Access to bifunctionalized biomolecular platforms using oxime ligation
Transcript of Access to bifunctionalized biomolecular platforms using oxime ligation
Accepted Manuscript
Access to bifunctionalized biomolecular platforms using oxime ligation
Karel Křenek, Radek Gaž ák, Gour Chand Daskhan, Julian Garcia, MicheleFiore, Pascal Dumy, Miroslav Šulc, Vladimír Křen, Olivier Renaudet
PII: S0008-6215(14)00181-5DOI: http://dx.doi.org/10.1016/j.carres.2014.04.020Reference: CAR 6737
To appear in: Carbohydrate Research
Received Date: 28 March 2014Revised Date: 28 April 2014Accepted Date: 29 April 2014
Please cite this article as: Křenek, K., Gaž ák, R., Daskhan, G.C., Garcia, J., Fiore, M., Dumy, P., Šulc, M., Křen,V., Renaudet, O., Access to bifunctionalized biomolecular platforms using oxime ligation, CarbohydrateResearch (2014), doi: http://dx.doi.org/10.1016/j.carres.2014.04.020
This is a PDF file of an unedited manuscript that has been accepted for publication. As a service to our customerswe are providing this early version of the manuscript. The manuscript will undergo copyediting, typesetting, andreview of the resulting proof before it is published in its final form. Please note that during the production processerrors may be discovered which could affect the content, and all legal disclaimers that apply to the journal pertain.
Access to bifunctionalized biomolecular platforms using oxime ligation
Karel Křenek,a Radek Gažák,a Gour Chand Daskhan,b Julian Garcia,b Michele Fiore,b
Pascal Dumy,b Miroslav Šulc,a Vladimír Křen*,a Olivier Renaudet*,b,c
a Institute of Microbiology, Academy of Sciences of the Czech Republic, Vídeňská
1083, CZ-14220 Praha 4, Czech Republic,
b Département de Chimie Moléculaire, UMR CNRS 5250 & ICMG FR 2607,
Université Joseph Fourier, BP53, 38041 Grenoble Cedex 9, France,
c Institut Universitaire de France, 103 boulevard Saint-Michel, 75005 Paris, France c
*E-mail: [email protected], [email protected]
Keywords
Chemoselective ligation; glycocluster; cyclopeptide; multivalency; oxime
Note
We previously reported the synthesis of original neoglycopeptide conjugates and the
evaluation of their immunological properties towards NK cells. Due to the inability to
reproduce the immunological data (Int. J. Mol. Sci. 2014, 15, 1271-1283), we have
recently decided to fully retract this paper (J. Am. Chem. Soc. 2014, 136, 1156-
1156). The present manuscript describes this synthetic strategy which was fully
validated, updated and enhanced with additional experiments.
Abstract
This paper describes an efficient oxime ligation strategy to prepare multivalent
conjugates wherein peptides alone or in combination with carbohydrate or oxime
group were coupled to a cyclopeptide scaffold. To demonstrate the versatility of this
approach, two classes of conjugates have been prepared. In one class, we attached
two or four peptide sequences to the cyclopeptide core together with free oxime
groups, while the second class contains an additional substitution with four or two
monosaccharides. The well-defined structure of these conjugates was confirmed by
high-resolution mass spectrometry.
Introduction
Carbohydrates and proteins are key structural motifs that exist in all living systems
where they play central roles in a wide range of biological events [1-3]. Synthetic
carbohydrates alone or combined with peptides and proteins represent promising
tools to decipher these complex biological processes as well as to develop potential
therapeutic and diagnostic agents [4-15]. However, chemical construction of such
structures is complicated due to difficulties associated with the low compatibility of
peptide/protein and carbohydrate chemistries, the fragility of glycosidic linkage and
the presence of multiple functionalities. Chemoselective and bioorthogonal strategies
have been developed to circumvent these difficulties and provide access to complex
bioconjugates [16-20]. Among these methods, we and other groups have focused on
oxime ligation that consists in using two functionalities namely, aldehyde and
aminooxy groups that are highly reactive in aqueous buffers [21]. This strategy has
been used successfully to synthesize numbers of original glycosylated constructs for
applications going from cell targeting to surface modifications [22-25].
