the use of 19f nmr to monitor organic reactions on solid ... · other questions are now beginning...
TRANSCRIPT
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Lehigh UniversityLehigh Preserve
Theses and Dissertations
2004
The Use of 19F NMR to Monitor OrganicReactions on Solid SupportsPaul KrolikowskiLehigh University
Follow this and additional works at: http://preserve.lehigh.edu/etd
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Recommended CitationKrolikowski, Paul, "The Use of 19F NMR to Monitor Organic Reactions on Solid Supports" (2004). Theses and Dissertations. Paper841.
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Krolikowski, Paul
The Use of 19FNMR to MonitorOrganic Reactionson Solid Supports
May 2004
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The Use of 19p NMR to Monitor Organic Reactions on Solid
Supports
by
Paul Krolikowski
A Thesis
Presented to the Graduate and Research Committee
of Lehigh University
in Candidacy for the Degree
of Master of Science
in
Chcmistry
Lehigh Uni\'crsity
April. 2004
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Acknowledgments
I gratefully acknowledge the support of Dr. N. Vasant Kumar and Dr. Ed Orton who
were kind enough to advise me on all aspects of this thesis. I especially appreciate their
patience during the writing of this document and their understanding of the
uncontrollable nature of mergers in the pharmaceutical industry (at least that is the
excuse I have been using to justify my own procrastination).
I also want to thank my wife Rhonda. She has never wavered in her support of me, even
when things seemed to grind to a complete halt. The rest of my family and friends also
served an important role in not forgetting to ask me when I was going to finish my
degree.
And last, but certainly not least, thank you Dr. Roberts. You have shown me great
understanding concerning my personal situation and an cqual amount of paticnce.
Without your help, this document would nevcr have been finished.
Special Thanks to: John Airey, Thomas Molnar, Andrew and Shelley Allcn, Julian
Levcll, Darren Engers, Nicole Lawson, Rose Mathew, Sharnlila Patcl, David
Krolikowski. S. Y. Tang. Stevc Pitzenberger. Thomas Kaliskcr and Raju Subramanian.
111
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Table of Contents
CHAPTER
List of Tables, Figures and SchemesAbstract1. Introduction2. Analytical methods for Solid-Phase Synthesis
2.1 Elemental Analysis, Gravimetric Analysis and Acid!Base Titrations
2.2 UV and Fluorescence Methods2.3 FT-IR and FT Raman Methods2.4 Mass Spectrometry2.5 Nuclear Magnetic Resonance Spectroscopy
3. Methods and Materials4. Results and Discussion
4.1 TFP Resin4.2 Fluorinated Chloromethlypolystyrene (FCP Resin)
5. Conclusions6. ReferencesBiography
IY
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Scheme 1Figure 1Table 1Figure 2Table 2Table 3Table 4Figure 3Figure 4Figure 5Figure 6Figure 7Figure 8Scheme 2Figure 9Figure 10Figure 11Figure 12Figure 13Figure 14Scheme 3Scheme 4Figure 15Figure 16Figure 17
List of Figures, Tables and Schemes
TFP Resin Preparation19F NMR ofTFP Resin PreparationComparing NMR Probes and Sample TechniquesTFP Resin Loading with Internal SIDTFP Resin Loading Study (Raw Data)TFP Resin Loading Study (mM Fluorine/ g resin)TFP Resin Loading Study (Average Results)Process 1 Calc 1 vs. Elemental AnalysisProcess 2 Calc 1 vs. Elemental AnalysisProcess 3 Calc 1 vs. Elemental AnalysisProcess 1 Calc 2 vs. Elemental AnalysisProcess 2 Calc 2 vs. Elemental AnalysisProcess 3 Calc 3 vs. Elemental AnalysisActivated Ester and Final Product FormationIH NMR, nanoprobe on INOVA 50019F NMR, nanoprobe on INOVA 50019F NMR, 5mm probe on VXR 300Kinetics of Ester Formation on TFP ResinI H NMR of amide products from Acid 2Acid 2-TFP resin after diethylamine product formationFCP Resin ProductionSolid-phase Michael Addition ReactionsMichael Addition Reaction Yields19F NMR Data of Michael AdditionIR Data of Michael Addition
PAGE
28293134363738394041424344484950525355575959616364
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Abstract
The use of Combinatorial chemistry and high throughput screening have revolutionized
the process of discovery and development of therapeutic agents in the pharmaceutical
industry. Typically, large numbers of compounds are synthesized in a combinatorial
manner either on a solid support or in solution phase. These are screened against a
variety of biological targets related to different disease states. Structural
characterization of these molecules and knowledge of chemistry on the solid supports
are of great importance in optimizing the synthesis of chemical libraries. Nuclear
Magnetic Resonance (NMR) spectroscopy may be utilized to investigate these
properties, however the use of solid-phase supports presents a new set of analytical
challenges. These challenges include limited sample availability, complex mixtures,
line-broadening problems which affect resolution, limited spectral dispersion and the
need for high throughput sample analysis.
We have developed 19F NMR methods for investigating resin-bound chemistry. These
techniques are sensitive and require a relatively small amount (1-3 mg) of sample. The
spectra have large chemical shift dispersion and no interfering fluorine signals due to
the resin itself. Application of magic-angle spinning in a Nano . nmr TIl probe further
reduces the line width and the amount of sample required for analysis. We illustrate the
usefulness of this technique to study solid-phase organic synthesis using the
tetrafluorophenol (TFP) resin which is synthesized by attaching 2.3.5.6
tetrafluorohydroxybenzoic acid to aminomcthyl resin. The phcnolic group is uscd to
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form esters and sulfonates. A pair of fluorine resonances is observed from the TFP
moiety of the resin in the -100 to -180 ppm region and is useful for monitoring the resin
bound chemistry. We have developed an internal standard method, using 3
Flourobenzamide, to determine the loading of TFP on the aminomethyl resin.
There has also been an effort to investigate the use of an internal Fluorine standard by
the co-polymerization of 4-fluorostyrene into the backbone of the resin bead. By using
this signal as an internal standard, certain solid phase chemical reactions were
optimized.
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The Use of 19p NMR to Monitor Organic Reactions on Solid
Supports
by
Paul Krolikowski
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1. Introduction
The method of solid-supported synthesis has been in existance for close to forty years.
The method was originally introduced by R. B. Merrifield in 1963 [1]. In this effort,
Merrifield was able to demonstrate covalent bound amino acids to
polystyrene/divinylbenzene resin beads. From this point additional amino acids could
be combined in a linear fashion through repetitive cycles of deprotection, coupling, and
washing steps. The final step was the cleavage of the desired peptide from the resin by
breaking the original covalent bond used to attach the first amino acid [2]. Attachment
to a solid surface allowed the chemist to avoid the time consuming isolation and
purification steps usually needed in traditional solution-phase synthesis. After the
coupling reaction to the solid support was completed, the chemist could simply wash the
resin to remove impurities and unreacted starting materials. Early efforts in solid-phase
synthesis were concentrated in producing peptides and oligonucleotides. By 1973,
efforts were being made to adapt traditional solution-phase chemistries to solid-phase
methods [2]. Solid-phase synthesis, also know as combinatorial chemistry, is now one
of the primary methods used to produce large varieties of highly pure samples of small
molecules. A large number of scientists in different industries are using combinatorial
and parallel synthesis to explore huge numbers of molecules in the hopes of finding one
that displays a particular list of desired properties. Scientists in the pharmaceutical
industry are readily utilizing these techniques in the hope of probing as many molecules
as possible against a specific disease target. Excellent reviews arc now available which
effectiYcly summarizc the cycr-growing field of solid-phasc synthesis [2.3. and 4].
