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7/27/2019 A Strategy for Adding Multiple Reporter Groups to Oligonucleotides by Tom Fleming
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UNIVERSITY OF SOUTHAMPTON
FACULTY OF NATURAL AND ENVIRONMENTAL SCIENCES
School of Chemistry
MChem 3rd Year Dissertation
A STRATEGY FOR ADDING MULTIPLE REPORTER GROUPS TO
OLIGONUCLEOTIDES
by Thomas Fleming
Supervisors:
Dr. Nittaya GaleProfessor Tom Brown
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Abstract
Advances in DNA functionalisation impact on medical, material and
forensic science, bio, nano and gene technology.1 Oligonucleotides as genetic
probes offer rapid detection of complementary sequences with sufficient
sensitivity to distinguish between sequences containing single base pair
mismatches and normal gene sequences. Fluorescent labelling is a central
feature of probe technologies. Single labelling is easily accomplished, but with
increasingly sophisticated probes and demanding application conditions, such as
sub-femtomolar target sequence concentrations, the demand for a convenient,
effective and flexible, multiple internal labelling strategy is of rising importance.
Current labelling strategies commonly use expensive dye-functionalisedphosphoramidite nucleosides with limited range of dye options. Alternatively,
monomers bearing appropriate functional groups can be incorporated into
oligonucleotides and subsequently reacted with functionalised labels amine-
NHS ester coupling, for example. This approach is constrained by compatibility
with the phosphoramidite method and labelling reaction efficiencies.
A synthetic strategy is reported that offers an efficient route to multiple
labelling or modification of an oligonucleotide. Orthogonal protecting group
strategies enable solid phase conjugation to phosphoramidite derivatives of label
molecules. Five modified nucleoside phosphoramidites have been synthesised
and incorporated into DNA oligonucleotides. Modifications at the 2- and 5-
position of pyrimidine nucleosides with Fmoc, Levulinyl and TBDMS protecting
groups have been investigated. A HyBeacon probe, multiply labelled with FAM
was synthesised and melting studies indicated successful discrimination between
mutant and wild-type target sequences, with biophysical results very close toconventional probe technologies. Advantages of this strategy include
compatibility with the phosphoramidite method, practical convenience, broad
scope of label options and high-yielding label installation.
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Contents
ABSTRACT' I!
ACKNOWLEDGEMENTS' 3!
ABBREVIATIONS'&'ACRONYMS' 4!
INTRODUCTION' 1!
Nucleic'Acid'Structure5' 2!Nucleosides!&!Nucleotides! 2!Watson1Crick!Base!Pairing!Specificity! 4!Monomers!to!Oligos! 5!
Oligonucleotides' 7!Oligonucleotide!Synthesis! 7!The!Phosphoramidite!Monomer! 9!The!Phosphoramidite!Cycle! 0!
Oligonucleotides'in'Genetic'Analysis' 18!
HyBeacon'Probes' 19!
Labelling'Strategies' 21!Previous!Strategies!for!Multiple!Labelling!of!Oligonucleotides! 25!
A!New!Strategy!for!Adding!Multiple!Reporter!Groups!to!Oligonucleotides! 3!
Retrosynthesis'&'Alternative'Approaches' 34!
RESULTS'&'DISCUSSION' 37!
Monomer'Design' 37!
Synthetic'Approach' 41!51O1(4,41Dimethoxytrityl)121O1(21(91fluorenylmethyloxycarbonyl)ethyl)151methyluridine131 O1
(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!)! 4!51O1(4,41Dimethoxytrityl)151(31(91fluorenylmethyloxycarbonyl)1propynyl)121deoxyuridine131 O1
(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!2)! 46!51O1(4,41Dimethoxytrityl)121O1(61(tert1butyldimethylsilyloxy)hexanamido)ethyl)151
methyluridine131O1(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!3)! 49!51O1(4,41Dimethoxytrityl)151(31(61(tert1butyldimethylsilyloxy)1hexanamido)1propynyl)121
deoxyuridine131O1(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!4)! 55!51O1(4,41Dimethoxytrityl)151(31(61(levulinyloxy)1hexanamido)1propynyl)121deoxyuridine131 O1
(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!5)! 56!51O1(4,41Dimethoxytrityl)151(31(61(91fluorenylmethyloxycarbonyl)1hexanamido)1propynyl)121
deoxyuridine131O1(O121cyanoethyl1N,N1diisopropyl)!phosphoramidite!(Monomer!6)! 57!
Oligonucleotide'Synthesis'Strategy' 59!Approach!A! 59!
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Approach!B! 6!Approach!C! 66!HyBeacon!Studies! 67!
CONCLUSION'&'FUTURE'WORK' 71!
Conclusion' 71!
Future'Work' 72!Variant!Labelling! 72!Branching!Oligonucleotides! 73!Cell!Imaging! 74!Combinatorial!Labelling! 74!
EXPERIMENTAL' 77!
General'Methods' 77!General! 77!Spectroscopic! 77!Phosphitylation! 78!The!Phosphoramidite!Method! 78!Oligonucleotide!Purification!&!Characterisation! 79!Melting!Analysis! 79!
Synthesis'of'Modified'Monomers' 80!MONOMER!! 80!MONOMER!2! 85!MONOMER!3! 88!MONOMER!4! 92!MONOMER!5! 94!
REFERENCES' 99!
APPENDICES' 1!
Interim'Report' 1!Introduction! !Results!&!Discussion! 4!Proposals!for!Future!Work! 7!References! 0!
Oligonucleotide'Synthesis'Optimisation' 11!Conditions! !
Mass'Spectrometry'Results' 12!HPLC1MS!&!Deconvoluted!Peaks! 4!
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Acknowledgements
Thank you to Professor Tom Brown for taking account of my interests and
personal ambitions and assigning me a project that suited them so well. To be
given a project with real significance in the progression of the field is an honour
and knowing that my work is of some importance has been a great motivator.
I would very much like to thank Dr. Nittaya Gale for working closely with
me on this project and for making it both enjoyable and the success that it has
been. I have learnt the rewards of persistence in problem solving and I have also
learnt to remain positive when faced with disappointment or mistakes an asset
to a healthy work-attitude that extends beyond the laboratory. I have been
privileged to work alongside someone who has demonstrated and passed on
such a high standard of laboratory skills and practices.
Thank you to Dr. Simon Gerrard for always taking the time to answer my
questions. Thank you to Xiaomei Ren for submitting many spectroscopic samples
on my behalf. Thank you to Dr. Afaf El-Sagheer for on-hand advice, for keeping
an eye on me and for making me go home when its getting late. Working
alongside such hard-working, exceptional people has been inspiring.
For their love, support and interest in all that I do, thank you to my Mum
and Dad.
