in the perineurial space and ECM
around regenerating axons after 50 days of regeneration. The reaction was stronger in the
proximal part of the longitudinal section which also featured a more advanced regenerative
status with bigger axons than the distal part of this nerve (figure 14, D3 & D4). In the distal
cross-sections, decorin was found to be expressed homogeneously in the perineurium and in
the ECM of the perineurial space of the graft around groups of axons organized into nerve fiber
clusters (figure 14, D1). The proximal cross-section showed less positive reaction and a more
diffuse staining pattern for decorin in the perineurium and ECM in the perineurial space of the
38
graft and nerve fiber clusters surrounded by endoneurium were sporadically stained. The
density of decorin had declined in the ECM of the proximal nerve section (figure 14, D2).
Several sections of conduit repaired nerves were evaluated after 20 days of regeneration
and decorin was found to be abundant and diffusely expressed in a central longitudinal section
around axonal sprouts (figure 15, A3). A more proximal longitudinal section showed bigger
newly-formed axons and decorin expression was much lower in the perineurial space and ECM
around those axons (figure 15, A4). Two proximal cross-sections were positive in the
perineurial space for decorin which was found in the ECM and around clusters of regenerating
axons. The presence in the ECM was more pronounced in the perineurial space where no
clusters of newly-formed axons were observed (figure 15, A1). Two distal cross-sections
showed a negative reaction for decorin, but those sections also showed axonal regeneration and
nerve fiber clusters (figure 15, A2).
After 30 days of regeneration, decorin expression was found to be markedly increased
in the periphery of the perineurial regeneration area, but not in the center where the reaction
was weak in the proximal and negative in the distal section. The ECM in the endoneurial space,
around nerve fiber clusters, comprised groups of newly-formed axons and was, together with
blood vessel walls, moderately positive for decorin (figure 15, B1 – B3). Longitudinal sections
showed a very weak staining in the endoneurial space around small axons (figure 15, B4).
After 50 days of regeneration, distal cross-sections displayed a negative reaction for
decorin in the center of the perineurial regeneration area in the conduit. However, towards the
conduit wall and at the outer edge of the regeneration area, the expression was positive in the
ECM. Nerve fiber clusters were observed in which the ECM showed positivity for decorin and
these clusters were located in the periphery of the perineurial space (figure 15, C1). Proximal
sections displayed newly-formed axons and a more homogeneous expression pattern of decorin
in the ECM over the perineurial regeneration area (figure 15, C2 & C3). In longitudinal sections,
decorin was found in the ECM of the endoneurial space and differently sized axons were
observed. The reaction was strong and homogeneous highlighting the undulated pattern of the
newly-formed axons (figure 15, C4).
39
Figure 14: Results of immunohistochemistry for decorin in control (A1) and autograft repaired nerves after 20 (B),
30 (C) and 50 (D) days of implantation. In the control nerve, decorin expression is limited to the ECM of the
perineurial space between only few axons (A1). In autograft repaired nerves after 20 days of implantation, decorin
is found in the epineurium and in the ECM of the endoneurial space (B1). The distal section is completely negative
(B2). In the longitudinal section, the reaction is very weak and decorin is observed around several regenerating
axons (B3). In sections of 30 days after implantation, the presence of decorin is markedly increased in the
perineurial space and ECM. The expression pattern is homogeneous, but regenerating axons and organized decorin
within the ECM are observed only in the proximal section (C2). The distal section is negative for decorin in the
ECM, but positive in the epineurium and connective tissue (C3). Further, decorin is expressed in the ECM
surrounding regenerating axons in the longitudinal section (C4). Cross-sections of 50 days after implantation show
decorin expression in the endoneurial space (D1 & D2), but the proximal section (D2) has a lower and non-
homogeneous reaction pattern (D2). The longitudinal section D3 shows advanced regeneration of axons and decorin
expression in the ECM. In the distal part, axons are less advanced in regeneration and smaller, but also surrounded
by decorin in the ECM (D4). Small arrows indicate blood vessels. Block arrows indicate perineurium positive for
decorin. Scale bar = 60 µm (B2) and 30 µm (A1, B1, B3, C & D).