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One of the biggest challenges in the field of solid-phase synthesis has been finding
suitable analytical methods to monitor solid-phase reactions. Most of the traditional
analytical methods used to monitor organic synthesis were optimized for unattached
small molecules, which could be readily dissolved in a variety of solvents and
subsequently separated from complex mixtures and analyzed. Attaching small
molecules to resins presents a variety ~f new challenges to the analytical chemist For
example, how does a chemist actually determine if a reaction has gone to completion on
a resin bead without cleaving the product from the resin after each step in a synthesis?
If a combinatorial chemist can determine that a reaction has actually gone to
completion, the next logical question might be one of determining kinetics. These and
other questions are now beginning to be answered by adapting existing analytical
techniques to compensate for the presence of the solid-phase support [5,6, 7]. Two
specific applications using 19F NMR to monitor solid-phase synthesis will be
summarized in the remainder of this document. The first application includes the use of
TFP resin to optimize amide library synthesis on solid supports. The second application
is the use of a fluorine containing monomer in the polymerization of a specific resin.
This resin contains an intemal 19F standard which was used to optimize certain solid
phase chemistries.
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2. Analytical Methods for Solid-Phase Synthesis
2.1 Elemental Analysis, Gravimetric Analysis and AcidlBase Titrations
Combustion elemental analysis has been used to quantitatively monitor solid-phase
synthesis. These results were highly consistent with those obtained from well-
established methods such as Fmoc monitoring [8]. In one particular study conducted at
Novartis, quantitative elemental analysis results were obtained for eight resin-bound
compounds. In addition to a six-step peptide synthesis, a dansylhydrazone synthesis
was quantitatively monitored using elemental analysis. Several elements including
carbon, hydrogen, nitrogen, chlorine, sulfur and bromine were analyzed during this
study. The amount of sample required for analysis ranged from 2 to 35 mg for each
measurement. Special emphasis was placed on washing and drying samples since resin-
trapped reagents or solvent molecules would cause variable results. Quantitative results
for resin loading in each synthetic step are observed in this study [8]. However, a
considerable amount of resin was destroyed to obtain the experimental results. These
losses might be acceptable for the discovery phase of library development, but not for
library production. Modem production methods are using smaller amounts of resin [2].
Bing Yan and his colleagues from Novartis also studied resin loading using gravametric
analysis [9]. The results from these studies wcrc often misleading. The wcight gain in
each ste~p svnthcsis was too small to be detected relativc to the dominatc resin weight.\ \.J ~
H i I (j d k . . . '1 d . Ilnany so vcnts, rcagents, an cven un 'nown tmpunttes werc east y trappe Into t lC
resin beads. causing unpredictable weight variations [9]. Acidlbase titrations have also
been used to quantitate resin loading. Howcver. it was suspected that negative charges
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would accumulate in the polymer matrix and could inhibit titration of the remaining
acid groups. Therefore, the accuracy of this method is still under question.
2.2 UV and Fluorescence Methods
The UV spectrophotometric quantitative measurement of Fmoc release from derivatized
amino groups is still a very common method for measuring resin loading [6]. One
method involves determining the absolute amount of aldehyde and non-hindered ketone
groups on a resin. Roughly a two-fold excess of dansylhydrazine was mixed with DMF
swollen aldehyde/ketone resin and a plain polystyrene (control) for 30-50 minutes. The
amount of aldehyde/ketone groups was calculated from the reduced fluorescence peak
areas or UV absorbance. The amount of noncovalent dansylhydrazine trapped in the
resin was corrected for by subtracting the amount of dansylhydrazine consumed on an
identical amount of plain polystyrene resin [9]. A similar method involves the reactions
between 9-anthroylnitrile or I-pyrenyldiazomethane (PDAM) and resin bound hydroxyl
or carbonyl groups. The quantitation was attained by analyzing 2-10 mg of resin in 30
60 minutes. The lowest amount of hydroxyl groups studied was 0.05 mmol/g of resin.
The 9-anthroylnitrile method was free from interference from most other organic
functional groups and the PDAM method was highly selective for carboxylic acid
groups [10]. For both of these methods, single-bead FT-IR was used to determine when
the reactions with the specific reagents had gone to completion. The authors suggest
that from a synthetic chemist's point of vic\\'. the UV-visible method is very
advantageous because the operation is simpler. the spectral reading is more stable. and
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the instrument is widely available [10]. Efforts have also been made to determine single
bead fluorescence microspectroscopy for the detection of self-quenching in
fluorescence-labeled resin beads [11].
2.3 FT-IR and FT Raman Methods.
Fourier Transform infrared spectroscopy (FTIR) is a very useful technique to confirm
the presence of a desired functional transformation in a solid phase reaction. In 1971,
KBr disks of ground beads were used to obtain spectra in the normal transmittance-type
mode [5, 7]. Diffuse reflectance infrared FT (DRIFT) technique enables the collection
of spectra without the need of producing KBr pellets and produced better data in the
'OH' spectral region. Photoacoustic (PA) FTIR has also been utilized to study solid
phase reactions. The spectra from the PA-FTIR method were found to be free of
baseline artifacts caused by light scattering and sample inhomogeneity [7].
Single-bead FTIR is probably the most widely used IR technique to monitor solid-phase
reactions by IR [5, 7, 12]. This method involves the use of an IR microscope to locate
and focus the IR radiation on a single bead. The beads are slightly flattened to decrease
the sample pathlcngth to 10-15 11m, reducing spectral distortion and interference [5, 7,
and 12]. A second method uses Attenuated Total Reflection (ATR). The ATR
objective is in physical contact with a single bead, which flattens the bead as well. An
lR spectrum is obtaincd of the matcrial on the surface of the bead (typically to a dcpth of
a fcw micrometcrs) [5]. This technique is vcry scnsitive. with a limit of detcction in the
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femtomole region. Bing Yan and his colleagues from Novartis Phannaceutical
Corporation have used this technique to monitor the kinetics of esterification of
hydroxyl groups on Tentagel and Wang resins [7]. Several other examples of kinetics
and reaction monitoring have been presented by this group using a combination of IR,
Fluorescence and FT Raman methods [9, 10, 11, 12, 13]. One particular study involves
the comparison of eight FTIR and FT Raman techniques applied to 10 resin-bound
compounds. An extensive review of each compound is given along with results and
suggestions for the most appropriate choice of FTIR or FT Raman technique [12].
Infrared spectroscopic techniques are certainly useful for direct functional group
analysis and can permit qualitative and quantitative analysis of each reaction step
throughout a synthesis. However, spectral overlap for similar functional groups in
complex molecules can limit the usefulness of infrared spectroscopy for qualitative and
quantitative analysis. This problem could be circumvented by substituting a reactant
with its deuterium-labeled counterpart. This greatly improved the functional group
selectivity of infrared analysis by allowing the carbon-deuterium (C-D) stretching to be
observed in a primarily interference-free spectral region from 2300 to 2200 cm- I (14).
One drawback of this method is the production of a mixture of labeled and unlabeled
final products.
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2.4 Mass Spectrometry.
Mass Spectrometry is the most widely used analytical technique for investigating
libraries of compounds generated by combinatorial methods [15]. There are two broad
approaches in using MS for investigating solid-phase synthesis. The first method is to
liberate the molecule from the solid support and use HPLC or flow injection methods
for delivering and ionizing the sample for MS investigation ('cleave and analyze
method'). This is especially true with the advent of ionization methods for coupling
HPLC and MS instruments. These ionization methods often include electrospray
ionization (ESI) or atmospheric pressure chemical ionization (APCI) [15]. Once the
sample is ionized, MS can be used to investigate many issues regarding combinatorial
solid-phase synthesis. The second general method involves direct bead-bound analysis
[15] (discussed on page 13).
Mass spectrometry has been used to encode and decode library synthesis [16]. One
method incorporates the use of an acid-labile linker to release a series of molecular tags
that could be rapidly assessed by LC-MS [16]. Another method of encoding includes
the use of incorporating isotopically labeled tags (DC and 2H) onto the beads containing
the desired compound [17]. However, these coding methods have limitations. Each
coding method is actually an indirect-coding method and identifies the anticipated
product on the bead but does not confirm its presence or purity. The code can also
interfere or produce false positives/negatives in a bioassay [17].