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Abbreviations & Acronyms
A adenine
angstrom(s)
Ac acetyl
AcOH Acetic acid
Act activating group
aq. aqueous
bp base pair(s)
br broad (spectral)
Bu n-Bu normal (primary) butyl
tBu tert-butylBz benzoyl
C cytosine
C degrees Celsius
cat catalytic
CEP-(Cl) 2-Cyanoethyl N,N-diisopropyl(chloro) -
phosphoramidite
cm centimetre(s)
conc. concentrated
COSY correlation spectroscopy
CPG controlled pore glass
chemical shift in parts per million downfield from
tetramethylsilane
d day(s); doublet (spectral); deci; deoxy
DCA dichloroacetic acid
DCC N,N-dicyclohexylcarbodiimideDCM dichloromethane
DEA diethylamine
DEPT distortionless enhancement bypolarisation transfer
DIC diisopropylcarbodiimide
DIPEA diisopropylamine (Hnigs base)
DMAP 4-(N,N-dimethylamino)pyridine
DMF dimethylformamide
DMSO dimethylsulfoxide
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DMTr 4,4-dimethoxyltrityl
DNA 2-deoxyribonucleic acid
ds double-stranded
E1CB
unimolecular (conjugate base) elimination
EDC 1-ethyl-3-(3-dimethylaminopropyl)carbodiimide
EDTA ethylenediaminetetraacetic acid
eq. equivalent
ESI electrospray ionisation
Et ethyl
Et2O diethyl ether
EtOAc ethyl acetate
EtOH ethanolFAM fluorescein amidite
FCC flash column chromatography
FISH fluorescence in-situhybridisation
Fmoc 9-fluorenylmethoxycarbonyl
FT-ICR Fourier transform ion cyclotron resonance
G guanine
g gram(s)
h hour(s)
HPLC high-performance liquid chromatography
HRMS high-resolution mass spectrometry
Hz hertz
iB iso-butyl
iPrOH iso-propanol
J coupling constant (in NMR spectrometry)
K Kelvin(s) (absolute temperature)
L litre, dm3
Lev levulinyl
LPE light petroleum ether
wavelength
lit. literature value (abbreviation used with full stop)
LRMS low-resolution mass spectrometry
micro
m multiplet (spectral); metre(s); milliM molar (moles per litre); mega
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M+ parent molecular ion
Me methyl
MeCN acetonitrile
MeOH methanol
MHz megahertz
min minute(s)
mM millimolar (millimoles per litre)
mol mole(s); molecular (as in mol wt)
MS mass spectrometry
MW
mol. wt. molecular weight
m/z mass-to-charge ratio
n normalNHS N-hydroxysuccinimide
NMI N-methylimidazole
nm nanometre(s)
NMR nuclear magnetic resonance
NTP nucleoside triphosphate
OD optical density
ONT oligonucleotide
PAGE polyacrylamide gel electrophoresis
PG protecting group
Ph phenyl
pip piperidine
ppm part(s) per million
Pr propyl
iPr isopropyl
PS polystyrene
py pyridine
q quartet (spectral)
Rep reporter group
Rf
retention factor (in chromatography)
RNA ribonucleic acid
RP-HPLC reverse phase high performance liquid
chromatography
rs residue (gene, protein)rt room temperature
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s singlet (spectral); second(s)
SN1 unimolecular nucleophilic substitution
SN2 bimolecular nucleophilic substitution
SNP singlenucleotide polymorphism
STR short tandem repeats
Su succinimide
t triplet (spectral)
t time; temperature in units of degrees Celsius (C)
T absolute temperature in units of Kelvins (K); thymine
Tac2O tertbutylphenoxyacetyl acetic anhydride
TAMRA carboxytetramethylrhodamine
TBAF tetrabutylammonium fluorideTBDMS tert-butyldimethylsilyl chloride
TCA trichloroacetic acid
TEA triethylamine
TEAA tetraammonium acetate
tert tertiary
TFA trifluoroacetic acid
THF tetrahydrofuran
TLC thin-layer chromatography
TM
melting temperature
TMS trimethylsilyl; tetramethylsilane
TR
retention time
UV ultraviolet
vis visible
vol volume
v/v volume per unit volume (volume-to-volume ratio)
wt. weight
w/w weight per unit weight (weight-to-weight ratio)
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Introduction
DNA is a biological information storage molecule that contains the genetic
code a sequence made from an alphabet consisting of only four letters (A, G, C
& T), yet holds the fundamental instructions for growth and proliferation of
almost all living systems.3 With entire complex life forms operating on such
fundamentally simple instructions, it is not surprising that small errors in this
code can have serious consequences. Diagnostic techniques that interrogate the
genetic code are invaluable tools for forensic and medical science.4
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Nucleic Acid Structure5
Nucleosides & Nucleotides
DNA is a biological macromolecule (figure 1). In nature, it exists
predominantly in the double stranded DNA double helix form. Each strand of the
helix is a polymer of nucleotides, figure 6, of which there are four possibilities,
dependent on which of the four heterocyclic bases they contain (figure 2).
Figure 1 B-DNA -The Iconic Double Stranded Helix2
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Figure 2 Purines and pyrimidines - the four heterocyclic bases of DNA, nucleoside & nucleotide
structure and atom numbering convention
The 2-deoxyterminology indicates the absence of a hydroxyl group at the
2-position of the ribose sugar, the main structural differentiation between DNA
and ribonucleic acids (RNA), which has a hydroxyl group at the 2-position. The
other distinguishing feature between DNA and RNA is the replacement of the
pyrimidine thymine (T), DNA, with uracil (U), RNA (figure 3).
Figure 3 Distinctions in heterocyclic bases in DNA/RNA
N
NN
N
NH2
NH
NN
N
O
NH2
N
N
NH2
O
NH
N
O
O
O
OH
ROBase
Base =(A) (G) (C) (T)
Purine Pyrimidine
R = H, Nucleoside
R = PO32-, Nucleotide
1'
2'3'
4'
5'
1
2
3
4
5
67
1
2
3
4
5
68
9
A = Adenine
G = Guanine
C = Cytosine
T = Thymine
Heterocyclic
NH
N
O
O
NH
N
O
O
Uracil (RNA) Thymine (DNA)
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Watson-Crick Base Pairing Specificity
The two antiparallel strands of the DNA duplex are said to be
complementary in their pairing. Each base hydrogen bonds specifically to its
complementary, or opposite, partner. The two strands are bound primarily by
this specific hydrogen-bonding pattern and the overall structure is additionally
stabilised by other non-covalent interactions such as base-stacking and entropic
contributions from the internally-positioned hydrophobic bases. It is the specific
hydrogen bonding between bases, however, that confers information storage
ability.
Figure 4 Watson-Crick Base Pair Hydrogen Bonding Scheme
James Watson and Francis Crick elucidated the structure of the DNA double
helix in 1953 with the help of the work of several other prominent researchers.
The base-pairing scheme (figure 4) was named in their honour. Watson-Crick
base pairing specificity is the basis upon which DNA can accurately copy itself.
During semi-conservative DNA replication, the helix is separated and the twoseparated halves of the parent provide all the information required for the
formation of two exact-copy daughter strands (figure 5).
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Figure 5 The semi-conservative nature of DNA replication, a consequence of Watson-Crick base
pairing specificity2
The key concept is that DNA is an accurate and consistent source of
biological information.
Monomers to Oligos
Polymeric nucleoside strands are connected through a 3,5-
phosphodiester bond (figure 6) giving DNA/RNA strands intrinsic directionality.
At physiological pH (7.4), the phosphate groups exist in their deprotonated,
anionic form, hence the name - nucleic acid. The two strands of a double helix
run in opposite directions to each other, termed antiparallel.
Parent Strand
Daughter Strands
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Figure 7 Three nucleic acid duplex conformations, A, B & Z. B is the most common2
Oligo, from Greek few, is the prefix attached to nucleotides to describe
polymeric single nucleic acid strands from anywhere between a dinucleotide
(dimer) to several hundred mers. Oligonucleotides will bind readily to form
stable duplexes with complementary sequences. It is this key aspect of the
oligonucleotide that makes it a perfect tool for investigating specific DNA
sequences, a tool with applications in diverse fields due to the significance of the
information that DNA contains.
Oligonucleotides
Oligonucleotide Synthesis
The chemical synthesis of oligonucleotides follows a solid-phase strategy
conceived in 1959 by Bruce Merrifield. His invention that was originally designed
for the task of peptide synthesis was awarded the 1984 Nobel Prize in Chemistry.
Application of the solid-phase approach to oligonucleotide synthesis retains all
the advantages of the Nobel Prize-winning conception.6
The phosphoramiditemethod has opened new doors in hybrid DNA research, stimulating scientific
A B Z
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progress in biochemistry, molecular biology, pharmacology, drug design &
development and gene technology.
Synthesis on a solid matrix enables synthesis of nucleotide polymer
lengths of up to around 200 - far longer than would otherwise be possible.1b
Complex purifications are replaced by quick, simple and efficient washes that
regularly achieve stepwise yields in excess of 99.5% - a prerequisite for the
viability of longer oligonucleotide syntheses. Large reagent excesses can be
applied, driving reactions rapidly to completion. The nature of the process is
well-suited to computerised automation, enabling highly efficient and
reproducible syntheses.
Table 1 Impact of coupling efficiencies on overall yield
Length
of Oligo
Average Stepwise Yield (Coupling Efficiency)
90% 95% 97% 98.5% 99.5%
10 38.7 63.0 76.0 87.3 95.6
FinalYield(
%)20 13.5 37.7 56.1 75.0 90.9
50 - 8.1 22.5 47.7 78.2
100 - - 4.9 22.4 60.9
150 - - 1.1 10.5 47.4
200 - - - 4.9 36.9
As demonstrated in table 1, high-yielding coupling reactions are necessary
for the successful synthesis of oligonucleotides of reasonable length.
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The Phosphoramidite Monomer
The key aspect of nucleoside building blocks is the phosphoramidite
moiety at the 3-alcohol (figure 8), which undergoes reaction with exposed 5-
alcohol groups under mild acid catalysis. The DMTr group that protects the 5-
alcohol is also of importance as it prevents off-target polymerisation of the
monomers.
Figure 8 Highlighted features of a dT phosphoramidite monomer
HN
O
O N
O
O
O
PO
NN
O
O
Dimethoxytrityl moiety
2-Cyanoethyl N,N-diisopropylphosphoramidite moiety
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The Phosphoramidite Cycle
Oligonucleotide synthesis via the phosphoramidite method begins with a
single protected nucleoside that is covalently attached to a solid support, often
polystyrene or controlled-pore glass (CPG) granules 500-3000 in diameter,
within the confines of a column. Elongation of the nucleotide chain occurs
through the sequential addition of phosphoramidite monomers by a series of
chemical processes that constitute the phosphoramidite cycle (figure 10).
Figure 9 Diagram of solid-phase oligonucleotide column
The functionalised resin column (figure 9) is loaded onto the DNA
synthesiser and subjected to the synthesis cycle.