A1 C1
C2
C3
C4
D1
D2
D3
D4
B1
B2
B3
40
A1
A2
A3
A4
B1
B2
B3
B4
C1
C2
C3
C4
Figure 15: Results of immunohistochemistry for decorin in conduit repaired nerves after 20 (A), 30 (B) and 50 (C)
days of implantation. After 20 days of regeneration, decorin is observed in the perineurial space and ECM
surrounding newly-formed axons in the proximal section (A1). The distal section is negative for decorin (A2). In
the central part of the longitudinal section, the expression was strong in the ECM surrounding axonal sprouts (A3).
The proximal part of the longitudinal section displays more advanced regeneration of axons and less decorin
expression in the ECM surrounding those axons (A4). After 30 days of regeneration, the perineurial space of the
conduits is mostly negative for decorin, but towards the borders of the perineurial space the expression increases in
the ECM (B1 & B2). Decorin is found in the ECM surrounding clusters of newly-formed axons (B3). The
longitudinal section shows very weak reaction of decorin (B4). 50 days after implantation, there is no expression
of decorin observed in the center of the regeneration area, but is observed only at the borders of the perineurial
space. Axons are packed into clusters which are surrounded by decorin positive ECM (C1 – C3). In the longitudinal
section, decorin expression is increased and it is present in the ECM around axons (C4). The transition from center
to periphery of the regeneration area is indicated by block arrows. Scale bar = 60 µm (B1, B2, C1 & C2) and 30
µm (A, B3, B4, C3 & C4).
41
3.6 Versican, fibromodulin and biglycan IHC. The IHC protocol for versican was
carried out using formalin-fixed autograft and conduit repaired nerve sections after 20, 30 and
50 days of implantation. In all sections, including control sections of healthy nerve, the reaction
was negative and no staining pattern was observed (figure 16, A1 – A4). Due to the hematoxylin
counterstain, it was possible to observe cell nuclei and blood vessels in the tissues. The
transition between autograft and conduit lumen, perineurium and epineurium and surrounding
connective tissue was visible (figure 16, A2 & A3).
Results from IHC stainings for fibromodulin in methacarn-fixed sections of autograft
and conduit repaired nerves after 20, 30 and 50 days of implantation indicated no staining
pattern in the nerve tissues. In several sections of both types of repaired nerves only the wall of
blood vessels and parts of the connective tissue showed a weak reaction (figure 16, B2 & B3).
The ECM in the regenerating nerve tissues was negative for fibromodulin. Blood vessels and
cell nuclei were found due to hematoxylin counterstain.
The IHC protocol for biglycan was performed in formalin-fixed autograft and conduit
repaired nerve sections of 20, 30 and 50 days after implantation. All sections displayed negative
reactions for biglycan and no expression was observed. The hematoxylin counterstain allowed
for the observation of cell nuclei and blood vessels based on their lumen and muscle-layered
wall (figure 16, C1 – C4).
42
Figure 16: Overview of several results of immunohistochemistry for versican (A), fibromodulin (B) and biglycan
(C). A1 and A3 display the negative reaction for versican after 20 and 50 days, respectively, after implantation of
autografts. Blood vessels (small arrows) and the perineurium (block arrows) as well as cell nuclei are observed
based on the hematoxylin counterstain. A2 and A4 show the negative reaction for versican in conduit repaired
nerves after 20 and 50 days, respectively, after implantation. In sections B2 (conduit repaired nerve, 20 days after
implantation) a slightly positive reaction for fibromodulin in the perineurium is observed (block arrow). In B3
(autograft repaired, 50 days after implantation) a slightly positive background reaction in the autograft epineurium
(block arrow) and blood vessel walls (small arrow) is observed. Autograft repaired sections of 20 and 50 days (C1
and C3, respectively) and conduit repaired sections of 20 and 50 days (C2 and C4, respectively) after implantation
show negativity for biglycan in all sections. Only blood vessels are observed based on erythrocytes reaction to DAB
(C1 & C2, small arrows). Scale bar = 60 µm.