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Flow Injection Analysis (FIA) mass spectometry is often used by many groups to
confirm the identity of anticipated products. High throughput and ease of automation
are observed using FIA-MS [18]. Parallel FIA-MS methods are employed to
dramatically increase throughput. T. Wang and coworkers used an array of injector
valves to introduce samples simultaneously. The valves were sequentially rotated from
load to inject to produce a fast, serial sampling of the library. The samples in a
microtiter plate were analyzed in about 12 minutes [18].
To improve library quality, HPLC-MS has become the preferred method [19]. In
comparison to flow injection, LC adds information concerning purity and quantity of the
compound being analyzed. Fast HPLCIMS methods have been developed which use
'universal-like' HPLC gradients and short columns (usually 4.6 mm i.d. x 30 mm in
length) operating at higher flow rates (3-5 mUmin). These conditions give run times
between 3 and 5 minutes including re-equilibration of the column [19]. These methods
have also been extended to include Parallel HPLCIMS systems configured with at least
two sets of HPLC pumps to supply equal flow to an array of HPLC columns [17].
These columns are supplied by a multiple probe autosampler, a muliplex UV detector,
and an ion source interface to independently sample simultaneously sprayed samples.
Research has also included the use of Supercritical Fluid Chromatography in
combination with Mass Spectrometry (SFC/MS) [20, 21]. A supercritical fluid and a
modifier. such as methanol, enable separations during this method. Under these
conditions. separations occur at linear speeds that are 3 to 5 times faster than LC~lS
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[20,21]. Of course there is the added benefit of mobile phase disposal when a large
component of the effluent is an inert gas under atmospheric conditions. A supercritical
fluid such as carbon dioxide could simply be released into the atmosphere after the
separation has been completed.
Other detection methods have also been used to find a more universal response.
Ultraviolet and mass spectrometry detection methods can have limited response if a
compound lacks a chromophore or resists ionization. Chemiluminescence Nitrogen
Detection (CLND) and Evaporative Light Scattering Detection (ELSD) are being
utilized with UV and MS to investigate library purity [22, 23]. The ELSD detector in
particular appears to offer a more 'universal response' than the other methods. In an
effort to improve MS response, negative and positive ion scan modes are often used on
the same sample. The selection of buffers and modifies must be carefully made
depending on which scan mode is being used [15].
Automated systems are now in place to purify combinatorial libraries before the
compounds are sent for biological testing [15, 24]. Ultraviolet or MS results trigger the
fraction collection after an HPLC injection in these automated systems. The
combination of UV and MS has a certain advantage in that it allows the fraction
collection to be triggered by a desired mass rather than just a predetem1ined UV
threshold. This greatly reduces the number of fractions collected and helps identify the
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desired compound for purification and further testing [15,24]. This methodology has
also been extended to preparative LC systems [25,26].
Mass Spectrometry has also been utilized for drug screening purposes. One method
involves the use of Size-Exclusion Chromatography and Mass Spectrometry (SEC-MS)
[27]. The soluble target receptor is incubated with a compound library and then
exposed to a SEC column. The unbound library components pass through the column
first and can be collected for future assessment. The protein bound ligands are then
collected and liberated from the receptor or protein and identified by mass spectrometry
[27]. A screening method has also been demonstrated by using affinity chromatography
and mass spectrometry [28]. Direct observations of gas phase protein-ligand
complexation correlated to binding affinity was observed using ESI-MS [29].
The second general method using mass spectrometry involves direct bead-bound
analysis. The unique ionization requirements of resin-bound molecules limit methods to
Matrix-Assisted Laser Desorption (MALDI) [15,30]. This ionization method involves
the crystallization of the sample with an organic acid to form a crystal matrix. The
matrix is then exposed to UV-laser radiation. The absorbed energy causes a proton
transfer which vaporizes and ionizes both the matrix and analyte [15, 30]. In order for
MALDI to be used directly on resin-bound molecules, a photolabile linker must be
utilized. The wavelength required to cleave the compound from the resin must also be
consistent with the wavelength of the i\IALDI laser [31]. The cleavage step can also be
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preformed just prior to matrix production using an acid labile linker and trifluoroacetic
acid [32, 33].
2.5 Nuclear Magnetic Resonance Spectroscopy.
Although Nuclear Magnetic Resonance (NMR) is not as fast or sensitive as mass
spectroscopy or HIR, it can supply more detailed information about the structure of a
molecule and does not require the sample be cleaved from the resin before analysis.
Unlike mass spectroscopy and elemental analysis, NMR is nondestructive and after
analysis the sample can be returned for further chemistry [34]. As in the case of mass
spectroscopy, NMR analysis can fall into two broad categories including solution-phase,
tubeless NMR and on-bead or gel-phase NMR.
Although the major consideration in combinatorial synthesis has been on solid phase
analysis, the use of traditional solution phase organic synthesis to produce compound
collections should not be overlooked. Mass spectroscopy is certainly the method of
choice when a combinatorial chemist wants to analyze a mixture of compounds in a
solution phase library. Potential problems can arise when isomolecular weight
compounds are present. These compounds can be stereoisomers, positional isomers or
identical molecular weight compounds. In these cases and others, compound
identification by mass spectroscopy can be difficult [34-].
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The development of HPLC-NMR allows for the separation of components in mixtures
and subsequent identification by NMR. A popular technique is the use of stop-flow
methodologies. In this method, the HPLC effluent leaves the column and passes
through an initial detector (UV or MS) which is used to detect a desired component in
the mixture. Special timing experiments are conducted to determine the amount of time
needed for a peak to move from the initial detector to fill the flow-cell in the NMR
probe at a particular flow rate. At this point, the HPLC pumps are turned off and the
desired, isolated component is 'parked' in the flow probe. Because the diameter of the
tubing is relatively small compared to the flow-cell, the sample remains in the flow cell
with only small and often unperceived diffusion effects. The sample can remain in the
flow-cell for long periods of time allowing for several 2-D acquisitions. Although not
as many examples exist for the analysis of combinatorial libraries [35,36], HPLC-NMR
has been very successful in the analysis of mixtures of drug metabolites [37 thru 40]. In
most of these studies, very small amounts, 10-50 /lg, of each metabolite is present in the
active volume of the NMR flow-cell and can require hundreds of scans for ID proton
data. A series of capillary loops can be used to collect fractions of a particular HPLC
run. These individual fractions are then pumped into the NMR probe for stop-flow
analysis [36]. The HPLC-NMR technique can also be useful for investigating unstable
metabolites. Certain metabolites can not survive the final solvent elimination
procedures during isolation. Stop-flow NMR effectively avoids these problems [37].
Because of often severely limited sample amounts. the use of cryogenically cooled
N~IR probes becomes especially attractive [38]. In the case of metabolite
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investigations, completely deuterated mobile phase is often used to avoid solvent
suppression issues, which can destroy useful regions of the spectrum. By coupling LC
NMR with MS it is possible to use the MS data to trigger the stop-flow for subsequent
NMR experiments [41].
In on-flow HPLC-NMR, the HPLC effluent flows continuously through the probe.