Solvents & reagent solutionspass through freely
Filters retain growingoligonucleotides onsolid supports
Insoluble solid support(resin) particles anchoroligonucleotides withinthe column
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Table 2 A typical DNA oligonucleotide synthesis cycle for a 0.2 mol scale synthesis
Operation Reagent/Solvent Time/s
Wash Acetonitrile 30
Detritylate 3% TCA/DCM 50
Monitor trityl - -
Wash Acetonitrile 30
Flush Argon 10
Couple0.1 M phosphoramidite monomer and 0.5 M tetrazole in
acetonitrile30
Wash Acetonitrile 30
Flush Argon 10
CapAcetic anhydride/py/THF 1/1/8 and 17.6% w/v N-methyl
imidazole in acetonitrile30
Wash Acetonitrile 30
Flush Argon 10
Oxidise 0.02 M iodine in water/pyridine/THF 2/20/78 45
Wash Acetonitrile 30
Flush Argon 10
Detritylation
The resin is functionalised with protected nucleoside monomers. The
DMTr protecting group prevents polymerisation during functionalisation, but
must be removed to allow coupling to the next base (figure 11). The acid-
catalysed detritylation is achieved with a 3% TCA/DCM or 3% DCA/DCM solution.
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Figure 11 Acid-catalysed (TCA or DCA) detritylation mechanism
The trityl cation is a highly-conjugated and stable species, absorbing
strongly in the visible wavelength range. Automatic and real-time UV-Vis
absorption analysis with a radiation source (495 nm
) of the column effluent
quantifies the efficiency of the synthesis, terminating it if yields fall below a
certain threshold to preserve reagents.7
Activation & Coupling
Coupling to the next base (figure 12) requires a mild acid catalyst,
tetrazole (or derivative of), to activate the phosphorous of the incoming
nucleoside phosphoramidite group towards nucleophilic attack. The protonation
of the diisopropylamino group makes it a better leaving group and facilitates
O
O
O
O
O
BH2
O
O
NH
O
OCl
Cl
ClH
O
O
O
O
O
BH2
O
O
NH
O
OCl
Cl
Cl
H
O
O
HO
O
O
NH
BH2
O
O
O
O
etc.
DMT cation (orange)
= Resin (CPG, PS)
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5-alcohol groups to prevent further participation of erroneous oligonucleotides
in further elongation cycles (figure 13).
Figure 13 An electrophilic acylation cocktail prevents deletion-mutation oligonucleotide inclusion
in further elongation cycles
The reaction of acetic anhydride with NMI creates a strong nucleophile
and also an equivalent of acetic acid. Pyridine is therefore included in the
capping cocktail to maintain the alkaline conditions required to avoid premature
detritylation.
Oxidation
The product of the coupling reaction yields a phosphorous (III) linkage
between the bases. This phosphite triester must undergo oxidation to an acid-
stable phosphorous (V) phosphotriester before the next acidic detritylation takesplace (figure 14). Treatment with iodine in water and pyridine affords the
cyanoethyl-protected PV backbone.
O
O
HOB
O
OHN
NN
O O
O
O
NN
O
O
OB
O
OHN
O
HO
ON
NN
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Figure 15 Ester hydrolysis of succinyl linker - cleavage from solid support
Once cleaved from the solid support, the oligonucleotide/conc. aq.
ammonia solution is heated at 55C for 5 h in order to remove the phosphorous
backbone-protecting cyanoethyl groups and any exocyclic nucleobase nitrogen-
protecting groups (figure 16), however, the choice of protecting group varies
depending on the modification within the oligonucleotide e.g. those unstable to
standard conditions.8
Figure 16 Standard protection of exocyclic amines for phosphoramidite oligonucleotide synthesis
The oligonucleotide can then be purified by the method appropriate to the
oligonucleotide and application e.g. gel filtration, HPLC (reverse phase or ion
exchange-HPLC) or PAGE.
O
O
OB
O
OHNNH4
OH
O
OHN
OH
O
OH
OB+/- H
NH3
N
HN
ON
O
OH
HO
O
PhNH
N
N
O
NHN
O
OH
HO
O
N(4)-benzoyl dC (dCBz) N(2)-isobutyryl dG (dGiB)
N
NN
N
HN
O
OH
HO
Ph
O
N(1)-benzoyl dA (dABz)
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Oligonucleotides in Genetic Analysis
Watson-Crick base pairing specificity makes short
oligonucleotides ideal as reliable and sequence-specific probes of
complementary sequences. Labelling of such oligonucleotides is
required, as an oligonucleotide possesses no inherent
detectability. Labelling probes with fluorescent organic molecules
(dyes) confers many useful properties which are exploited in the
various synthetic oligonucleotide applications.1b Many different probe
technologies have been developed, a common theme being the generation of a
fluorescent signal upon hybridisation to complementary sequences.9
Figure 17 Components of a FAM dye phosphoramidite used for labelling ONTs at 5 terminus
The labelling of these probes is achieved through covalent linkage
between the oligonucleotide and the corresponding functionalised derivatives of
the labels. Fluorescent dyes, quenchers and affinity tags with pre-installed
coupling functionality (figure 17) are commercially available and their properties
are well-documented.10 Many applications, such as HyBeacon probes, require,
or can be enhanced by, the inclusion of multiple fluorescent labels.1b
O
O
O
O
ONH
O
O
O
OP
O
N
N
Reactivegroup
Spacer Signalling moiety
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HyBeacon Probes
An excellent application and measure of success of the fluorescent
labelled oligonucleotide is the HyBeacon probe. HyBeacons are linear single-
strand oligonucleotides labelled with fluorescent groups, such as fluorescein.
HyBeacons are the simplest format of oligonucleotides used in genetic analysis,
for example in probing single nucleotide polymorphisms (SNP)s and short
tandem repeats (STRs).4a The principal of the HyBeacon probe is to produce an
increase in fluorescence upon hybridisation to a complementary sequence (figure
18). This fluorescent enhancement upon hybridisation occurs due to the
reduction of distance-dependent fluorescence quenching interactions between
fluorophores and between fluorophores and nucleobases.11
Upon hybridisation,the formation of the ordered and relatively rigid helical duplex reduces the
proximity between fluorophores and quenching structures reliably increasing
fluorescence.12
Figure 18 Signal generation principle of a HyBeacon probe
Correctly-paired Watson-Crick bases contribute to a more
thermodynamically stable duplex than one containing mismatches.13 The
analytical technique exploiting this property is the melt study. The melting
temperature (TM) is the temperature at which the two complementary strands
make the transition between the separate, free strands and the hybridised
duplex. Raising the temperature of a duplex eventually provides enough thermal
energy to overcome the inter-strand attractive interactions and the duplex
denatures; upon cooling the process is reversed. Duplex formation/denaturation
is tracked by changes in fluorescence; the TM
is taken as the point of inflection
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on a fluorescence vs. temperature plot maxima of the first derivative (figure
19).
Figure 19 Melt curve and first derivative of a oligonucleotide duplex, TM= 53C, with correct
Watson-Crick base pairing
Melting experiments quantify duplex stability and can accurately
differentiate between perfect and imperfectly paired gene sequences.
Experiments using HyBeacon probes provide a quick and cheap means of
detecting SNPs, STRs and mutations through fluorescent measurement.
-50
0
50
100
150
200
250
300
350
400
450
7,000
8,000
9,000
10,000
11,000
12,000
35 37 39 41 43 45 47 49 51 53 55 57 59 61 63 65 67 69 71
-dFI/
dT
/K-1
Fluoresc
entIntensityat
525
(FI)
/
ArbitraryUnits
Temperature (T) / C
Melt Curve and First Derivative of anOligonucleotide Duplex
Raw Melt Data
First Derivative
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Labelling is most commonly achieved through phosphoramidite ligation,
a), by the inclusion of a modified monomer containing the functional moieties or
linker arms described that react with the incoming phosphoramidite label.15
Phosphoramidite labelling is advantageous in that it is high-yielding and
compatible with the automation of the DNA synthesiser.
Each type of labelling reaction has its strengths and limitations: Methods
b, c, and d) are post-synthetic techniques requiring amino or thiol-modified
monomers and corresponding electrophilic label derivatives. They offer a
strategy for introducing labels that arent stable to oligonucleotide deprotection
conditions. They may suffer from low chemoselectivity due to reactivity of the
electrophilic labels with amino groups of the oligonucleotide bases.
16
Additionally, the corresponding resultant functional group connections are
susceptible to hydrolysis, an outcome only partially avoidable via careful
handling of pH with appropriate buffer system.16 They are not the most efficient
strategies.
Enzymatic incorporation of labelled NTPs, strategy e), is limited to small
scales, but does allow for high-density multiple label incorporation.16 Due to
enzyme-substrate specificity, however the nature of the dye is limited.16 Other
conceivable labelling strategies include the Staudinger ligation and Diels-Alder
type reactions (figure 21).16
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Figure 21 Labelling by h) & i) Diels-Alder [4+2] cycloadditions and j) Staudinger ligation
Compatibility with solid-phase synthesis; retention of dsDNA helix
stability; retention of Watson-Crick pairing specificity and practical synthetic
convenience are challenges in the area of oligonucleotide labelling. Certain in
vivoapplications add the demands of bioorthogonality and toxicity to this list.17
The properties of a particular label must be considered carefully to assess
suitability. The labelling process must be compatible with oligonucleotide
chemistry i.e. easy to attach with mild reagents. Its mode of attachment mustretain the required properties of the label e.g. fluorescence. Interference with
oligonucleotide function, i.e. specific hybridisation and duplex formation, should
be minimal. Additionally, the stability of the labelled oligonucleotide should be
sufficient to withstand storage at -20C.