A2
A3
A4
B1 C1
B2 C2
B3 C3
B4 C4
A1
43
4. Discussion and conclusion
The H&E stainings gave a histological overview of control, autograft and conduit
repaired nerves. It allowed us to evaluate and compare the basic morphological patterns during
sciatic nerve regeneration in rats at different time intervals, i.e. 20, 30 and 50 days after
implantation of autografts or conduits. Clusters of regenerating axons were present at an earlier
stage in time, i.e. 20 days after implantation, in conduit repaired nerves than in autograft
repaired nerves. The tissue in the autograft is first under progressive degeneration where axons
and myelin are degraded before the regenerating axons advance in the graft. The collagen-based
conduits therefore seemed to promote axonal regrowth and the formation of new nerve fiber
clusters in proximal and distal nerve stumps at an earlier stage in the regeneration process than
autografts. Further, the histochemical reaction in the ECM was more intense around those nerve
fiber clusters at 20 days after implantation in conduit repaired nerves compared to autograft
repaired nerves where the ECM density was lower due to the ongoing degeneration. However,
this difference was not observed after 30 and 50 days of implantation which indicates an equal
density and composition of ECM at those points in time.
The presence of newly-formed axons in the conduit repaired nerves after 20 days of
implantation showed that the regenerating nerve was in an advanced state. Typically,
regeneration in a hollow conduit occurs in different phases where new nerve tissue is formed
progressively. First, components with neurotrophic and supporting activities fill up the lumen
of the conduit during the first days after implantation in the fluid phase. Afterwards, a fibrin
network is formed between the proximal and distal end of the sectioned nerve and fibroblasts
along with other cells infiltrate the lumen from both nerve ends in this matrix phase. At that
time, Wallerian degeneration is taking place in the distal nerve stump where Schwann cells and
other cells recycle and remove the axonal breakdown products. This environment is important
for the Schwann cells and newly-formed axons in the second week of regeneration, the cellular
phase, where both of them migrate along the fibrin network and axons proceed from proximal
into the distal nerve end target. In the third week and later on, the axons continue to regenerate
and are myelinated by Schwann cells in the following 2 to 8 weeks in the so-called axonal phase
(38) (39). In this study, sections of conduit repaired nerves after 20 days of implantation showed
that the nerve tissue had proceeded into the axonal phase and newly-formed axons were present
in the distal nerve end.
The myelination status and collagen reorganization are important in the process of PN
regeneration and hence the MCOLL histochemical method can be conducted to determine the
44
degree of myelination and collagen expression and organization (25). The use of the MCOLL
histochemical method allowed us to observe the demyelination in autograft and absence of
myelin in conduit repaired nerves after 20 days of implantation in both types of nerve repair.
Demyelination and Wallerian degradation with loss of axon numbers and mass are typical
features of transected nerves (3). Residual myelin was observed in one autograft section which
was later degraded since all sections of 30 days after implantation of the graft were completely
negative for myelin. Also, only conduit repaired nerves, which were completely negative for
myelin after 20 days of implantation, showed myelination after 30 days of regeneration in the
proximal nerve ends. Unfortunately, there were no longitudinal sections of 50 days after
implantation of conduit repaired nerves to evaluate myelination, but in autograft repaired nerves
remyelination was observed after 50 days of implantation. The degree of myelination was still
lower than in control nerves and cross-sections of both type of nerve repair were negative for
myelin after 20, 30 and 50 days of regeneration which indicates that the myelination process
was still ongoing and far from being completed.
Collagen is an important molecule in the ECM during regeneration and guides the
axonal sprouts by forming a network along which the axons can grow (8) (12) (13). Its
expression in autograft and conduit repaired nerves was found to be linked to the degree of
axonal regeneration. 20 days after implantation of autografts or conduits, the density of the
collagen network was lower and axonal sprouts were smaller than at 50 days after implantation.
Especially autograft repaired nerves displayed a loose network of collagen in the ECM of the
perineurial space at 20 days after implantation. At this time point, collagen was found in the
perineurium and endoneurial ECM around clusters of newly-formed axons of the conduit
repaired nerves. This indicates that the conduit environment promotes the precise collagen
organization in the ECM around clusters of axons to facilitate axonal pathfinding and growth.
Further, proximal and distal sections could clearly be differentiated based on the differences in
collagen density, organization and axonal size. Although the conduit environment seemed to be
positive for collagen organization and axonal regeneration, fibrosis and scar tissue formation
which are characterized by excessive collagen deposition was observed in conduit repaired
nerve sections 20, 30 and 50 days after implantation. This phenomenon is frequently observed
in regenerating nerves and is known to influence the proper regeneration and growth of axonal
sprouts (14).