As a part of a long term program, we have demonstrated the utility of cyclopeptide
scaffolds, commonly known as Regioselectively Addressable Functionalized
Templates (RAFT) [26], for the multivalent presentation of carbohydrate or peptide
ligands in well-defined spatial orientation [27-28]. The utilization of this scaffold is
indeed interesting to us due to its conformational stability and the presence of two
independent domains that can be functionalized regioselectively. In particular, we
demonstrated recently the robustness of oxime ligation to prepare well-defined
cyclopeptide-based glycodendrimers displaying clusters of carbohydrates on the
upper domain of the scaffold [29-33]. In this paper, we show that both addressable
domains of the cyclopeptide can be functionalized successively with peptides and
carbohydrates using an oxime-based ligation process. To demonstrate the versatility
of our strategy we have prepared two classes of compounds (Figure 1). In the first
one, we have combined two or four peptides together with free oxime groups, i.e.
compounds 1 and 3 respectively. The second classes display an additional
substitution with four or two GalNAc attached through an oxime ether linkage, i.e.
compounds 2 and 4, respectively.
Figure 1. Structure of oxime-peptide (1 and 3) and carbohydrate-peptide (2 and 4)
conjugates.
Results and Discussion
We have previously showed that the synthesis of glycodendrimers [31] using
successive oxime conjugations is efficient but should be performed following a strict
sequence to avoid side reactions. In particular, we have observed that the
simultaneous presence of both aminooxy and oxime functionalities within a single
molecule can induce trans-oximation reactions [31]. To avoid this problem, two
different cyclodecapeptide cores with orthogonal protecting groups have been
prepared (Scheme 1) as key intermediates for the nonglycosylated and glycosylated
peptide conjugates 1-4.
Scheme 1. Synthesis of oxime-peptide (1) and carbohydrate-peptide (2) conjugates.
The first cyclopeptide 5 display four lysines pre-functionalized with serines [34] on the
upper domain and two lysines protected with N-(1-(4,4-dimethyl-2,6-
dioxocyclohexylidene)ethyl) (Dde) [35] on the lower domain. Dde protecting groups
were first removed using a solution of 3% of hydrazine in DMF. N-
Hydroxysuccinimidyl ester of ethoxyethylidene aminooxy acetic acid linker (Eei-Aoa-
OSu) [36] was next coupled to the free lysines to afford compound 6. Final
deprotection of the four serine and two aminooxy moieties was performed by
acidolysis with a solution of trifluoroacetic acid/triisopropylsilane/water (TFA/TIS/H2O,
95:2.5:2.5) to provide the fully deprotected scaffold 7.
The molecular assembly was performed using successive oxime coupling and
aldehyde formation. For this purpose, we have synthesized a pentapeptide that
contains diverse functionalities (i.e. carboxylic acids and alcohol). This model peptide
was terminated with a serine which can be easily converted into glyoxylic aldehyde (-
COCHO) by oxidative cleavage with sodium periodate [37-38]. The oxime coupling
was performed with an excess of the peptide-COCHO and the aminooxy-containing
scaffold 7 in a mixture of CH3CN/H2O containing 0.1% of TFA. The conversion was
complete and we obtained quantitatively a peptide conjugate displaying two peptide
and four serine moieties. An additional treatment with sodium periodate afforded four
COCHO functions that were used to conjugate either hydroxylamine or aminooxy
αGalNAc [39] to the second addressable domain of the scaffold. The oxime coupling
was performed under similar conditions and the desired compounds 1-2 were
obtained quantitatively as confirmed by analytical HPLC of the crude mixtures (Figure
2).
(a)
(b)
Figure 2. HPLC profile (linear gradient: 5 to 90% CH3CN in 15 min, λ = 250 nm) of
the crude reaction mixture of (a) compound 1; (b) compound 2.
We followed the same procedure to prepare the conjugates 3 and 4 from the scaffold
8, which contains reverse functionalities, i.e. two pre-functionalized and four
protected lysines (Scheme 2). No difference of reactivity was observed and both
compounds 3 and 4 were obtained as pure products after HPLC purification in similar
yields.
Scheme 2. Synthesis of oxime-peptide (3) and carbohydrate-peptide (4) conjugates.
The fragmentation of oxime ether linkages during ionization process of mass
spectroscopy spectrometry analysis are well documented in the literature [31, 33, 40].
To avoid this problem and received high resolution MS data we have chosen matrix-
assisted laser desorption/ionization ion source combined with Fourier transform ion
cyclotron resonance as detector, time-of-flight mass spectroscopy (MALDI-TOFFT-
ICR-MS) for mass spectrometry experiments. The average monoisotopic molecular
weight of the synthesized conjugates 1-4 was measured by MALDI-TOF FT-ICR MS
mass spectroscopy analysis using α-cyano-4-hydroxycinnamic acid (CCA) or 2,5-
dihydrobenzoic acid (DHB) as MALDI matrices for compounds 1-3 and 4,
respectively (Table 1).