NMR spectra are obtained at predetermined time intervals. The resulting 1D data sets
can be viewed in a 2D-like display, with the chemical shift dimension along the X-axis
and retention times along the Y-axis. Modem solvent suppression techniques, such as
WET (Water suppression Enhanced through T1 effects) [42], allow for the use of non
deuterated solvent systems. Using a combination of shaped RF pulses, pulsed-field
gradients, and selective I3C decoupling, the WET technique allows for the suppression
of multiple frequencies with controllable bandwidths. The WET suppression technique
can also compensate for the use of solvent gradients during an HLPC run. In the case of
acetonitrilefD20 mobile phase gradient runs, the process uses a small-tip-angle single
pulse "scout" to locate the acetonitrile peak. The transmitter is reset to that frequency,
the next largest peak (HOD) is located and a soft-shape pulse is calculated which will
excite both the acetonitrile and water resonances. By interleaving scout scans and the
time-averaged scans, the solvent positions are fully and :mtomatically tracked during thc
coursc of the solvcnt gradient [42]. Flow-NMR requires larger amounts of sample than
stop-flow because of the limited time the samplc spcnds in the receivcr coil. Onc
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benefit of a protonated mobile phase system is the elimination of deuterium exchange,
which can complicate MS data acquisition for LC-MS-NMR systems.
In an effort to increase sample throughput, flow-NMR techniques are replacing more
traditional glass NMR tube techniques [43]. A combinatorial chemist could take every
member of a combinatorial library, place them in NMR tubes, and use traditional robot
automation techniques to run all the samples. These libraries can have hundreds of
members, the cost of NMR tubes alone would be staggering. Direct-Injection NMR
(DI-NMR) has been developed to combine flow-NMR technologies with 96-well
microtiter plate sample handling techniques which are often used for synthesis and
screening of combinatorial libraries [43]. A Gilson Model 215 Liquids Handler was
used to inject each individual sample on a 96-well plate into the NMR flow-cell. In LC
NMR, the sample is not removed from the NMR flow-cell by pushing new effluent into
the cell. In the case of DI-NMR, the sample is pulled back out of the bottom of the
flow-cell. Nitrogen gas acts as a push-gas and is applied from the top of the flow-cell.
The flow-cell is rinsed one time with the same solvent that was used to dissolve the
original sample. After the rinse procedure, a new sample is pushed into the probe.
Because the flow-cell is empty before the next sample arrives, there is no sensitivity loss
due to dilution for the new incoming sample. Data acquisition is accomplished in a
stop-flow mode. Once the acquisition is complete. the liquid handler pulls the sample
from the flow-probe and returns it in an unaltered state to its original position in the 96
well plate. Gradient shimming and WET solycnt suppression can be standard protocols
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during the automated run. The total recycle-time for each sample, including sample
injection, shimming, acquisition (32 scans), sample recovery, probe rinsing (one cycle),
and automated plotting was 5.5 min per sample [43]. The NMR data could be collected
on every member of a 96-well plate in about 8.8 hours. One disadvantage of DI-NMR
compared to LC-NMR is the possibility that the tubing in the system could become
clogged with particulate matter if unfiltered samples are injected.
Pulsed-Field Gradient diffusion-ordered NMR (DOSY) is potentially an important
technique for the analysis of complex mixtures [44]. This method allows NMR signals
of discrete compounds to be resolved because of differences in translational molecular
diffusion as well as chemical shift. The NMR data are displayed in a 2D-like format
with a diffusion dimension and a chemical shift dimension. It is possible to resolve
mixture components whose diffusion coefficients differ by only a few percent [45]. If
components in a mixture have chemical shift overlaps, the diffusion coefficient
dimension will not be able to separate these signals. This chemical shift overlap will
produce a single peak at an averaged diffusion coefficient [44]. This can certainly
become a problem with combinatorial chemistry synthesis. Libraries generated by these
methods are often structurally related. A number of experiments, which reduce the
chance of signal overlap in the chemical shift dimension, have been developed.
Experiments such as DOSY-NOESY and DOSY-TOCSY (DECODES) have been used
in this manner [44]. The advantage of the DECODES experiment is that all I H
resonances in a spin-system are correlated allowing oycrlapped resonances to be
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correlated to resonances that are resolved [46]. The 2D-J resolved-DOSY experiment
has also been utilized to resolve diffusion coefficients in mixtures [47]. Three-
dimensional experiments including DOSY-HMQC have also been described [48]. This
experiment combines a normal 2D frequency-frequency correlated spectrum with a
diffusion-coefficient dimension. The HMQC data also resolve signals based on their
13C chemical shifts. A total experiment time of 17 hours was needed to collect one
DOSY-HMQC experiment.
The use of NMR as a screening tool has also been investigated. The SAR by NMR
method is a process by which NMR is used to identify ligands that have receptor
binding affinity [49]. This method involves the acquisition of a series of HSQC spectra
of a 15N labeled receptor protein in the presence and absence of selected ligands. The
degree of binding is determined by the degree of perturbation observed for the 15N and
I H chemical shifts of the receptor [49]. During this particular study, two ligands with
micromolar affinities for FK506 binding protein were tethered together to discover
compounds with nanomolar affinities for the same protein. It is important to have an
accurate map of the 15N and I H assignments of the receptor. An advantage of this
method is the use of 15N_HSQC spectra to detect the binding of small, weakly bound
ligands to an 15N-Iabeled target protein. Because of thc 15N spectral cditing, no signal
for the ligand is obscrvcd. Thercfore. binding can bc detected cven at high compound
concentrations. High compound concentrations generatc large background signals for
fluorometric or colorimetric assays making weakl\' bound ligands morc difficult to- ..... .' .....
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recognize. Medicinal chemistry programs with a larger array of potential lead
compounds can use the SAR by NMR technique. Limitations of this method include
the requirement for a receptor of appropriate size for NMR studies (less than 30 kDa),
appropriate solubility, and availability of 15N labeled receptor [49].
Pulsed-Field Gradient diffusion NMR can also be utilized for compound screening. In
this method (called affinity NMR), it was shown that the diffusion coefficient of a small
molecule binding with a receptor in solution is considerably different than the small
molecule alone observed under the same PFG conditions [50 thm 52]. One advantage
for the affinity NMR method is that a complete assignment of the receptor is not
necessary. Disadvantages of this method include the presence of receptor signals
obscuring ligand signals and chemical exchange between "bound" and "free" states of
weakly bound ligands can result in significant signal distortion. These drawbacks can
be minimized with the use of isotope-filtering [53] and the use of a bipolar longitudinal
eddy current delay sequence, respectively. The bipolar longitudinal eddy current delay
sequence eliminates the exchange effects and preserves diffusion infonnation without
intensity distortion [54].
The second general category (first mentioned at the beginning of the NMR section on
page 14) of N~lR used to investigate combinatorial synthesis samples is the study of
compounds directly attached to the resin or solid support. Within this second category
are two more specific ones. The first is often referred to as gel-phase NMR.
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In gel-phase NMR, resin samples are placed in a traditional 5 or 10 mm NMR tube and
swelled with an appropriate solvent [44]. 'Traditional' 5 and 10 mm NMR probes are
then used to analyze the swelled samples. A considerable amount of work has been
done to determine which solvents will effectively swell a particular resin [55]. Care
must be taken to select the correct solvent to obtain optimal swelling. The better the
swell rate the more the covalently attached molecule will mimic a solution state
environment. The swelling rate can have a direct impact on NMR signal line widths.
Even with careful solvent selection, there is extensive line broadening observed for IH
NMR data, often making the spectrum unusable for structural analysis. The
heterogeneous gel-phase samples lead to differences in magnetic susceptibility resulting
in signal line-broadening [66]. Because of these general line-broadening effects, NMR
studies are often conducted on heteronuclei such as 13C, 19p, 31 p, and 15N, which have
larger chemical shift dispersions. Pluorine-19, 31 p, and 15N have the added benefit of no
competing signals from the resin backbone [44].
Carbon-13 NMR has been used extensively to monitor solid-phase organic synthesis
[44]. It has been used to monitor functional group interconversion of polymer-bound
cholic acids [56]. The analysis of these reactions could be determined without cleavage
from the resin support. The reaction of enantiomerically pure epoxy-3-penylpropanol
anchored on Merrifield resin was monitored by DC gel-phase NMR [57]. These DC
acquisitions often require several thousands of scans to provide sufficient signal-to-
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noise ratios. To avoid these lengthy acquisition times, selected l3C labeling has been
used to monitor reactions on solid supports [58].