Multiple labelling is often desirable. Detection of complementary
sequences is often limited by the concentrations at which the targets are
present. Low concentrations yield low intensity fluorescence upon hybridisation.
LOligo NL
Oligo
h)
i)
O
O
O
N
O
O
O
LOligo NL
Oligoj)
O
N
O
O
O
LN3Oligo
OligoO
O
Ph2P
O
O
NH
Ph2P
O
L
O
L Oligo= Label with Spacer, = Oligonucleotide
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Although highly sensitive equipment exists, detection of target sequences
at biological concentrations i.e. picomolar or lower, can prove challenging.18
Enhancing the fluorescent signal of a probe through addition of multiple
fluorescent reported groups helps address this problem. Fluorescence in-situ
hybridisation (FISH) is a technique for imaging living cells and visualising the loci
genes in a chromosome. FISH typically uses 100-1000 bp probes with a labelling
frequency of 1 fluorescent label per 30 nucleotides. For greater specificity in
probe-binding, shorted sequences are desirable, but limitations come with the
low levels of fluorescence this produces. FISH probes are typically synthesised by
enzymatic incorporation of fluorescently-labelled nucleotide triphosphates in a
polymerase process such as nick translation, random priming or the polymerase
chain reaction.
9a
Enzymatic incorporation of fluorescent nucleotides, however,limits the diversity of fluorescent groups that can be attached due to enzyme-
substrate specificity.
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Previous Strategies for Multiple Labelling of Oligonucleotides
Currently, the most common strategy for multiple labelling is via the
inclusion of commercially-available phosphoramidite monomers with pre-
installed dye functionality, such as the monomer shown in figure 22. Prominent
companies offering such compounds include Glen Research8, Link Technologies19
and Invitrogen20.
Figure 22 Components of a general reporting phosphoramidite monomer, such as thosecommercially available from Glen Research8
Such dye phosphoramidite monomers are, however, often expensive and
they are limited by the requirement that the dye and conjugating functional
groups (amide bonds in the above example) must withstand the oligonucleotide
synthesis cycles.
Another current approach is through the inclusion of monomers bearing
the functional groups outlined in figure 22. Amide coupling yields, however,
rarely match those attainable by phosphoramidite coupling. A commercially
available amino modifier is shown in figure 23.
O
O
O
N
HN
O
O
O
NH
HN
O
O
O
P O
NN
Rep
Phosphoramidite nucleobase Linker Reporter group(Rep)
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Figure 23 Fmoc Amino-Modifier C6 dT, 5'-(4,4-Dimethoxytrityl)-5-[N-((9-fluorenylmethoxycarbonyl)-aminohexyl)-3-acrylimido]-2'-deoxyUridine,3'-[(2-cyanoethyl)-( N,N-diisopropyl)]-phosphoramidite, commercially available from suppliers, such as Glen Research8
Incorporation of monomers bearing orthogonal protecting groups into the
oligonucleotide is less well-documented, but offers several advantages over the
previously mentioned approached. Post-synthetic deprotection and exposure of
alcohol groups permits coupling to dye phosphoramidites that do not require the
same levels of resilience to the oligonucleotide phosphoramidite synthesis cycle.
This broadens the scope of potential dyes/labels/reporter groups and may offer
a cheaper and high-yielding multiple labelling strategy.
Previous methods, using modified, protected phosphoramidite monomers,
have achieved successful internal labelling (figure 24).21 These strategies typically
involve interruption of the DNA oligonucleotide solid-phase synthesis at the
point of modification addition. This is then allows manual deprotection of the
modification, and labelling with phosphoramidite-functionalised fluorescent
dyes, such as TAMRA or FAM, before returning to the DNA synthesiser to
complete the sequence.
O
O
O
N
HN
O
O
O
N
H
HN
O
O
O
O
P O
NN
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Figure 24 Internal labelling monomer used in previous work by Dobson et al. 2-Fmoc uridineCEP, 5-O-(4,4-Dimethoxytrityl)-2-O-[2-(9-fluorenylmethyloxycarbonyloxy)]ethyl uridine
The oligonucleotide synthesis strategy for the incorporation and labelling
of such monomers is outlined in figure 25.
O
O
O
N
NH
O
O
O
O
PO
NN
OO O
O
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Figure 25 Previous synthetic approaches to internal labelling21
The implication of this strategy is that, in order to achieve multiple
labelling, the automated DNA synthesis cycle must be interrupted at the point of
3'5'
OPG
3'5'
OH
Couple to reporter phosphoramidite
3'5'
3'5'
Cleavage & exocyclicnucleobase deprotection
3'5'
Extend
Extend
Remove, deprotect
Return to synthesiser forextension until sequence complete
PG = Protecting Group
Modified Monomer
Solid Support (PS/CPG)
Rep = Reporter Molecule
PO
O
O
O
Rep
PO
O
O
O
Rep
PO
O
O
O
Rep
5'
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Results & Discussion
Monomer Design
For most applications, the success of a particular oligomer modification is
judged primarily by two factors: signal sensitivity upon hybridisation and
retention of normal hybridisation behaviour. A consequence of the highly
sophisticated and precise nature of the DNA double helix is that random
modifications to its components are more likely to interfere with, rather than
improve duplex stability and Watson-Crick complementarity.
Modification at 2-position does not directly interfere with the
phosphoramidite synthesis method, but steric bulk may reduce coupling
efficiencies.22 Distancing of bulky groups from the 3-CEP group with alkyl
spacers is expected to reduce steric inhibition of the coupling reaction.
Modification at the C-5 position of pyrimidines is a common target since it
is not involved base-pair hydrogen bonding. The modification is projected into
the major groove of the helix, allowing for significant steric tolerance and
minimal inhibition of helix formation (figure 33).
Figure 33 Modification at pyrimidine C-5 projects into major groove
N
NN
NN
NN
O
O
HH
H NN
N
N O
N
NN
N
O
H
HH
H
H
Major
Groove
Minor
Groove
Major
Groove
Minor
Groove
= Modification
A T G C
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The protecting groups chosen must be orthogonal to the conditions used
to remove the DMTr group (acid labile). The fluorenylmethoxycarbonyl (Fmoc)
moiety was used as an alcohol-protecting group, introduced by nucleophilic acyl
substitution and removed by -elimination (figure 34). -elimination is easily
achieved with mild bases, such as morpholine, piperidine, piperazine, for
example, due to the electron-withdrawing fluorene ring system. Decarboxylation
also provides a strong thermodynamic driving force.
Figure 34 Fmoc cleavage by (1,2)-elimination with piperidine
The 2-deoxyuridine version of monomer 1 has been used previously by
Dobson et al. in the successful synthesis of a dual-labelled probe using Fmoc
chemistry.15 This monomer is now synthesised via an improved syntheticstrategy. Use of this monomer to construct a multiply-labelled oligonucleotide
RO O
OH
RO O
O
14 e , 4n+ 2, n= 3Planar Aromatic System
HN
NHH
NH
RO
O
O
NHH
R OH
- CO2
N
- eliminationE1cb
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was attempted, but afforded disappointing yields indicating the need for
optimisation of the synthesis protocol.
The second generation of protecting groups were levulinyl and TBDMS.
The levulinyl protecting group was introduced vianucleophilic acyl substitution
from the corresponding acid anhydride. Hydrazinolytic cleavage was achieved
with hydrazine monohydrate in pyridine/acetic acid (figure 35).
Figure 35 Post-synthetic removal of levulinyl protecting group by hydrazinolysis
The tert-butyldimethylsilyl (TBDMS) protecting group was introduced by
nucleophilic substitution (SN1) and removed with fluoride chemistry, usingTEA.HF as fluoride source (figure 36).
Figure 36 TBDMS removal viahypervalent silyl intermediate
TBDMS and levulinyl (Lev) protecting groups were selected as suitable
protecting groups due to their proven orthogonality with DNA oligonucleotide
synthesis, as demonstrated in a previous use in the construction of cross-linked
DNA.23
O
O
O
H2N NH2
+/- HOH
O
OHN
H2N
OSi
F
Si OFSi
F
HO
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Synthetic Approach
5-O-(4,4-Dimethoxytrityl)-2-O-(2-(9-fluorenylmethyloxycarbonyl)ethyl)-5-
methyluridine-3-O-(O-2-cyanoethyl-N,N-diisopropyl) phosphoramidite (Monomer 1)
Precursor 9 was synthesised in accordance with the method described by
Richardson et al, 2009. The first transformation in this sequence, (i), was
achieved with 79% yield. This compares well with the reported literature figure of
90% when the relative scales of synthesis are considered.9e
NH
O
ON
O
OHOH
HO
N
O
O N
O
OH
HO(i)
N
O
O N
O
OH
O(ii)
NH
O
ON
O
OOH
O (iv)
NH
O
ON
O
OOH
O (v)
NH
O
ON
O
OO
O
DMTr
DMTr
OHO
FmocCEP O
Fmoc
DMTr DMTr
(iii)
1109
7 8
Scheme 1 Synthetic route to Fmoc-protected monomer 1 (i) Diphenyl carbonate (1.1 eq.), NaHCO3
(cat), DMF, 100C, 18 h, 79%; (ii) DMT-Cl (1.4 eq.), py, rt, 24 h, 67%; (iii) Ti(i
PrOH)4 (1.4 eq.), ethyleneglycol (5.0 eq.), DMF, rt, 22 h, 62%; (iv) Fmoc-Cl (1.1 eq.), DIPEA (2.0 eq.), DCM, rt, 2.5 h, 40%; (v)CEP-Cl (1.2 eq.), DIPEA (2.0 eq.), DCM, rt, 3 h, 71%.