Table 1 MALDI-TOF FT-ICR MS analysis of conjugates 1-4.
Cpnd Formula Calcd. mass Found mass (m/z)
Error (ppm)
1 C118H188N32O46 2812.324768 [M+Na]+ 2812.31664 2.9
2 C150H240N36O66 3624.642258 [M+Na]+ 3624.64305 0.3
3 C174H278N42O70 4076.955767 [M+H]+ 4076.95899 0.8
4 C190H304N44O80 4483.114512 [M+H]+ 4483.19100 17.0
We next performed molecular modelling study with peptide-glycoconjugates 2 and 4.
Energy minimizations were calculated in vacuo using Insight II/Discover. We first
observed that minimized structures are conformationally stable and the cyclopeptide
remains rigid in both cases. In addition, no steric clashes were observed between the
peptides fragments and the carbohydrates attached onto both addressable domains
of the cyclopeptide. This suggests that such scaffolds can be functionalized with
diverse recognition or structural elements in well-defined spatial orientation without
interfering with their biological function.
(a)
(b)
Figure 3. Molecular modelling of (a) compound 2; (b) compound 4.
Conclusion
In summary, we have described a straightforward strategy for the synthesis of
bifunctionalized cyclopeptide scaffolds bearing peptide and carbohydrates on two
separated addressable domains. By employing successive and reproducible oxime
ligations, new classes of peptide-conjugates 1-3 and 2-4 were prepared using
attachment of either peptide-aldehyde, hydroxylamine or aminooxy αGalNAc onto
RAFT scaffolds displaying aminooxy and masked aldehyde groups. The well-defined
structure of these conjugates was determined by high-resolution mass spectrometry.
Molecular modelling study also confirmed the spatial separation of both addressable
domains, thus providing an attractive biomolecular platform for diverse biomedical
applications.
Experimental
General methods. All chemical reagents were purchased from Aldrich (Saint-
Quentin Fallavier, France) or Acros (Noisy-Le-Grand, France) and were used without
further purification. Protected amino acids and Fmoc-Gly-Sasrin resin were obtained
from Advanced ChemTech Europe (Brussels, Belgium), Bachem Biochimie SARL
(Voisins-Les-Bretonneux, France) and France Biochem S.A. (Meudon, France).
PyBOP was purchased from France Biochem. Reaction progress was monitored by
reverse-phase HPLC on Waters equipment using C18 columns. Analytical HPLC
(Nucleosil 120 Å 3 µm C18 particles, 30 × 4.6 mm2) was performed at 1.3 mL/min and
preparative HPLC (Delta-Pak 300 Å 15 µm C18 particles, 200 × 25 mm2) at 22
mL/min with UV monitoring (214 nm and 250 nm) using a linear A–B gradient (buffer
A: 0.09% TFA in H2O; buffer B: 0.09% TFA in 90% CH3CN). Routine mass spectra
were recorded on a VG Platform II by electron spray ionization in the positive mode.
Accurate mass spectra were obtained for compounds 1-4 on a MALDI-APEX Qe-FT-
ICR mass spectrometer equipped with a 9.4 T superconducting magnet and a ion
Combi Source (Bruker-Daltonics, Bremen, Germany). Positive mass spectra were
obtained by accumulating ions in the collision hexapole and running the quadrupole
mass filter in non-mass-selective RF-only mode so that ions of a broad m/z range
(850–5000) were allowed to enter the analyzer cell. All spectra were calibrated
externally using the monoisotopic [M+H]+ ions of Pepmix2 calibrant (Bruker-
Daltonics, Germany). A 5 mg/mL solution of CCA or 10 mg/mL solution DHB in 50%
CH3CN and 0.3% CH3CO2H was used as matrix. A 1 µL of sample dissolved in
CH3OH was mixed with a 1.0 µL of the matrix solution. A 0.3 µL of mixture was
loaded on the target and allowed to dry at ambient temperature.