Fluorine-19 gel-phase NMR has been used to monitor solid-phase reactions and has
beneficial characteristics which make it useful for NMR studies [44,59]. These
characteristics include a large chemical shift dispersion, high sensitivity and no
competition from the resin backbone signals [44, 59]. In fact, the sensitivity is quite
similar to l H and only a few dozen scans are needed to obtain useful spectral
information. Structural changes in a molecule that are five to six bonds away will often
result in changes in the chemical shift of the fluorine resonances [59]. Using linkers
which contain 19F as part of their structure has also proved to be a useful method to
track synthesis on solid supports [60,61]. Due to its sensitivity and dispersion, 19F
NMR has also been used to encode combinatorial libraries to determine the final
structures of solid-phase products based on combinations of 19F signals [62].
Phosphorus-31 NMR, although not a sensitive as 19F NMR, is still useful for monitoring
chemical reactions on solid support. Phosphorus-31 NMR signals can be obtained in
about 10 min with 50 mg ofresin [63]. Phosphorus-31 NMR was used to evaluate
solid-phase oligonucleotide synthesis [63]. The oxidation of phosphite to phosphate
was monitored by the change in chemical shift from 137 to 5 ppm. The Homer
Wadsworth-Emmons alkene S)llthesis was also monitored [64-]. This starting material
has a resin bound phosphonate at 22 ppm. This signal disappears and is replaced with a
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diethyl phosphate at 0 ppm. With the use of labeled material, 15N NMR can also be
used to probe reactions in solid-phase synthesis [65].
Magic-Angle Spinning (MAS) represents the final NMR method for investigating solid
phase organic synthesis. Significant line-broadening exists in gel-phase samples due to
residual dipolar interactions and variations in bulk magnetic susceptibility [66].
Broadening due to magnetic susceptibility and dipole-dipole couplin,g both depend on
the angle between the dipole pair and the static magnetic field. This angle dependence
is represented by 3cos28-1. Spinning the sample at 54.7° with respect to the magnetic
field removes these line-broadening effects [44]. Spinning the sample also averages the
bulk magnetic susceptibility, reducing line broadening [66]. By spinning samples at
relatively high rates at the magic angle, significantly improved IH NMR spectra are
possible. The NMR probe manufactures have taken advantage of MAS and the use of
'magnetic-susceptibility-matched' materials in their recent probe designs [66]. In
particular, Varian Inc. introduced the Nano· nmr Th1 probe. The Nano· nmr Th1 probe
was the first probe designed to place the entire sample within the active region of the
receiver coil [66,67]. The sample tubes for the Nano· nmr n1 probe have a total
volume of about 40 Jll. This smaller sample volume results in the use of 3-5 mg of
swelled resin compared to 20-50 mg for a conventional 5mm probe. In addition to
MAS, other techniques have been used to impro\'c spectral quality. Presaturation of
resin backbone signals has been shown to greatly reducc their impact in a typical I H
spectra [68]. It was also found that by using thc non-tilted projection from a 2D
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i-resolved experiment, high quality NMR data could be obtained with measurable
coupling-constants [69]. A large variety of 2D MAS NMR experiments have also been
demonstrated on gel-phase samples including TOCSY, HMQC and NOESY [70,71].
The development of gradient equipped MAS probes allow for gradients to be used for
selecting the coherence pathway and removing spectral artifacts [72].
In summary, there are a variety of techniques available to study solid-phase organic
reactions. Nuclear magnetic resonance is a very useful nondestructive technique to
evaluate resin bound compounds. The utilization of MAS 19p NMR to investigate
specific solid-phase organic syntheses will be summarized in the remainder of this paper
[73,74].
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3. Methods and Materials
Unless otherwise specified, all 19F NMR spectra were obtained using a Varian INOVA
500 spectrometer operating at a 19F frequency of 470.2 MHz. A Nano . nmr TM probe
was tuned to this 19F frequency. Unless the Nano· nmr TM probe was not used, all
spectra were obtained at ambient room temperature. Varian uses the spinning or
rotation gas as the cooling gas for this particular probe. If the gas supply for sample
rotation is suddenly turned off, this could damage the thermocouple in the probe.
Therefore temperature regulation was not used. The spectral width was typically set to
100,000 Hz and 32K points (l6K real and 16K imaginary points) were collected. A ten
second delay was used between each pulse as well as 30% of the 90° pulse width
(pw90) for observing the 19F while using the Nano· nmr ™ probe. A small amount of
CFCh was added to the bulk NMR solvents as an internal standard and referenced to 0
ppm. The Nano· nmr ™ probe is oriented at the magic angle of 54.7° with respect to
the Bofield and the samples are spun at a rate of 1000-1500 Hz. For experiments using
the Nano· nmr Thl probe, 16 scans were often sufficient. There was approximately 2-5
mg of resin in each nanotube. All deuterated NMR solvents (D, 99.5% or better) were
obtaincd from Cambridge Isotope Labs. Most of the Nano· nmr Thl probe spectra were
obtaincd by swelling the resin in DMF-d6. It is an easier to handle DMF when making
up samples in the nanotubc compared to some solvents. It is also a useful solvcnt
considcring that many of the solid-phase reactions are done in DMF.
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Fluorine-19 Spectra of resins were also acquired in more traditional 5 mm NMR probes.
In these cases the typical sample amount can range from 10 to 40 mg of resin,
depending on how efficiently that solvent swelled in the chosen NMR solvent. The
solvent of choice for these experiments is CDCh. Most of the resins swell reasonably
well in CDCh and it is much less expensive compared to DMF. The relatively high
density of CDCh is also a benefit for 5mm tube studies. After the dry resins are placed
into a 5mm NMR tube, a small amount of CDCh is added just to swell the resin. When
the resin has swelled, excess CDCl3 can be added to float the resin plug into a region of
the tube to adequately fill the receiver-coil in the probe. This allows much less resin to
be used rather than filling the entire 500 to 700 ~L volume with swelled resin. Similar
spectrometer conditions (spectral width of 100,000 Hz, 30% of pw90, 30K total points)
were used for the 5mm probe experiments except in the case of experiments run on
lower field strength instruments. In these cases, a larger number of scans (256) were
required to achieve acceptable signal to noise levels. The 5mm probe experiments on
the INOVA 500 were regulated at 25°C. The experiments run at lower field strengths
were run at ambient room temperature (-21 or 22° C).
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4. Results and Disscusion
4.1 Tetrafluorophenol (TFP) resin
It is commonly known that pentafluorophenol carboxlylate esters are used for amide
coupling reactions [73]. The pentafluorophenol acts to activate the ester making it more
susceptible to a wide array of N-nucleophiles. Therefore, it is reasonable to assume that
if a method could be devised to generate a polymeric version of this activating group,
the carboxylate esters would show a similar increase in reactivity towards N
nucleophiles. By reacting 4-hydoxy-2,3,5,6-tetrafluorobenzoic acid with aminomethyl
ploystyrene, a new ploymeric 4-hydroxy-2,3,5,6-tetrafluorobenzamido (TFP) resin is
produced [73]. Scheme 1 (page 28) summarizes TFP resin preparation. Fluorine-19
MAS NMR can follow each of the three steps in the preparation of TFP resin (Figure 1,
page 29). A mixture of products, including ester formation, is observed in spectrum A.
From spectrum A, it is clear that there are more than the expected 2 fluorine peaks from
the 2 pairs of equivalent fluorine atoms. The second step involves the unmasking of the
phenol by incubating the resin with a small excess of piperidine (spectrum B). The final
step is a removal of the piperdine salt by exposure with HCI (2 M) in DMF (spectrum
C). The final TFP resin gives very consistent 19F NMR signals at -144.8 and -161.8
ppm. Spinning sibebands are observed for the move intense peaks. The final product is
washed with DMF. THF. and dichloromethane and then dried under vacuum at 45°C to
give TFP resin. In the TFP resin paper by Salvino et. al. [73]. resin loading was
detennined by elemental analysis by fluoride ion selective chromatography to be 1.17
millimolcs per gram of resin (mmol/g).