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The second transformation, the protection of the 5-alcohol with the trityl
group viaa nucleophilic substitution (SN1) reaction with dimethoxytrityl chloride
is both mechanistically and practically simple. Regioselectivity for the 5-alcohol
in preference to the 3-alcohol was accomplished on grounds of steric hindrance.
The DMTr-Cl is a bulky tertiary alkyl halide that does not react readily with the
secondary alcohols at either 2- or 3-positions. The substitution reaction
proceeds with the concomitant loss of hydrogen chloride from the reagents
necessitating the presence of at least one equivalent of a suitable base due to
the acid-ability of the resulting DMTr protecting group. The reactivity of the
tertiary DMTr carbocation with to the hydroxide ion calls for careful exclusion of
water. The necessarily basic conditions of this reaction mean that the presence
of water would lead to rapid undesired consumption of DMTr-Cl throughformation of DMTr-OH.
The reaction was achieved in 67% yield, lower than that reported in the
literature value- 89%.9e The smaller scale predisposed the reaction to a lower
yield, but other factors also contributed. The reaction proved to be stubborn and
additional aliquots of DMTr-Cl, time and patience were required. Eventually (t =
22 h), the reaction was determined incomplete, but was quenched, worked-up
and purified regardless. Upon repetition of this reaction, more rigorous
exclusion of water would be observed.
A notable feature of syntheses whose reagents or products include the
DMTr protecting group is the distinctive orange colour that indicates presence of
the DMTr cation in solution (figure 38). This can alert the chemist to the
presence of moisture in solvents, for example. Due to the strong molar
extinction coefficient of the DMTr cation however, it is rare that reaction
mixtures remain completely colourless as very low levels of the cation confer
colouration. Also, heat-induced detritylation of compounds offers a rapid and
informative TLC plate visualisation technique.
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Figure 38 UV Absorption spectra of DMT cation in acetonitrile24
Opening of the anhydro ring (figure 39) was achieved in a 62% yield,
slightly lower than the literature value of 79%.9e A possible cause for disparities
in apparent yield success may be due to the contamination of the product
reported in the literature with titanium complex remains accounting for higherapparent yield. Thorough, repeated centrifugation of the reaction mixture
ensured that a highly pure product was obtained, but inevitably at the loss of
some compound to the retentate, although this was washed several times and
checked viaTLC until satisfactorily clean.
Figure 39 Nucleophilic alkoxide ring opening mechanism
Absorption, /nm
400 450 500 550 600
0.0
0.5
1.0
1.5
498 70 000 dm3 cm-1 mol-1
410 28 960 dm3 cm-1 mol-1
Absorbance(unitless)/ArbitraryUnits
Ti(OiPr)4HO
OH
N
O
O N
O
OH
ODMTr
Ti(OCH2CH2O)O
O
H
HN
O
O N
O
OH
ODMTr
TiL3
O
O
+/- H
+/- L
HN
O
O N
O
OH
ODMTr
O
OH
2 Ti(OCH2CH2O)2
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The major source of loss was due to compound-impurity overlap during
column chromatographic purification that necessitated the exclusion of impure
fractions from the pure fraction pool. Total recovery of compound with a second
column could be achieved if it were needed for subsequent syntheses, or if a
valuable amount of reagents had been committed and warranted isolation. A
competitive reaction that may have reduced yield involves the isopropoxide
acting as the ring-opening nucleophile. However, due to greater steric bulk of
the isopropoxide and using an excess of ethylene glycol, this pathway does not
appear to interfere significantly.
Fluorenylmethyloxycarbonyl was chosen to protect the remaining primary
alcohol group as it offers orthogonal compatibility with the conditions of thephosphoramidite method (see experimental, the phosphoramidite method).
Nucleophilic substitution of chloride at the chlorocarbonate group of Fmoc-Cl by
the primary alcohol yields the product with the concomitant overall loss of
hydrogen chloride from the reagents. The basic conditions employed in the
reaction protect the DMT-protected alcohol group from acid-induced exposure
and deprotonation of the alcohol assists in its nucleophilic attack at the Fmoc
carbonyl carbon atom.
The reaction was initially attempted using pyridine functioning as both
solvent and base. Bis-addition of Fmoc resulted, as determined by LRMS.
Experimentation with reaction conditions led to the use of DIPEA as base and
DCM as solvent, addition of Fmoc-Cl as solution and at 0C. This had three
advantages. Firstly, the reaction proceeded more reliably and required fewer, if
any, extra additions of Fmoc-Cl. Secondly, addition of Fmoc-Cl as a solution is
practically cleaner than exposing the reaction to the external environment and
allows for more control over addition rate. Thirdly, DCM can be removed quicker
and more completely than pyridine, which was often detectable by NMR in early
experiments. The combination of lower reaction temperatures and very gradual
addition of Fmoc-Cl solution successfully afforded the desired product, 40%.
Further optimisation would benefit this reaction.
The phosphitylation was performed with great care and afforded the
phosphoramidite monomer 1 in 71% yield. High product purity was required, asno further purification would take place before the compound entered the
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Figure 40 The Palladium & Copper mediated catalytic cycles of the Sonogashira reaction26
The product was only obtained in 49% yield. Possible side products
include the alkyne-alkyne homocoupled dimer and the furano-pyrimidine
nucleoside (figure 41).
ThePalladiumCycle
TheCopperCycle
OxidativeAddition
trans-cisIsomerisation
Reductive
Elimination
RR' R' X
Transmetallation
RCu
Cu X
RH
Cu X
R3N
R3NH X
PdII
L
L
R' X
PdIIR'
L
L
R
RCu
PdII
R'
L
L R
PdL2
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Figure 41 Proposed furano-pyrimidine side-product formation mechanism
Fmoc protection was successful, achieving a yield of 82%. Originally, this
was attempted using the less-reactive reagent - Fmoc-OSu to achieve the
required primary alcohol selectivity, but the reaction did not proceed so gradual
addition and low temperature, 0C, was employed.27
Phosphitylation to yield monomer 2 was moderately successful as
reflected in the yield of 60%. Improvements in yield could be made through
obtaining better separation of crude components. The product eluted over 18fractions indicating that a lower-polarity eluent system would not be suitable to
achieve better separation of components. Instead a larger volume, wider
diameter column could be tried in order to achieve separation with a slightly
more polar system.
N
O
O N
O
OH
O
OH
DMTr
Et3N H
Cu
N
O
O N
O
OH
O
OH
DMTrEt3N
Cu
H
N
O
O N
O
OH
ODMTr
OH
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The mechanisms of hydrazinolysis and the Staudinger reduction are both
particularly interesting and are shown in figures 42 and 43, respectively.
Figure 42 Mechanism of primary amine deprotection by hydrazinolytic phthalimide cleavage
The phthalimide-protected amine can be installed via an SN2 reaction
between the corresponding primary alkyl halide and potassium phthalimide.29
The combined subsequent phthalimide deprotection constitutes the Gabriel
synthesis.29 This precursor was synthesised in-house by Dr. Montserrat
Shelbourne, following the approach described by Manoharan et al.30
NH
O
ON
O
OOH
ODMTr
N
NH
O
ON
O
OOH
ODMTr
NH2
O
ONH2
NH2NH
O
ON
O
OOH
ODMTr
NH
O
O
HNH2N
+/- H
+/- H
14
O
HN
HN
O
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Figure 43 Primary amine formation mechanism by Staudinger reduction, affording primary amine,
14 upon aqueous work-up
Nucleophilic attack by triphenylphosphine at the terminal azide nitrogen
followed by ring closure forms a phosphazide. Irreversible loss of nitrogen forms
the iminophosphorane. Hydrolysis occurs upon aqueous work-up and isthermodynamically driven by the formation of the strong phosphorous-oxygen
double bond.
To extend the length of the linker at the 2-amino ethoxy dT, an amide
coupling between the NHS-ester and the amine was used to give compound 15 in
78% yield. The activated acid offers good reactivity; the reaction proceeded
rapidly without need for carbodiimide coupling agents. Amide coupling is a
frequently-employed connection approach throughout the syntheses of these
monomers. A general mechanism is given in figure 44.