Synthesis of compound 5. The linear precursor peptide (0.25 mmol; analytical RP-
HPLC: Rt = 12.2 min (5 to 100% B in 15 min, 214 nm); ESI-MS: calcd. for
C118H203N20O31 2397.5 [M+H]+; found: m/z 2397.9) was cyclized in CH2Cl2 (500 mL)
with PyBOP (156 mg; 0.3 mmol) and DIPEA (82 µL; 0.5 mmol; pH 8). After stirring for
1 h at room temperature, the solution was evaporated and peptide 5 was recovered
by precipitation in Et2O. Analytical RP-HPLC: Rt = 14.9 min (5 to 100% B in 15 min,
214 nm); ESI-MS: calcd. for C118H201N20O30 2378.5 [M+H]+; found: m/z 2378.1.
Synthesis of compound 6. Protected cyclodecapeptide 5 (0.25 mmol) was treated
for 1 h at room temperature with a solution of 3% hydrazine in DMF (50 mL). After
evaporation and precipitation in Et2O, Eei-Aoa-OSu (129 mg; 0.5 mmol) and DIPEA
(83 µL; 0.5 mmol) were added and the solution was stirred in DMF (25 mL). The
coupling reaction was monitored by analytical HPLC and reached completion after 2
h. The solvent was then evaporated and the excess of the activated ester removed
by precipitation in Et2O. Yield: 52% (300 mg) from the corresponding linear peptide
sequence (3 steps); analytical RP-HPLC: Rt = 14.1 min (5 to 100% B in 15 min, 214
nm); ESI-MS: calcd. for C110H195N22O32 2336.4 [M+H]+; found: m/z 2336.2.
Synthesis of compound 7. Crude compound 6 (196 mg; 0.084 mmol) was treated
with a cocktail of TFA/TIS/H2O (50 mL; 95:2.5:2.5). After 2 h of stirring at room
temperature, the solution was evaporated and fully deprotected cyclopeptide 7 was
recovered by precipitation in Et2O. Analytical RP-HPLC: Rt = 5.7 min (5 to 60% B in
15 min, 214 nm); ESI-MS: calcd. for C66H119N22O22 1571.9 [M+H]+; found: m/z
1571.9.
Synthesis of compound 8. Cyclodecapeptide 8 was synthesized for the linear
peptide precursor (0.25 mmol; analytical RP-HPLC: Rt = 10.5 min (5 to 100% B in 15
min, 214 nm); ESI-MS: calcd. for C114H185N18O27 2239.3 [M+H]+; found: m/z 2238.6)
by following the procedure described for 5. Analytical RP-HPLC: Rt = 12.9 min (5 to
100% B in 15 min, 214 nm); ESI-MS: calcd. for C114H183N18O26 2220.4 [M+H]+; found:
m/z 2220.1.
Synthesis of compound 9. Compound 9 was synthesized by following the
procedure described for 7. Analytical RP-HPLC: Rt = 5.7 min (5 to 60% B in 15 min,
214 nm); ESI-MS: calcd. for C64H115N22O22 1543.8 [M+H]+; found: m/z 1543.6.
Synthesis of compound 1. Peptide 7 (14 mg; 0.0069 mmol) was dissolved in a
mixture of CH3CN/H2O/TFA (2 mL; 1:1:0.1) and peptide-CHO (27 mg; 0.041 mmol)
was added to the solution. The mixture was stirred at 37°C overnight then acetone (1
mL) was added. The resulting peptide conjugate (was used without further treatment.
Analytical RP-HPLC: Rt = 12.6 min (5 to 40% B in 15 min, 214 nm); ESI-MS: calcd for
C122H205N32O46 2854.5 [M+H]+; found: m/z 2854.3. Sodium periodate (59 mg; 0.28
mmol) was then added to the crude solution and the mixture purified by RP-HPLC
after 1 h to isolate the corresponding oxidized conjugate in 95% yield (18 mg) from 7
(2 steps). Analytical RP-HPLC: Rt = 12.9 min (5 to 60% B in 15 min, 214 nm). This
compound (9 mg; 0.0033 mmol) was finally stirred at 37°C with hydroxylamine
hydrochloride (1.8 mg; 0.026 mmol) in CH3CN/H2O/TFA (2 mL; 1:1:0.1). After RP-
HPLC purification, compound 1 was obtained with a 70% yield (6.5 mg). Analytical
RP-HPLC: Rt = 7.6 min (5 to 100% B in 15 min, 214 nm); MALDI-FT-ICRTOF HRMS:
calcd for C118H188N32O46 2812.324768 [M+Na]+; found: 2812.31664.