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Scheme 1- Tetrafluorophenol (TFP) resin Preparation.
O:;N AF F OF F
~N~~OH~NH, + HO'O*OH
,Ofi
~N~OH+ole
F F F F F F FDMF
CDMF 1 0
~ ~~N ~-!J OH
Aq.HCI
~N ;!J o· 0F F DMF +N
F F
B
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Figure 1: 19F NMR ofTFP resin preparation (scheme 1)
Scheme 1: product A
OF F
~N~OH+F F
A
OF F \F)=(
~N~O ~OHF F F , F
tv\0
I I I I I i I (I illIii I I I! I '~I--l~' 1 II
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
Scheme 1: Product B
~F
~N ~-~ 0- 0+N
F F
BI Ii j 1 Iii i----T~'-l~,--l l~-rl~-----,----rl I i -T I I I I 11
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
Scheme 1: Product C TFP resin
jtF>=(~N V-0H
F· F
c A
I I !T'-- I I ,. 1 I I I I I I I r--r T-- ,----, I iIi , I I 1 I I I [I I l ' I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
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A brief comparison of NMR probes and sample techniques was conducted. The results
of this comparison study are summarized in Table 1 (page 31). The two NMR probes
used in this study include the Nano· nrnr ™ probe and a 5 mm Varian Z.Spec ™ IHl19F
probe. The 5 mm NMR experiments were conducted on a Varian INOVA ™ 600 MHz
spectrometer (vs. 500 MHz for the Nano· nrnr ™ probe). Based of the results from
Table 1 (page 31), the Nano· nrnr ™ probe clearly provides superior performance and
should be selected to study 19F NMR of resin-bound molecules. The figure of merit was
generated by dividing the signal to noise ratio by the square-root of the number of scans
and then dividing this value by the amount of resin (mg) used in that particular sample.
The figure of merit value for the Nano· nmr ™ probe is more than an order of
magnitude higher than the 5 mm probe, regardless of the sample technique used. The
receiver coil length for the 5 mm probe is 1.8 em. It was empirically determined that
approximately 23 mg of this particular TFP resin was needed to fill the receiver coil of
this probe with a swelled resin "plug". Susceptibility matched plugs (Doty Scientific)
were used in Sample D for an effort to circumvent susceptibility issues that would be
expected in Sample C. Use of these plugs resulted in approximately a 10 %
improvement in the linewidth at half-height (558 vs 620 Hz). The 5 mm sample
containing roughly 69 mg (Sample B) of swelled resin produced the best linewidth (359
Hz) of the three 5 mm samples. Evcn this rcsult was much broader than the
Nano· nmr Thl probe at 96 Hz (Sample A). According to the results of thc above
comparison study (Table I). an ordcr of magnitude less sample (0.4 mg of rcsin) could
he used in a quantitation study using the Nano· nmr Thl probe.
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VJ
Table 1: Comparison of NMR Probes and Sample Techniques using TFP resin.
Normalized Figure of Merit
SampleSIN for 1 scan SIN
NMR Field- Linewidth at Signal to noise Number ofSample probe strength amount halfbeight ratio (SIN) scans (NS) SIN JNS
(MHz) (mg) (Hz) JNS Sample (mg)
A NANO 500 4.06 ± 0.1 96 363 16 90.8 22.4
BIHll9F
600 69± 10% 359 205 32 36.2 0.52(5mm)
CIHlI9F
600 23 ± 10% 620 168 128 14.9 0.65(5 mm)
DIHJ19F
600 23 ± 10% 558 287 128 25.4 1.10(5 mm)
Sample A: 4.06 mg of resin swelled in DMF.Sample B: - 69 mg of resin swelled in CDCI3 (- 6 cm of swelled resin).Sample C: - 23 mg of resin swelled in CDCI3 (1.8 cm of swelled resin) floated into probe receiver coil with excess solvent.Sample D: - 23 mg of resin swelled in CDCl3 (1.8 em of swelled resin) with susceptibility matched plugs above and
below the swelled resin.
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With a 16 scan experiment on 0.4 mg of this TFP resin, a signal to noise ratio of
approximately 40 to 1 would be expected.
An NMR method for TFP loading analysis was also developed. A 2.00 mL volumetric
stock solution of 3-flurobenzamide (aldridge) was prepared be dissolving 34.783 mg.
into DMF-d6 (D, 99.5%) to produce a 0.125 M standard solution in a 2 mL volumetric
flask. Using a Metler microbalance, 3 to 4 mg of nine different TFP resins were
carefully weighted into nanotubes. Six samples of each resin were used in this study. A
2-20 III Eppendorf pipet was used to carefully add 20 III of the standard to each
nanotube containing the pre-weighed TFP resin. Because of the small size of the
nanotubes, gel-electrophoresis transfer tips were used with the Eppendorph pipet. The
initial addition of stock solution served two purposes. The first was to add a known
amount of a fluorine containing standard to the resin. The second was to swell the resin
in DMF-d6. The total volume of a typical nanotube is approximately 40-50 Ill.
Therefore another 20 III of DMF-d6 was added to each sample and a Teflon plug was
inserted in the tube opening. A small spinner was placed at the top of each tube and the
sample was inserted into the Nano· nmr Thl probe at the magic angle, through a small
window in the side of the probe. The probe was then inserted into the magnet and the
appropriate cables and air lines connected. This is one of the biggest drawbacks of the
Varian Nano . nmr Thl probe. The probe must be removed from the magnet every time a
new sample is introduced. Removing the probe for each sample has a negative impact
on sample throughput. A reasonable amount of care must be taken to ensure the probe
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is not damaged during this procedure. Removing the sample from the probe just
requires tilting the probe to\he side and sliding the sample out. All samples were spun
at a rate of 1000 to 1500 Hz. Spinning the sample should be done in stages of 500 Hz.
This will ensure the sample is rotating properly in the probe. The sample should spin at
a constant rate during the entire experiment. If the spin rate begins to fluctuate, the
sample is essentially wobbling in the probe and will eventually cause damage. An
experiment was performed to determine the minimum relaxation delay (dl) need to give
quantitative results. By arraying dl, it was determined that a dl value equal to 2.7 sec.
was the minimum dl required before the 19F signal reached an equilibrium. This
experiment used a pulse width of 900 (pw90) for 19F (in this particular probe) of 8.1
microseconds. Because the experiments were used to quantify 19F signals, the pulse
width (pw) was set to 3.3 microseconds and a dl value of 10 sec. By decreasing the
pulse width and increasing the relaxation delay, this gave sufficient time for the 19F
nuclei to completely relax before the next pulse was applied. Using the above described
method, 19F NMR data for each resin were obtained. Figure 2 (page 34) displays an
example of the 19F spectra obtained for these samples. The internal standard 19F
resonance is at approximately -112 ppm and the resin peaks are at -144 and -162 ppm
respectively. The transmitter offset was placed between the internal standard at -112
ppm and the first upfield resin peak at -144 ppm. The transmitter offset was centered
(between the internal standard and resin signals) in an attempt to insure that all of the
19F nuclei would receiYe the same amount of radiofrequency energy from each pulse of
the transmitter.
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v.l.j:::.
Figure 2: TFP loading wi internalSTD.
3-Fluorobenzamide added as internal standard
F
CKNH2If ~
- 0
A
AF)=(~N UOH
F F
A
I I I I I I------.---l~--~i I I I I I' I I
-100 -1l0 -120 -130 -140 -150 -160 -170 ppm
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The following equation was developed to determine the mmollg loading of TFP on the
amino-methyl resin:
Millimoles/g Resin = (lr)(Qs)
Ir =Average integral value of two integrals for resin signalsQs =Moles of Standard added (2.5x 10-6, use 2.5 in calculation)Is =Integral of standardWr =Mass of resin used (mg.)