NH
O
ON
O
OOH
ODMTr
NH214
NH
O
ON
O
OOH
ODMTr
N
N
N PPh3
NNN
PPh3
N
NN
PPh3
N PPh3 N PPh3-N2
H2O
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Figure 44 General mechanism of amide bond formation
NHS-activated acids offer enhanced reactivity, permitting the use of milder
conditions, by providing a more stable leaving group than the hydroxide anion.
They are of intermediate reactivity - between that of carboxylic acids and acid
chlorides. They are easy to handle yet their enhanced reactivity is still significant
enough to offer a real synthetic advantage. Occasionally the amide couplingdoes not proceed satisfactorily and carbodiimides can be used to drive the
reaction. The mechanism of this process is illustrated in figure 45.
Figure 45 Carbodiimide-promoted amide bond formation
Undesired side-reactions can occur from the O-acylisourea and include a
rearrangement for form a stable N-acylurea and a reaction with an additional
carboxylic acid molecule to form an acid anhydride of the carboxylic acid (figure
46).
R1 NH2
HO
O
R2 +/- H
- H2O
NH
O
R2
R1
NC
NG G
NH
CN
G G
O
O
RH
O
O
R
G NH
N
O
G
O R NH2R'
+/- H
R'NH
O
R NH
O
NH
GG
O-acylisourea
G =
cyclohexyl (DCC)
isopropyl (DIC)ethyl (EDC)
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Figure 46 O-acylisourea rearrangement forming stable N-acylurea
The acid anhydride can go on to react with the amine to form the desired
amide and release a carboxylic acid (figure 47).
Figure 47 Reaction of carboxylic acid with O-acylisourea to form dicyclohexylurea and acid
anhydride - further reacting to give desired amide and an equivalent of corresponding carboxylic
acid
Phosphitylation was successful and without complication. Column
purification however, was problematic. Elution was protracted and caused
overlap with excess phosphitylating reagent. The pure fractions yielded only
29%.
G
HN N
O
G
O
R N-acylurea
NH
O
N
O
R
G
G
G =cyclohexyl (DCC)isopropyl (DIC)ethyl (EDC)
O
O
R
G NH
N
O
G
O R+/- H
R'NH
O
R
N
H
O
N
H
GG
* Acid anhydrideof carboxylic acid
R
O
O
O
R
H2N R'
*
R
O
OH G =cyclohexyl (DCC)isopropyl (DIC)ethyl (EDC)
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A common problem is the inclusion of unreacted phosphitylating reagent.
When elution of this reagent, or if PV species overlap with that of the monomer,
the contaminated fraction(s) cannot be combined. Their presence can be
visualised on TLC plates stained with p-anisaldehyde and are observed as a white
spot. This is easily distinguishable from the monomer that stains black with p-
anisaldehyde. If this separation proved particularly difficult for a particular
compound then the reaction could be performed with phosphitylating reagent in
limiting proportions.
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5-O-(4,4-Dimethoxytrityl)-5-(3-(6-( tert-butyldimethylsilyloxy)-hexanamido)-propynyl)-
2-deoxyuridine-3-O-(O-2-cyanoethyl-N,N-diisopropyl) phosphoramidite (Monomer 4)
The TBDMS group was installed viaunimolecular nucleophilic substitution
(SN1) of its chloride derivative. The acid was activated to the NHS ester to
promote amide coupling. The NHS group is a better leaving group than the
hydroxide anion and coupling can be achieved with milder conditions.
Amide coupling via the NHS-activated acid proceeded without
complication. The clean reaction facilitated simple column chromatography and
afforded compound 16 in 63% yield. Phosphitylation was achieved in 70% yield.
HN
O
O N
O
O
O
NH
4CEP
O
O
TBDMS5
DMTr
HN
O
O N
O
OH
O
N
H
O
O
TBDMS5
DMTr
OH
O
HO
HN
O
O N
O
OH
O
NH2
DMTr
OH
O
OTBDMS
O
O
OTBDMS
N
O
O
(i)
(ii)
(iii)
(iv)
16
Scheme 4) Synthetic route to TBDMS-protected monomer 4 (i) TBDMS-Cl (1.2 eq.), DIPEA (2.0 eq.),DCM, rt; (ii) NHS (1.3 eq.), EDC-Cl (1.2 eq.), DIPEA (3.0 eq.) DMF, rt; (iii) DIPEA, (1.5 eq.), DCM, DMF, rt,4 h 63% iv CEP-Cl 1.2 e . DIPEA 2.0 e . DCM rt 2.5 h 70%.
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5-O-(4,4-Dimethoxytrityl)-5-(3-(6-(levulinyloxy)-hexanamido)-propynyl)-2-
deoxyuridine-3-O-(O-2-cyanoethyl-N,N-diisopropyl) phosphoramidite (Monomer 5)
Compound 17 was produced by a carbodiimide-assisted amide formation
reaction. Synthesis of compound 18 was achieved in 70% yield through reaction
between the alcohol and the acid anhydride, which was prepared in-situ. This
terminal alkyne product was subsequently coupled to the 5-iodouridine by a
Sonogashira cross-coupling reaction in 59% yield.
HN
O
O N
O
O
O
NH
5CEP
O
O
Lev5
DMTr
HNO
O N
O
OH
O
NH
O
O
Lev5
DMTr
OH
O
HO
NH
O
HO
(i)
HN
O
O N
O
OH
ODMTr
I
NH
O
OLev
(iv)
(iii)
17 18
19
O
O
OH
O
O
O
O
O
(ii)
(v)
Scheme 5 Synthetic route to levulinyl-protected monomer 5 (i) Propargylamine (1.5 eq.), EDC-Cl(1.5 eq.), DMF, rt, 18 h, 67%; (ii) DCC, Et2O, rt; (iii) Levulinic anhydride (prepared in-situ) (1.4 eq.),DMAP (0.5 eq.), DCM, DMF, rt, 1.5 h, 70%; (iv) CopperI Iodide (0.25 eq.), Pd0(PPh3)4 (0.1 eq.), DMF, TEA,rt, 1.5 h, 59%; (v) CEP-Cl (1.2 eq.), DIPEA (2.0 eq.), DCM, rt, 3.5 h, 74%.
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5-O-(4,4-Dimethoxytrityl)-5-(3-(6-(9-fluorenylmethyloxycarbonyl)-hexanamido)-
propynyl)-2-deoxyuridine-3-O-(O-2-cyanoethyl-N,N-diisopropyl) phosphoramidite
(Monomer 6)
Scheme 6 (i) TMS-Cl (1.2 eq), DIPEA (2.0 eq.), DCM, rt, 3 h, 64%; (ii) Fmoc-Cl (1.2 eq.), DIPEA (2.0
eq.), DCM, rt; (iii) EDC-Cl (1.3 eq.), DIPEA (3.0 eq.), DCM, rt, 2 h, 56%; (iv) Py.HF (1.1 eq.), py, DCM,
unsuccessful; (v) Not yet attempted
Inclusion of a TMS protection step improved a previous approach.
Previously the Fmoc-protected acid was reacted with compound 20 without the
3-O-TMS protecting group and resulted in bis Fmoc coupling. Deprotection of
the TMS group, however, resulted immediate cleavage of the DMTr group. An
attempt to recover the compound was made since the DMTr group could be
selectively reinstalled at the 5-position, however the recouped yield was
insufficient to warrant further efforts.
Approaching monomer 6 via the 5-O-(4,4-Dimethoxytrityl)-5-(3-(6-
(hydroxy)-hexanamido)-propynyl)-2-deoxy uridine, treated with Fmoc-O-
succinimide did not proceed even with addition of 4-dimethylaminopyridine, acoupling catalyst (figure 48).
HN
O
O N
O
O
O
NH
CEP
O
O
Fmoc5
DMTr
HN
O
O N
O
OH
O
NH
O
O
Fmoc5
DMTr
HN
O
O N
O
O
O
NH
O
O
Fmoc5
DMTr
TMS
HN
O
O N
O
O
O
NH2
DMTr
HN
O
O N
O
OH
O
NH2
DMTr
(i)
(iv) (v)
TMS
O
OHHO
O
OHO
Fmoc
(ii)
(iii)
20 21
22 6
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Figure 48 Mechanism of catalytic action of DMAP in an amide coupling reaction
The reaction mixture was worked-up and dried in vacuoand the reaction
attempted at -42C (MeCN, CO2(s)) with the more reactive Fmoc reagent Fmoc
chloride. The reaction produced four DMTr-containing products as identified by
TLC, but which degraded to starting material before purification was achieved. It
is suspected that the presence of pyridine or remaining DIPEA from the reaction
mixture, which was added to maintain basicity during the HCl-producingreaction, was responsible for the premature Fmoc cleavage. In conclusion,
handing of compounds bearing the Fmoc moiety must be treated carefully with
respect to over-exposure to basic conditions.