IHC stainings for two specific forms of collagen, i.e. collagen type I and III, reveal more
precisely their expression and organization in the ECM of autograft and conduit repaired nerves
45
at 20, 30 and 50 days after implantation. Collagen I and III belong to the group of fibril forming
collagens and are found in the basal lamina of myelinating Schwann cells and in the
endoneurium (10) (12) (13) (14). The results from collagen I IHC in autograft repaired nerves
indicate that the endoneurial ensheathment of regenerating axons is not restored after 50 days
in distal section, but is restored in proximal sections after 30 days and 50 days of implantation.
This collagen network which originates in the proximal nerve end and develops along the earlier
formed bands of Büngner is crucial for the axonal growth towards the distal end. Regeneration
can thus only be successful if the collagen network and ensheathment is provided for the axonal
sprouts up to the distal nerve end (16). In conduit repaired sections, axonal ensheathment by
collagen I in the endoneurium is already observed after 20 days of implantation in proximal and
distal sections. However, the reaction in the ECM is rather weak in later stages of regeneration
where individual axonal ensheathment is not observed and the highest collagen I density is
observed around clusters of newly-formed axons. It seems peculiar that collagen I is not
observed in axonal sheaths at 50 days after implantation since this ensheathment was observed
in autograft repaired nerves after 50 days and thus should also be present in conduit repaired
nerves at this time. It is possible that the antibody reaction was not optimal in those conduit
sections and the collagen was not completely stained.
Collagen III expression and organization appears to be similar to collagen I, however
collagen III was not as abundant in both types of repaired nerves as collagen I. Further, it is
observed that collagen III is present in perineurium and endoneurium of the regenerating nerves
and probably also in the basal lamina which connects myelinating Schwann cells to the axons.
The relationship of Schwann cell and the newly-formed axon is crucial for the nerve
regeneration (8) (12) and it is observed in conduit repaired sections at 20 days after
implantation. These findings indicate that the conduit repair promotes restoring the collagen III
ensheathment of newly-formed axons at an earlier point in time than autograft repair promotes
the endoneurial collagen III sheath formation.
Decorin has been reported to play a crucial role in fibril formation by interacting with
collagens (13) (53) (54). Our results suggest that decorin is expressed in the perineurial space
in close concert with collagen I and III, first in proximal nerve ends and later also in distal nerve
ends. Further, in autograft repaired nerves, decorin is not found in distal sections at 20 and 30
days after implantation while conduit repaired nerves are positive for decorin in the perineurial
and endoneurial space in both proximal and distal nerve endings after 30 days of implantation.
Additionally, it appears that advanced regeneration in conduit repaired nerves leads to lower
46
decorin expression in the endoneurial ECM and this expression equals the low decorin
expression in healthy nerves. Therefore, it seems that the conduits promote the fibril formation
of endoneurial collagen earlier than autograft repair from proximal to distal nerve ends by
increased decorin expression. This should be a factor for enhanced nerve regeneration since the
collagen fibril network is necessary and crucial factor in successful axonal pathfinding and
nerve repair (12).
The CSPG versican has been reported to be an inhibitor of axonal growth during nerve
regeneration (55). Furthermore, versican has been observed by IHC in distal nerve stumps and
in newly formed endoneurial sheaths of regenerating rat sciatic nerves (35). Another study
looked at specific isoforms of versican, namely V0/V1, and found that these isoforms were
upregulated in the proximal segment of rat sciatic nerve (56). In contrast, in the present study
it was not possible to obtain a positive staining in control or repaired nerves for versican. It is
assumed that the antibody works properly, but it may be possible that the nerve tissues were
either not treated properly or did not express versican at all or a form of the versican epitope
that is detectable with this antibody system.
Fibromodulin is expressed in connective tissues and plays a role in collagen
fibrillogenesis by binding to collagen type I and II (13) (53) (54). The positivity obtained by
the IHC for fibromodulin in our study was due to background reaction in the perineurium and
connective tissue surrounding the nerve fiber bundle. In the present study, a dense collagen I
and III network with possible fibril formation could be observed in regenerating nerves and
fibromodulin which has been reported to impede the fibril formation could be absent in those
sections to not interfere with collagen I fibrillogenesis in the ECM. However, complete absence
of fibromodulin in knockout experiments in other tissues has been shown to cause dysfunctions
in those tissues (20) suggesting that fibromodulin is needed to regulate proper collagen
fibrillogenesis at least in certain tissues. Whether fibromodulin expression is needed and in
which compartment of regenerating PN it has to be expressed for correct collagen
fibrillogenesis remains to be elucidated.