The integrals for the resin peaks were processed three different ways. The first process
carefully cut the integrals of the spinning sidebands (2 sidebands) and the resin peaks
separately, and then adds the three values together. The second process included only
the resin peaks and ignored the side bands. The third process cut a larger integral to
include the spinning side bands and the resin as one integral.
Two slightly different calculations were used to generate the mmollg data found in Table
3. The downfield resin peak at -144 ppm representing two fluorine nuclei is the only
peak used in the first calculation (Calc I). An average of the two fluorine signals from
the resin representing a total of four fluorine nuclei is used in the second calculation
(Calc 2). Seven different TFP resins were used for this quantitation study. Tables 2 thru
4. (pages 36 thru 38) are a summary of all the data and results. Figures 3 thru 8 (pages 39
to 44) display plots of the 19F NMR \'s. fluorine elemental analysis results. Using
elemental analysis as an accepted method. the second process has a slope closest to a
value of 1.
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Table 2. TFP Loading study (NMR data and Elemental Analysis Raw Data)
Integration Integration Integration ElementalSample Mass Standard Process 1 Process 2 Process 3 Analysis
(1112) (%)
1 3.806 100 320.1 314.7 283.2 277.8 325.1 320.7 8.863.641 100 420.8 408.4 376.6 365.9 430.0 417.3 8.713.649 100 368.4 356.8 328.0 317.3 383.6 374.3 8.633.699 100 377.5 372.3 338.5 332.7 392.7 388.4 8.463.754 100 381.0 380.7 346.1 336.3 382.4 384.0 8.693.722 100 401.5 394.8 366.6 357.8 403.8 399.8
2 3.883 100 326.1 316.3 299.7 289.7 339.1 330.6 7.513.906 100 343.3 334.0 304.7 295.3 345.3 335.6 7.723.846 100 274.0 260.7 243.7 235.2 285.6 272.4 7.663.635 100 304.6 301.0 275.7 268.9 314.8 311.5 7.473.885 100 308.6 297.0 277.4 267.8 321.8 311.8 7.843.620 100 306.3 303.1 279.3 267.9 315.0 315.1
3 3.825 100 116.0 112.7 105.0 100.7 118.8 115.7 2.804.039 100 120.9 116.7 110.5 104.1 124.8 118.6 2.834.041 100 122.5 117.8 109.6 101.7 125.0 117.2 2.813.979 100 116.5 114.5 105.9 99.9 121.8 116.6 2.734.049 100 119.9 117.8 110.9 106.8 121.8 118.9 2.744.014 100 104.9 101.3 92.7 87.8 106.6 101.7
4 3.964 100 455.3 449.7 425.4 419.0 476.4 472.0 8.654.138 100 512.1 500.9 459.5 448.4 535.0 519.9 8.713.985 100 437.4 431.6 393.1 380.4 443.2 435.2 8.684.041 100 394.2 391.6 361.5 353.6 419.4 410.6 8.933.808 100 451.9 438.0 419.2 409.9 472.7 463.7 8.734.057 100 351.3 344.3 329.8 322.1 371.8 368.2
5 4.060 100 394.1 383.0 370.0 362.2 420.3 412.4 7.133.806 100 292.4 283.0 279.2 270.4 312.3 304.4 7.293.852 100 308.9 305.0 291.5 283.7 322.2 306.8 7.243.917 100 288.1 281.5 274.8 267.6 308.8 303.0 7.274.062 100 300.3 293.7 278.0 270.0 322.0 315.9 7.334.025 100 301.9 299.2 287.2 281.4 320.2 318.3
6 3.409 100 120.7 120.4 101.7 97.9 127.2 125.7 2.813.626 100 103.7 102.1 95.5 83.6 111.8 109.7 2.633.500 100 112.3 111.9 98.0 95.7 117.0 116.4 2.733.500 100 86.9 84.9 76.5 68.1 92.5 90.6 2.803.571 100 105.4 102.4 96.0 86.4 112.8 105.1 2.773.565 100 112.6 112.7 100.3 9.15 119.4 120.2
7 4.107 100 491.5 484.7 455.5 446.7 507.2 501.3 9.883.984 100 467.6 463.6 433.4 427.6 480.1 478.6 9.983.BiO 100 456.9 450.0 423.6 418.9 4i2.6 467.6 9.914.0n 100 466.4 460.& 434.3 427.9 481.9 4i8.9 9.663.902 100 496.8 485.2 4iO.6 457.9 516.8 506.8 9.493.909 100 389.6 381.2 363.3 359.0 402.1 39-1.1
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Table 3. TFP Loadin~study (mM Fluorine I g resin)
Sample Process 1 Process 2 Process 3Elemental
Calc 1 Calc 2 Calc 1 Calc 2 Calc 1 Calc 2 Analysis
1 1.0513 1.0424 0.9300 0.9212 1.0678 1.0605 1.16581.4445 1.4233 1.2928 1.2745 1.4762 1.4545 1.14611.2620 1.2421 1.1234 1.1051 1.3139 1.2981 1.13551.2757 1.2668 1.1437 1.1340 1.3270 1.3197 1.11321.2685 1.2680 1.1525 1.1362 1.2734 1.2759 1.14341.3483 1.3371 1.2310 1.2162 1.3562 1.3494
2 1.0497 1.0340 0.9648 0.9486 1.0917 1.0780 0.98821.0985 1.0836 0.9750 0.9600 1.1051 1.0895 1.01580.8901 0.8690 0.7920 0.7782 1.9284 0.9067 1.00791.0475 1.0413 0.9481 0.9363 1.0826 1.0769 0.98290.9929 0.9743 0.8925 0.8771 1.0354 1.0193 1.03161.0578 1.0521 0.9643 0.9447 1.0878 1.0879
3 0.3790 0.3736 0.3431 0.3361 0.3883 0.3833 0.36840.3742 0.3677 0.3419 0.3320 0.3863 0.3767 0.37240.3790 0.3717 0.3391 0.3268 0.3865 0.3745 0.36970.3659 0.3628 0.3328 0.3233 0.3826 0.3744 0.35920.3702 0.3670 0.3424 0.3361 0.3761 0.3716 0.36050.3265 0.3209 0.2885 0.2810 0.3321 0.3244
4 1.4356 1.4268 1.3415 1.3314 1.5022 1.4951 1.13821.5471 1.5300 1.3881 1.3713 1.6162 1.5934 1.14611.3720 1.3629 1.2331 1.2131 1.3901 1.3776 1.14211.2195 1.2155 1.1183 1.1061 1.2972 1.2837 1.17501.4832 1.4604 1.3761 1.3608 1.5516 1.5368 1.14871.0823 1.0715 1.0162 1.0044 1.1455 1.1401
5 1.2132 1.1961 1.1391 1.1272 1.2939 1.2818 0.93820.9605 0.9449 0.9168 0.9025 1.0256 1.0126 0.95921.0024 0.9961 0.9458 0.9332 1.0455 1.0206 0.95260.9192 0.9087 0.8768 0.8653 0.9854 0.9726 0.95660.9240 0.9139 0.8554 0.8431 0.9910 0.9816 0.96540.9377 0.9335 0.8920 0.8830 0.9944 0.9915
6 0.4425 0.4420 0.3727 0.3658 0.4663 0.4635 0.36970.3575 0.3547 0.3293 0.3088 0.3854 0.3818 0.34610.4012 0.4004 0.3501 0.3459 0.4177 0.4167 0.35920.3103 0.3068 0.2734 0.2583 0.3302 0.3269 0.36840.3689 0.3636 0.3360 0.3193 0.3948 0.3813 0.36450.3946 0.3950 0.3516 0.3397 0.4185 0.4200
7 1.4959 1.4855 1.3864 1.3730 1.5436 1.5346 1.30001.4669 1.4608 1.3597 1.3507 1.5065 1.5040 1.31321.4757 1.4647 1.3681 1.3605 1.5264 1.5183 1.30391.4318 1.4231 1.3332 1.3235 1.4792 1.4747 1.27111.5914 1.57':.9 1.5077 1.4873 1.(,555 1.6395 1.2487
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" )/mMFIt d (Aa e " oa 109 S U ly verage UOrIne g resm
Sample Process 1 Process 2 Process 3 ElementalAnalysis
Calc 1 Calc 2 Calc 1 Calc 2 Calc 1 Calc 2
1 AveraQe 1.2751 1.2633 1.1456 1.1312 1.3024 1.2930 1.1408SId. Dev. 0.1299 0.1268 0.1233 0.1205 0.1340 0.1299 0.0190
%RSD 10.19 10.03 10.76 10.65 10.29 10.04 2.17