N
N
OO
O
N
O
O
N
N
O
O
N
N
O
O
O
OO
O
N N
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Oligonucleotide Synthesis Strategy
Modified monomers 1-5 were introduced into a HyBeacon probe by three
different approaches. Following deprotection of the modifications, the exposed
groups were labelled with 6-FAM phosphoramidite. The probe sequence was
programmed to differentiate between wild-type and mutant gene for an SNP
implicated in statin-induced myopathy, rs4149056.31
Approach A
In the first approach (figure 49), the modified monomer is incorporated
into the sequence at the desired positions as follows. The sequence is
synthesised until after the coupling of the modified monomer. Keeping the
terminal 5- DMTr group on, the synthesis is paused and the oligonucleotide
column is treated with an appropriate cocktail to remove protecting group (Lev,
Fmoc or TBDMS) of the hydroxyl. The column returned to the synthesiser and the
synthesis cycle resumed at the point of coupling to the next nucleoside in the
sequence. The label phosphoramidite is coupled to the modified monomer and
then the sequence continued until, at the next modification, the process isrepeated until the sequence is complete.
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Figure 49 Labelled-oligonucleotide synthesis approach A
3'5'
OPG
Remove, deprotect
3'5'
OH
Couple to 6-FAM-phosphoramidite
3'5'
Return to synthesiser for
extension until next modification
3'5'
Cleavage & exocyclic nucleobase deprotection
3'5'
Extend
Extend
Return to synthesiser forextension until sequence complete
3'5'
PG = Protecting Group
Modified Monomer
Solid Support (PS/CPG)
Extend
Rep = Reporter Molecule, FAM
PO O
O
ORep
PG
O
PO OO
ORep
PO O
O
O
Rep
PO O
O
O
Rep
PO O
O
ORep
PO O
O
ORep
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This approach was tested with monomer 1 with the following sequence, where
superscript XF represents FAM labelling:
5-GTGGATA1FATGCG1FTCATGG
The crude HPLC-MS and the MS are shown in figure 50. The major peak
corresponds to the correct oligonucleotide product and indicates a yield of
around 80%. This approach afforded a high-purity probe (figure 50), but the
complexity of the procedure may deter many from its use.
The labelled oligonucleotide product was isolated and tested as a
HyBeacon probe in a melting analysis.
Figure 50 Left:HPLC trace for monomer 1, sequence: GTGGATA1FATGCG1FTCATGG (1F = monomer1, labelled with FAM) synthesised with Approach A, correct ONT product (2 FAM additions), T
r: 8.6
min; Right: MS showing the correct expected product calc. MS = 7535.97 Da, found MS =7536.41Da)
Approach B
Approach B (figure 51) offers a less-complicated labelling protocol for the
installation of multiple labels. The entire oligonucleotide is synthesised with the
protected, modified bases in their desired location within the sequence, the
terminal 5-DMTr is left on. The oligonucleotide column is removed from the
synthesiser, treated with DEA (as above), the modification protecting groups
removed and the column returned to the synthesiser at the point of next
coupling. Finally, the phosphoramidite label is applied and the synthesis is
complete, ready for standard deprotection and cleavage.
4 5 6 7 8 9 10 11 Time [min]
0
50
100
150
Intens.
[mAU]
res3210_GB5_01_14311.d: UV Chromatogram, 290nm
4511.6 4949.05314.1
5650.0
6317.2
6767.4
7206.4
7536.4
9028.2
-MS, 8.5-8.7min, Deconvoluted (MaxEnt)
0
1
2
3
4x10
Intens.
4000 5000 6000 7000 8000 9000 10000 11000 m/z
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Figure 51 Labelled-oligonucleotide synthesis approach B
Several oligonucleotides were synthesised following this approach in order
to optimise the conditions. For monomers 1 and 2, the results were
unsatisfactory (figures 52 & 53) 0-15% product was found. Attempts at
optimisation were made, changing capping conditions from acetic anhydride to
Tac2O (milder capping reagent) and no capping. Further optimisation attempts
5'
Remove, deprotect
Cleavage & exocyclic nucleobase deprotection
3'5'
Synthesise entire ONT
PG = Protecting Group
Modified Monomer
Solid Support (PS/CPG)
Rep = Reporter Molecule, FAM
3'5'
OPGOPG
Couple to 6-FAM-phosphoramidite
3'
OHOH
5' 3'
O
5'
5'
P
OO
O
Rep
O
P
OO
O
Rep
O
POO
O
Rep
O
POO
O
Rep
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included doubling the coupling times (10 to 20 mins), concentration of the
applied phosphoramidite monomer (0.1 to 0.2 M) and using fast-deprotecting
nucleosides (dGDMF, dCAc). An example HPLC trace is shown in figure 52, full
details are given in HPLC section of the appendix.
Figure 52 Left: HPLC trace for res3261, sequence: GTGGATA2FATGCG2FTCATGG3 (2F = monomer 2,labelled with FAM, 3 = propanol), synthesised with Approach B, peak at T
R= 7.4 min: no FAM, 8.1
min: only 1 FAM; Right: Mass spec of peak at TR
= 8.1 min
Figure 53 HPLC UV 290 nm
chromatrogram for res3263, sequence GTGGATA1FATGCG1FTCATGG3 (1F= monomer 1, labelled with FAM, 3 = propanol), peak at T
R= 7.4 min no FAM, 8.1 min: only 1 FAM
addition and TR
= 8.6 min: expected product with 2 FAM label. Right: MS of peak at TR= 8.6 min.
Monomer 4 was incorporated into the following sequence (res3373):
5-GTGGATA4FATGCG4FTCATGG
Deprotection of monomer 3 was attempted with TEA (20% in MeCN, 45
min) then TEA.3HF (2 x (0.3 mL, 30 min)). The mass spectrometry results did not
produce any clear peaks (figure 54). Purification was attempted with RP-HPLC,but no separation was achieved. This could be due to the TEA.3HF, a strong
0 2 4 6 8 10 12 14 16 Time [min]
0
50
100
150
200
Intens.
[mAU]
Res3261c_RC1_01_14667.d:UV Chromatogram,290 nm
6325.26421.2
6629.2
6958.3
-MS,7.9-8.1min,Deconvoluted(MaxEnt)
0
1
2
3
4
4x10
Intens.
5500 5750 6000 6250 6500 6750 7000 7250 7500 7750 8000 m/z
0 2 4 6 8 10 12 14 16 Time [min]
0
50
100
150
200
Intens.
[mAU]
Res3263c_RC3_01_14669.d: UV Chromatogram, 290 nm
5394.06011.1
7535.4
9007.6 9420.4 10528.8 13192.5
-MS, 8.6-8.7min, Deconvoluted(MaxEnt)
0.00
0.25
0.50
0.75
1.00
1.25
4x10
Intens.
5000 6000 7000 8000 9000 10000 11000 12000 13000 14000 m/z
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base, prematurely deprotecting the exocyclic nucleobase amine groups causing
FAM to add to free amines of the nucleobases, resulting in numerous products
and preventing successful purification. Optimisation is required.
Figure 54 HPLC UV 290 nm
chromatogram for res3373, using polystyrene support (TBDMSdeprotection incompatible with CPG, fluoride ion reacts with the Si-O structure of the CPG)
Monomer 5 was incorporated into the following sequence:
GTGGATA5F
ATGCG5F
TCATGG
Table 3 Experimentation with ONT synthesis
ONT ID Conditions Chromatogram
res3371
CPG resin
Treated with 20% DEA/MeCN, 25 min to deprotect
the acetal capping of the CPG hydroxyl groups
A
res3390
CPG resin
No treatment with DEA (control experiment) Bres3391 PS resin C
All oligonucleotides in table 3 were treated with DEA (10% DEA/MeCN, 10
min) to deprotect the phosphate backbone prior to levulinyl deprotection.
Levulinyl deprotection conditions were hydrazine monohydrate:acetic
acid:pyridine, 0.031:0.5:2.0 v/v/v, rt, 12 min.
0 2 4 6 8 10 12 14 16 Time [min]
0
50
100
150
Intens.
[mAU]
RES3373_RC4_01_16570.d: UV Chromatogram, 290 nm
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A
B
C
Figure 55 HPLC UV 290 nm
chromatograms, A) res3371, B) res3390 & C) res 3391 sequence:GTGGATA5FATGCG5FTCATGG (5F = monomer 5, labelled with FAM), peak at T
R= 7.5 min:
unlabelled; TR= 8.2 min: 1 FAM addition; T
R= 8.9 min: 2 FAM additions (correct product); MS traces
are shown in appendix (HPLC and Deconvoluted MS)
Treatment with DEA prior to synthesis produces a higher amount of
product than when untreated (figure 55). It is suspected that coupling to FAM
phosphoramidite was reduced by migrating acetyl groups from the CPG-hydroxy
protection. These were removed with the DEA and were therefore not present to
complicate capping.
0 2 4 6 8 10 12 14 16 Time [min]
0
10
20
30
40
Intens.
[mAU]
RES3371_RC5_01_16571.d: UV Chromatogram, 290 nm
0 2 4 6 8 10 12 14 16 Time [min]
0
20
40
60
Intens.