Biglycan is thought to be expressed in many tissues and to interact with collagen type I
and to work cooperatively with decorin in the process of fibrillogenesis (13) (18) (54).
However, it has also been reported that biglycan together with fibromodulin can inhibit collagen
fibrillogenesis in certain tissues (20). In this study, biglycan could not be detected by IHC
means in any compartment of the nerve sections. Since collagen type I was abundant and
47
decorin was also found, it was expected that biglycan should also be present. However, since a
dense collagen I and III network with possible fibril formation was found, biglycan could be
absent to not interfere with the ECM-collagen network in the perineurial space and
fibrillogenesis. It is rather unlikely that biglycan only has negative effects on fibril formation
and thus should be completely absent when fibril formation is observed (54). It is more likely
that in our study biglycan was not detected due to masking of the epitope or the use of protocol
with which it is not possible to detect biglycan.
Regarding the proteoglycans decorin, versican, fibromodulin and biglycan, it is difficult
to say whether they are required to be expressed and therefore detectable by IHC during sciatic
nerve regeneration and where they should be expressed in the ECM. It is clear that these
proteoglycans play important roles in the ECM of various tissues and except for versican, they
also influence collagen fibril formation in one way or the other (13) (53) (54). At least for
decorin this study shows an expression pattern in the ECM which is linked to the expression of
collagen I and III in a spatiotemporal manner and suggests that decorin is required for nerve
repair in association with collagen I and III. These perineurial and endoneurial fibril-forming
collagens which also form the ensheathment of axons are particularly important for PN
regeneration (14). The expression and distribution of these collagen types were more organized
in the perineurial and endoneurial space of conduit repaired nerves than in autograft repaired
nerves. This may further indicate that conduit repair has structural regeneration advantages over
autograft repair when this histological view is concerned.
In conclusion, the use of specific IHC protocol provided a solid base for the evaluation
though attention is needed to further improve these protocols to obtain better results in future
studies. The presence of clusters of newly-formed axons and the size of these axons showed
that conduit repair enhances the sciatic nerve regeneration compared to autograft repair within
the first 20 days after implantation. Also, myelination of the newly-formed axons occurred
earlier in conduit than in autograft repaired nerves which shows advanced regeneration after
conduit repair. This form of nerve repair also has structural advantages for collagen I and III
reorganization in the perineurial and endoneurial space and therefore axonal growth from
proximal to distal ends. Autograft repair demands more time to produce a collagen network for
axonal regeneration. Further, decorin expression and organization is enhanced by using conduit
repair and close to normal expression patterns were observed after 50 days of implantation.
This should improve collagen fibril formation and axonal regeneration more than autograft
repair. Other proteoglycans, i.e. versican, fibromodulin and biglycan were not expressed in
48
healthy or regenerating sciatic nerves and may not be required for nerve repair within the first
50 days after implantation of the autograft or conduit. Eventually, conduit nerve repair displays
advantages over autograft repair for the expression and reorganization of several important
components of the PN ECM.
Acknowledgment
The in vivo analyses and tissue collection was performed in the tissue engineering group
of the University of Granada, Spain. This study was supported by the Spanish Plan Nacional de
Investigación Científica, Desarrollo e Innovación Tecnológica (I+D+i) from the National
Ministry of Economy and Competitiveness (Instituto de Salud Carlos III), grant FIS PI14-1343
and grant IPT-2011-0742-900000 (INNPACTO program). Both grants were co-financed by
Fondo Europeo de Desarrollo Regional (FEDER), European Union.