Synthesis of compound 2. Compound 2 was obtained from the previous oxidized
peptide (9 mg; 0.0033 mmol) and aminooxy αGalNAc (8 mg; 0.033 mmol) in
CH3CN/H2O/TFA (2 mL; 1:1:0.1) following the procedure described for 1. Yield: 80%
(9.5 mg); analytical RP-HPLC: Rt = 7.1 min (5 to 100% B in 15 min, 214 nm); MALDI-
FT-ICRTOF HRMS: calcd for C150H240N36O66 3624.642258 [M+Na]+; found:
3624.64305.
Synthesis of Compound 3. Compound 3 was prepared following the 3-step
procedure described for 1. Compound 9 (12 mg; 0.0068 mmol) was first treated with
peptide-CHO (28 mg; 0.041 mmol). The resulting conjugate was then oxidized with
sodium periodate (29 mg; 0.14 mmol) in water (7 mL) and purified by RP-HPLC after
1 hour. Yield: 91% (25 mg) from 9 (2 steps); analytical RP-HPLC: Rt = 8.3 min (5 to
100% B in 15 min, 214 nm). This peptide (11 mg; 0.0027 mmol) was reacted with
hydroxylamine hydrochloride (0.8 mg; 0.011 mmol) in CH3CN/H2O/TFA (2 mL;
1:1:0.1) to obtain 3 after purification. Yield: 68% (7.5 mg); analytical RP-HPLC: Rt =
8.4 min (5 to 100% B in 15 min, 214 nm); MALDI-FT-ICRTOF HRMS: calcd for
C174H278N42O70 4076.955767 [M+H]+; found: 4076.95899.
Synthesis of compound 4. Compound 4 was obtained from the previous oxidized
peptide (14 mg; 0.0034 mmol) and aminooxy αGalNAc (3 mg; 0.014 mmol) in
CH3CN/H2O/TFA (2 mL; 1:1:0.1) following the procedure described for 3. Yield: 66%
(10 mg); analytical RP-HPLC: Rt = 8.1 min (5 to 100% B in 15 min, 214 nm); MALDI-
FT-ICRTOF HRMS: calcd for C190H304N44O80 4483.114512 [M+H]+; found:
4483.19100.
Molecular modeling. Structure calculations were performed in vacuo using InsightII /
Discover (Version 2005, Accelrys, SanDiego,CA,USA) software, and the energy of
the system was calculated by the consistent CVFF force field (version 2.3). To
shorten the range of Coulomb interaction, a distance-dependent relative dielectric
constant, εr, was used (εr = 4r). The resulting molecule was subjected to 2000
iterations of steepest descent minimization, followed by 3500 iterations of conjugate
gradient minimization and the convergence of minimization was followed until the
RMS derivative was less than 0.01 kcal.mol-1.
Acknowledgements
This work was supported by the Université Joseph Fourier (UJF), the Centre National
de la Recherche Scientifique (CNRS), the “Communauté d’agglomération Grenoble-
Alpes Métropole” (Nanobio Program), the Ligue contre le cancer (MF) and the ANR-
12-JS07-0001-01 “VacSyn” (GCD). O.R. acknowledges support from the Labex
Arcane (ANR-11-LABX-003), and O.R.&V.K. acknowledge European project
“MultiGlycoNano” ESF COST chemistry action CM1102 (MSMT LD13042).
References
1. Varki, A. Glycobiology 1993, 3, 97-130.
2. Collins, B. E.; Paulson, J. C. Curr. Opin. Chem. Biol. 2004, 8, 617-625.
3. Imberty, A.; Varrot, A. Curr. Opin. Struct. Biol. 2008, 18, 567-576.
4. Sears, P.; Wong, C.-H. Science 2001, 291, 2344-2350.
5. Bertozzi, C. R.; Kiessling, L. L. Science 2001, 291, 2357-2363.
6. Pratta, M. R.; Bertozzi, C. R. Chem. Soc. Rev. 2005, 34, 58-68.
7. J. D. Warren, Geng, X.; Danishefsky, S. J. Top. Curr. Chem. 2007, 267, 109-141.
8. Seeberger, P. H.; Werz, D. B. Nature, 2007, 446, 1046-1051.
9. Horlacher, T.; Seeberger, P. H. Chem. Soc. Rev. 2008, 37, 1414-1422.
10. Gamblin, D. P.; Scanlan, E. M.; Davis, B. G. Chem. Rev. 2009, 109, 131-163.
11. Gaidzik, N.; Westerlind, U.; Kunz H. Chem. Soc. Rev. 2013, 42, 4421-4442.
12. Rouhanifard, S. H.; Nordstrøm, L. U.; Zheng, T.; Wu, P. Chem. Soc. Rev. 2013,
42, 4284-4296.