[mAU]
RES3390_RC6_01_16572.d: UV Chromatogram, 290 nm
0 2 4 6 8 10 12 14 16 Time [min]
0
10
20
30
Intens.[mAU]
RES3391_RC7_01_16573.d: UV Chromatogram, 290 nm
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Approach C
A further improvement in terms of practical simplicity was developed in
approach C (figure 56). Interruption of the synthesis at the point of labelling was
avoided. The terminal DMTr group at the end of synthesis was removed (DMTrOFF) and the 5-alcohol capped with hex-5-ynyl phosphoramidite (X). This
means that no human intervention is required during the synthesis and a
standard phosphoramidite cycle program can be used without further
manipulation.
Figure 56 Labelled-oligonucleotide synthesis approach C
5'
Remove, deprotect
Cleavage & exocyclic nucleobase deprotection
3'5'
Synthesise entire ONT (DMTr OFF), cap with hex-5-ynyl phosphoramidite ('X')
PG = Protecting Group
Modified Monomer
Solid Support (PS/CPG)
Rep = Reporter Molecule, FAM
3'5'
OPGOPG
Couple to 6-FAM-phosphoramidite
3'
OHOH
5' 3'
O
5'
5'
P
OO
O
Rep
O
P
OO
O
Rep
OP
OO
O
Rep
OP
OO
O
Rep
X
X
X
X
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This strategy was used to synthesis the following oligonucleotide
(res3415) with monomer 5 on a PS solid support:
5-XGTGGATA5FATGCG5FTCATGG
Figure 57 Left: HPLC UV 290 nm
chromatogram for res3255, sequence: GTGGATA5FATGCG5FTCATGG(5F = monomer 5, labelled with FAM), peak at T
R= 8.6 min: [M-134], unknown, peak at T
R= 8.8 min:
2 FAM additions (correct product); Right: MS
This approach yielded the correct product (figure 57) in a high-yield and
was accomplished with a practically-uncomplicated protocol. This represents a
successful new strategy for adding multiple reported groups to oligonucleotides.
The dual-labelled oligonucleotide was tested as a HyBeacon probe.
HyBeacon Studies
A melting study provided a direct comparison between a conventionally-
labelled HyBeacon and one synthesised by the new strategy (figure 58). A
HyBeacon was synthesised using fluorescein dT, purchased from Glen
Research. The HyBeacon probes were identical apart from the mode of
fluorescein attachment, permitting an assessment of the effect of the phosphate
linker on fluorescence and duplex stability.
0 2 4 6 8 10 12 14 16 Time [min]
0
200
400
600
800
1000
Intens.
[mAU]
RES3415CR1_RB3_01_17066.d:UV Chromatogram,290nm
7206.2
7743.3
-MS,8.7-9.0min,Deconvoluted (MaxEnt)
0.0
0.5
1.0
1.5
5x10
Intens.
5000 5500 6000 6500 7000 7500 8000 8500 m/z
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Figure 58 Structural comparison of FAM dT monomers: A commercially-available, = F in res1137
and B - as produced by the reported strategy (5F,used in res3391)
The probe sequence was programmed as the complement for an SNP at
rs4149056, implicated in Statin-induced myopathy, forming a G:C base pair in
the matched sequences (WT) and G:A in the mismatched. The melting
temperatures of the probe-target duplexes were investigated. The results are
displayed in table 3.
Table 4 Melting temperature results of HyBeacon(TM) probe comparison study
Oligo.ID SequenceDuplex T / C TM / CWild Type Mutant
Probe 1res1137 GTGGATATAFGCGFTCATGG 43.0 53.0 10.0
Probe 2res3210 GTGGATATA5GCG1TCATGG 42.0 52.0 10.0
Probe 3res3391 GTGGATATA5GCG5TCATGG 45.0 54.0 9.0
WTTarget
res3375 CCATGAACACATATATCCAC --
MTTarget
res3376 CCATGAACGCATATATCCAC --
O
O
O
N
HN
O
O
O
NH
HN
O
O
O
HO
O
OH
O
O
O
N
HN
O
O
NH
O
OPO
O O
NH
O
O
O
HO
O
OH
A
B
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Conclusion & Future Work
Conclusion
This project set out to investigate a new strategy for adding multiple
reporter groups to oligonucleotides through incorporation of protected modified
monomers. Five monomers were synthesised and incorporated into
oligonucleotides. The most successful were tested as HyBeacon probes. The
probes successfully differentiated between the two alleles of a gene implicated in
statin-induced myopathy. The properties of the probe-target duplexes with
probes synthesised by the reported strategy and a probe synthesised using a
FAM-dT-phosphoramidite, purchased from Glen Research8, were compared. The
probes were found to have high similarity, indicating that the structural
differences in the base-label connection do not significantly interfere with either
duplex stability or fluorescent emission. This was a successful demonstration of
the strategy. It is clear that an effective multiple labelling strategy has been
developed.
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Future Work
Variant Labelling
Theoretically, through the use of two or more modified monomers in
which the label-linking functional groups (-OH or NH2) are mutually orthogonal
in their protection, multiple and variant labels could be easily installed (figure
61).
Figure 61 Capacity for multiple and variant labelling
5'
Remove, deprotect PGA
Cleavage & exocyclic nucleobase deprotection
3'5'
O(Rep)AO(Rep)A O(Rep)B O(Rep)B
3'
PG = Protecting Group
Modified Monomer
Solid Support (PS/CPG)
Rep = Reporter Molecule
3'5'
OPGAOPGB OPGBOPGA
Couple to reporter phosphoramidite A
3'
OHOPGB OPGBOH
5'
O(Rep)AO(Rep)A O(Rep)B O(Rep)B
5'3'
O(Rep)AOPGB OPGBO(Rep)A
Deprotect PGB
5' 3'
O(Rep)AOH OHO(Rep)A
Couple to reporter phosphoramidite B
Synthesise Entire ONT
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Variant label installation could prove useful in applications that desire
dendrimeric structures, asymmetric branching, or installation of multi-coloured
probes for wider instrument detection compatibility.
Branching Oligonucleotides
Installing multiple reporter groups could enhance HyBeacon probe
resolution. Ultra-high fluorescence outputs could be achieved through the use of
branching side chains containing multiple fluorescent groups (figure 62).
Similarly, fluorescence in-situ hybridisation (FISH) target detection capability
could be improved through higher fluorophore installation levels.
Figure 62 A) Orthogonally protected phosphoramidite monomer, B) Reporter groups or branchextensions C) Branched oligonucleotide
DNA and RNA sequences can be detected by surface-enhanced Raman
spectroscopy (SERS).32 The probe sequence is usually connected through a
thioether at the 3-terminus to a gold nanoparticle and labelled with a Raman-
active dye. The anchored strand has many degrees of freedom and the proximity
of the Raman dye to the gold surface, required for Raman enhancement, cannot
HN
O
O N
O
O
O
CEP
DMTr
O
OPG2
OPG1HN
O
O N
O
O
O
DNA
DNA
O
O
O
Rep1 or ONTs
Rep2 or ONTs
Rep1 or ONTs
Rep2 or ONTs
Rep3 or ONTs
Rep4 or ONTs
Rep5 or ONTs
Rep6 or ONTs
A) B)
C)
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be guaranteed. Branching oligonucleotides could provide multiple anchor points,
maintaining dye-surface proximity and optimum Raman signal enhancement.
Cell Imaging
For imaging sequences in living cells, the probe must enter the cell. This
can be achieved manually by microinjection or with by addition of a delivery
vehicle, such as lipofectamine, but both techniques can damage the cell and alter
its normal functioning. Natural cellular uptake mechanisms can be encouraged to
accept molecules bearing polyamines (figure 63), which exist in their protonated
cationic form at physiological pH.
33
A route for simple ligation of the sperminegroup and fluorescent groups to oligonucleotides may be of use in cell imaging
research.
Figure 63 Spermine phosphoramidite, commercially available from Glen Research
Combinatorial Labelling
The reported strategy for adding multiple reporter groups to
oligonucleotides is particularly well suited to large-scale synthesis. This is due to
the simple labelling protocol and single purification step. It is time and cost-
efficient, essential for viability of commercial applications.
N N N NO
TFA TFA
TFA TFA
O P O
NN
O
O
TFA = trifluoroacetyl protecting group F
FF
O
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Simultaneous, detection of many specific pathogens, bacterial, viral,
fungal, parasitic, could be achieved with a cocktail of FISH probes, each with
specific pathogen targets. The synthesis of the probe cocktail could be easily
accomplished with a combinatorial process. Complete probe sequences can be
combined on their solid supports then deprotected and labelled in one batch.
The probe cocktail could be tailored to its application. A hand-wash gel,
loaded with the correct probe sequences could simultaneously detect the
predominant bacterial pathogens responsible for hospital infections or provide a
rapid detection system for biological warfare agents for use in high-risk facilities.
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Experimental
General Methods
General
Standard reagents were procured from Aldrich, Avocado or Fluka. Solvents
were distilled as follows: DCM, TEA, DIPEA, py from CaH2
and THF from sodium
with benzophenone as indication of anaerobic, anhydrous quality. Reaction