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6. Addendum
6.1 Immunohistochemistry – Collagen I
Primary antibodies: Rabbit Anti-Collagen I (Acris R1038)
Secondary antibody: Anti-Rabbit IgG (Polymer detection kit, Vector Laboratories) (MP-
7401)
Fixation: Methacarn for 3,5 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
3. Endogenous peroxidase block 3% H2O2 in PBS 10 min.
4. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 3 min. per solution
5. Block non-specific antibody
binding sites
Casein block 1:9 in H2Od,
Serum 15 min. per solution
6. Incubate primary antibody Rabbit Anti-Collagen I 1:500 in
PBS+Tween20 2 hours at R/T
7. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
8. Incubate secondary antibody Anti-rabbit IgG for both
Ready-to-use solutions 30 min. at R/T
9. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
10. Histochemistry: DAB DAB reagent solution
Between 30 sec. to 3 min. (watch
reaction under microscope until the
reaction is intense like controls),
stop reaction with H2Od
11. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 5
min. afterwards
12. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
13. Mount Standard mount medium -
6.2 Immunohistochemistry – Collagen III
Primary antibodies: Rabbit Anti-Collagen III (Abcam ab7778)
Secondary antibody: Anti-Rabbit IgG (Polymer detection kit, Vector Laboratories) (MP-
7401)
Fixation: Methacarn for 3,5 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
3. Endogenous peroxidase block 3% H2O2 in PBS 10 min.
4. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 3 min. per solution
5. Block non-specific antibody
binding sites
Casein block 1:9 in H2Od,
Serum 15 min. per solution
6. Incubate primary antibody Rabbit Anti-Collagen III 1:400 in
PBS+Tween20
Rabbit Anti-Collagen III for 1 hour
at R/T
7. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
8. Incubate secondary antibody Anti-rabbit IgG
Ready-to-use solutions 30 min. at R/T
9. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
10. Histochemistry: DAB DAB reagent solution
Between 30 sec. to 3 min. (watch
reaction under microscope), stop
reaction with H2Od when is intense
positive
11. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 5
min. afterwards
12. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
13. Mount Standard mount medium -
6.3 Immunohistochemistry – Decorin
Primary antibodies: Goat Anti-Decorin, R&D system (AF143)
Secondary antibody: Biotinylated Rabbit Anti-Goat (); Streptavidin HRP.
Pretreatment – Chondroitinase ABC 0,2 U/ml (Sigma cat nr. C3667): 40 ml H2Od, albumin
serum bovine 0,01g, sodium acetate 0,81g, Tris base 0,3g.
Fixation: Formalin 24 hours, methacarn 3,5 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Rinse in 37°C PBS 0,1M PBS (pH7,2-7,4) 20 min. at 37°C
3. Pretreatment with
chondroitinase ABC Chondroitinase ABC 0,2U/ml 1 hour at 37°C
4. Rinse twice in cold
PBS+Tween20 and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
5. Endogenous peroxidase block 3% H2O2 in PBS 10 min.
6. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
7. Block non-specific antibody
binding sites CAS-block solution 15 min.
8. Incubate primary antibody Goat Anti-Decorin 1:500 in
PBS+Tween20 1 hour at R/T
9. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
10. Incubate secondary antibody Biotinylated rabbit anti-goat 1:200
in PBS+Tween20 30 min. at R/T
11. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
12. Incubate streptavidin-
horseradish peroxidase
Streptavidin HRP 1:200 in
PBS+Tween20 30 min. at R/T
13. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
14. Histochemistry: DAB DAB reagent solution
Between 2 to 4 min. (watch
reaction under microscope), stop
reaction with H2Od
15. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 5
min. afterwards
16. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
17. Mount Standard mount medium -
6.4 Immunohistochemistry – Versican
Primary antibodies: Rabbit Anti-Versican, Abcam (ab19345)
Secondary antibody: Anti-Rabbit IgG (Polymer detection kit, Vector Laboratories) (MP-
7401)
Pretreatment – Chondroitinase ABC 0,2 U/ml (Sigma cat nr. C3667): 40 ml H2Od, albumin
serum bovine 0,01g, sodium acetate 0,81g, Tris base 0,3g.
Fixation: Formalin 24 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Rinse in 37°C PBS 0,1M PBS (pH7,2-7,4) 20 min. at 37°C
3. Pretreatment with
chondroitinase ABC Chondroitinase ABC 0,2U/ml 1 hour at 37°C
4. Rinse twice in cold
PBS+Tween20 and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
5. Endogenous peroxidase block 3% H2O2 in PBS 10 min.
6. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
7. Block non-specific antibody
binding sites CAS-block solution 15 min.