13. Park, S.; Gildersleeve, J. C.; Blixt, O.; Shin, I. Chem. Soc. Rev. 2013, 42, 4310-
4326.
14. Johnson, M. A.; Bundle, D. R. Chem. Soc. Rev. 2013, 42, 4327-4344.
15. Unverzagt, C.; Kajihara, Y. Chem. Soc. Rev. 2013, 42, 4408-4420.
16. Kolb, H. C.; Finn, M. G.; Sharpless, K. B. Angew. Chem. Int. Ed. 2001, 40, 2004-
2021.
17. Meldal, M.; Tornøe, C. W. Chem. Rev. 2008, 108, 2952-3015.
18. Dirksen, A.; Dawson, P. E. Curr. Opin. Chem. Biol. 2008, 12, 760-766.
19. Sletten, E. M.; Bertozzi, C. R. Angew. Chem. Int. Ed. 2009, 48, 6974-6998.
20. Dondoni, A.; Marra, A. Chem. Soc. Rev. 2012, 41, 573-586.
21. Rose, K. J. Am. Chem. Soc. 1994, 116, 30-33.
22. Lemieux, G. A.; Bertozzi, C. R. Trends Biotechnol. 1998, 16, 506-513.
23. Peri, F.; Nicotra, F. Chem. Commun. 2004, 623-627.
24. Hudak, J. E.; Yu, H. H.; Bertozzi, C. R. J. Am. Chem. Soc. 2011, 133, 16127-
16135.
25. Ulrich, S.; Boturyn, D.; Marra, A.; Renaudet, O.; Dumy, P. Chem. Eur. J. 2014, 20,
34-41.
26. Dumy, P.; Eggleston, M.; Cervigni, S.; Sila, U.; Sun, X.; Mutter, M. Tetrahedron
Lett. 1995, 36, 1255-1258.
27. Boturyn, D.; Defrancq, E.; Dolphin, G. T.; Garcia, J.; Labbé, P.; Renaudet, O.;
Dumy, P. J. Pept. Sci., 2008, 14, 224-240.
28. Galan, M. C.; Dumy, P.; Renaudet, O. Chem. Soc. Rev. 2013, 42, 4599-4612.
29. Renaudet, O.; Dumy, P. Org. Lett. 2003, 5, 243-246.
30. André, S.; Renaudet, O.; Bossu, I.; Dumy, P.; Gabius, H.-J. J. Pept. Sci. 2011, 17,
427-437.
31. Bossu, I.; Šulc, M.; Křenek, K.; Dufour, E.; Garcia, J.; Berthet, N.; Dumy, P.; Křen,
V.; Renaudet, O. Org. Biomol. Chem. 2011, 9, 1948-1959.
32. Berthet, N.; Thomas, B.; Bossu, I.; Dufour, E.; Gillon, E.; Garcia, J.; Spinelli, N.;
Imberty, A.; Dumy, P.; Renaudet, O. Bioconjugate Chem. 2013, 24, 1598-1611.
33. Thomas, B.; Berthet, N.; Garcia, J.; Dumy, P.; Renaudet, O. Chem. Commun.
2013, 49, 10796-10798.
34. Foillard, S.; Ohsten Rasmusssen, M.; Razkin, J.; Boturyn, D.; Dumy, P. J. Org.
Chem. 2008, 73, 983-991.
35. Bycroft, B. W.; Chan, W. C.; Chabra, S. R.; Hone, N. D. J. Chem. Soc. Chem.
Commun. 1993, 778-779.
36. Duléry, V.; Renaudet, O.; Dumy, P. Tetrahedron 2007, 63, 11952-11958.
37. Geoghegan, K. F.; Stoh, J. G. Bioconjugate Chem. 1992, 3, 138-146.
38. El-Mahdi, O.; Melnyk, O. Bioconjugate Chem. 2013, 24, 735-765.
39. Renaudet, O.; Dumy, P. Org. Biomol. Chem. 2006, 4, 2628-2636.
40. Nazarpack-Kandlousy, N.; Chernushevich, I. V.; Meng, L. J.; Yang, Y.; Eliseev, A.
V. J. Am. Chem. Soc. 2000, 122, 3358-3366.