8. Incubate primary antibody Rabbit Anti-Versican 1:100 in
PBS+Tween20 1 hour at R/T
9. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
10. Incubate secondary antibody Anti-rabbit IgG ready-to-use kit
(Vector) 30 min. at R/T
11. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
12. Histochemistry: DAB DAB reagent solution
Between 2 to 4 min. (watch
reaction under microscope), stop
reaction with H2Od
13. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 3
min. afterwards
14. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
15. Mount Standard mount medium -
6.5 Immunohistochemistry – Fibromodulin
Primary antibodies: Rabbit Anti-Fibromodulin, Larry Fisher (LF) 150
Secondary antibody: Anti-Rabbit IgG (Polymer detection kit, Vector Laboratories) (MP-
7401)
Pretreatment – Chondroitinase ABC 0,2 U/ml (Sigma cat nr. C3667): 40 ml H2Od, albumin
serum bovine 0,01g, sodium acetate 0,81g, Tris base 0,3g.
Fixation: Methacarn 3,5 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Rinse in 37°C PBS 0,1M PBS (pH7,2-7,4) 20 min. at 37°C
3. Pretreatment with
chondroitinase ABC Chondroitinase ABC 0,2U/ml 1 hour at 37°C
4. Rinse twice in cold
PBS+Tween20 and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
5. Endogenous peroxidase block H2O2 1:9 in PBS 10 min.
6. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
7. Block non-specific antibody
binding sites
Casein block 1:9 in H2Od,
Serum 15 min. for both blocks
8. Incubate primary antibody
Rabbit Anti-Fibromodulin 1:400
(methacarn-fixed) in
PBS+Tween20
1,5 hour at R/T
9. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
10. Incubate secondary antibody Anti-rabbit IgG ready-to-use kit
(Vector) 30 min. at R/T
11. Rinse 3 times in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
12. Histochemistry: DAB DAB reagent solution
Between 2 to 4 min. (watch
reaction under microscope), stop
reaction with H2Od
13. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 3
min. afterwards
14. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
15. Mount Standard mount medium -
6.6 Immunohistochemistry – Biglycan
Primary antibodies: Rabbit Anti-Biglycan abcam ab49701
Secondary antibody: Anti-Rabbit IgG (Polymer detection kit, Vector Laboratories) (MP-
7401)
Pretreatment –Citric acid buffer: 0,1g citric acid, 450 ml H2Od, adjust pH to 6,1-6,4 and fill
up to 500 ml with H2Od) for 25 min. at 95°C (steamer). Chondroitinase ABC 0,2 U/ml (Sigma
cat nr. C3667): 40 ml H2Od, albumin serum bovine 0,01g, sodium acetate 0,81g, Tris base 0,3g.
Fixation: Formalin 24 hours.
Procedure Solution Time
1. Deparaffinate and keep in H2Od 2x Xilol, 3x 99°OH, 3x 95°OH, 2x
70°OH, H2Od 10 min. C/Xilol, 5 min. C/OH
2. Pretreatment with citrate buffer
pH 6 Citrate buffer pH6 (preheated)
25 min. at 95°C (steamer), 20 min.
cool down at R/T, 5 min. in H2Od.
3. Rinse three times in PBS, last
rinse at 37°C
0,1M PBS (pH7,2-7,4) (last rinse
preheated) 5 min. per solution
4. Pretreatment with
chondroitinase ABC Chondroitinase ABC 0,2U/ml 1 hour at 37°C
5. Rinse twice in cold
PBS+Tween20 and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
6. Endogenous peroxidase block 3% H2O2 1:9 in PBS 10 min.
7. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
8. Block non-specific antibody
binding sites Casein block 1:9 in H2Od 15 min.
9. Incubate primary antibody Rabbit Anti-Biglycan abcam 1:100
in PBS+Tween20
1 hour at R/T
10. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
11. Incubate secondary antibody Anti-rabbit IgG Ready-to-use
solution 30 min. at R/T
12. Rinse twice in PBS+Tween20
and once in PBS
0,1M PBS (pH7,2-7,4) + 3ml
Tween20 per liter PBS 5 min. per solution
13. Histochemistry: DAB DAB reagent buffer solution
Between 2 – 4 min. (watch reaction
under microscope), stop reaction
with H2Od
14. Counterstain: Hematoxylin Mayer’s Hematoxylin 10 sec., put under tap-water for 3
min. afterwards
15. Dehydrate 2x Alcohol 96%, 2x isopropanol,
3x toluene 2 min. per solution
16. Mount Standard mount medium -