2 Average 1.0228 1.0091 0.9228 0.9075 1.0552 1.0431 1.0053SId. Dev. 0.0730 0.0773 0.0706 0.0697 0.0665 0.0717 0.0200
%RSD 7.14 7.66 7.65 7.68 6.30 6.87 2.01
3 Average 0.3658 0.3606 0.3313 0.3225 0.3753 0.3675 0.3661SId. Dev. 0.0199 0.0198 0.0213 0.0210 0.0216 0.0214 0.0058
%RSD 5.44 5.50 6.43 6.50 5.76 5.84 0.21
4 Average 1.3566 1.3445 1.2456 1.2312 1.4171 1.4045 1.1500SId. Dev. 0.1748 0.1710 0.1520 0.1509 0.1754 0.1713 0.0145
%RSD 12.89 12.71 12.20 12.26 12.38 12.20 1.67
5 Average 0.9928 0.9822 0.9377 0.9257 1.0560 1.0440 0.9542SId. Dev. 0.1122 0.1094 0.1036 0.1034 0.1188 0.1177 0.0099
%RSD 11.30 11.14 11.05 11.17 11.25 11.28 0.95
6 AveraQe 0.3792 0.3771 0.3355 0.3230 0.4021 0.3984 0.3616Std. Dev. 0.0448 0.0463 0.0339 0.0375 0.0450 0.0463 0.0096
%RSD 11.83 12.27 10.12 11.61 11.20 11.62 0.35
7 Average 1.4513 1.4399 1.3528 1.3416 1.4995 1.4907 1.2874Std. Dev. 0.1141 0.1133 0.1117 0.1076 0.1209 0.1206 0.0268
%RSD 7.86 7.87 8.25 8.02 8.06 8.09 3.44
T bl 4 TFPL d"
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Figure 3 Process 1 Calc 1 VS. Elemental Fluorine
C1 P1 V5. Elemental Fluorine
1.6000 ,-----------------------------------,y =1.1687x· 0.0684
R2 = 0.9853
1.4000
1.2000
1.0000
~g 0.8000a::;;z
0.6000
0.4000
0.2000
1.60001.40001.200006000 0.8000 1.0000
Elemental (mMlg)
0.40000.2000OOOOO+-----,-------r-----r-----,------,------.----.----~
00000
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Figure 4 Process 2 Calc 1 vs. Elemental Fluorine
C1 P2 VB. Elemental Fluorine
1.6000 ,---------------------------------,y = 1.0855x • 0.0757
R2 =0.9843
1.4000
1.2000
1.0000
~.§. 0.8000a::Ez
0.6000
0.4000
0.2000
1.60001.40001.200006000 08000 1.0000
Elemental (mMlg)
0.40000.2000ooooo+----..,..----..,..----..,..----..,..----..,..----...,..----...,..---~
0.0000
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Figure 5 Process 3 Calc 1 vs. Elemental Fluorine
C1 P3 Y5. Elemental Fluorine
1.6,-----------------------------------,Y= 1.2049.·0.0631
R' =0.9845
1.4
1.2
~§. 0.8a:::l;z
06
0.4
0.2
1.60001.40001.20001.000008000
Element.1 (mMlg)
0.60000.40000.2000O-l-----~---.,...._---~---~--~---~---~---_1
0.0000
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Figure 6 Process 1 Calc 2 VS. Elemental Fluorine
C2P1 vs. Elemental Fluorine
y = 1.1585x· 0.0689R' =0.9845
1.4
12
~.§. 0.8a::::Ez
0.6
0.4
0.2
1.60001.40001.20000.6000 0.8000 1.0000
Elemental (mWg)
0.40000.20000-+----.,----......----...,..------,--------..-----,.----,-------10.0000
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Figure 7 Process 2 Calc 2 vs. Elemental Fluorine
C2P2 V5. Elemental Fluorine
1.6,----------------------------------,y=1.0824x· 0.0856
R' = 0.9838
1.4
1.2
~.§. 0.8a:;l;z
06
0.4
0.2
1.60001.40001.200006000 0.8000 1.0000
Elemental (mMlg)
0.400002000O+-----r----,-----.----~---~---~---~---_;
0.0000
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Figure 8 Process 3 Calc 2 vs. Elemental Fluorine
C2P3 V5. Elemental Fluorine
1.6.------------------------------------,y=1.1992x· 0.0674
R' = 0.984
1.4
1.2
~.§. 0.8a::~z
0.6
0.4
0.2
1.60001.40001.200006000 0.8000 1.0000
Elemental (mMlg)
0.40000.20000+----...----...,..-----,------,-----,-----.,..----.,-----10.0000
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Whether one or both fluorine signals were used in the calculation did not have much of
an impact in the results. The range of values for the TFP resins was from 0.38 to 1.49
mmol/g. The Relative Standard Deviation (RSD) was 5 to 10 percent. The 19F NMR
method appears to have good linearity over the range of values observed in this study.
The seven resins that were used in the 19F NMR TFP loading study were also sent to
Robertson Microlit. Laboratories, Inc. in Madison NJ for fluorine elemental analysis.
This lab analyzed for fluorine by combusting the resin with oxygen in a closed flask.
The resulting ionic fluoride was absorbed in Total Ionic Strength Buffer (TISAB) and
subsequently analyzed using a fluoride-ion specific electrode. These results compare
closely with the NMR results. The RSD for the elemental analysis results are smaller
than for the NMR results. This might be explained by an error analysis of the NMR
method. Accurately weighing 3 to 3.5 mg of resin into 40 TI nanotubes was certainly a
unique challenge. Transferring the standard in 20 ~l of DMF d-6 also had to be done in
a careful manner. Fortunately, the dry resin rapidly absorbed the initial 20 ~L,
containing the standard and reduced the risk of spilling the standard or the resin. The
use of the Varian Nano· nmr Thl probe, in this particular study, actually helped to
eliminate potential error. Making gel-phase resin samples in a 5mm NMR tube
generally produces a resin plug and a variable amount of excess solvcnt. It is ncarly
impossible to add just the right amount of solvcnt to just swcll the resin. This potcntial
source of crror produces a sample with what could be describcd as a biphasic
cnvironmcnt. Whcn a small-molccule intcrnal standard is addcd. the concentration of
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this standard in the gel-phase region of the sample will be different than that found in
the excess solvent. Because the resin is insoluble, the small molecule standard cannot
completely penetrate the resin core. If the gel-phase region of the sample is in the
receiver coil of the probe, the signal from the internal standard will appear to be smaller
than it actually should be. Because the entire sample volume of the nanotube is in the
receiver coil of the Nano . nmr ™ probe, the fluorine signals from the resin and standard
are an accurate representation of the entire sample. Therefore, this 19F NMR method for
determining TFP loading would not work using a traditional 5 mm NMR probe. As the
TFP loading decreases, it becomes more difficult to determine the location of the
spinning sidebands. The intensity of the spinning sidebands also decreases
significantly. As the TFP loading value approaches 1.0 mmol/g of resin (Table 3, page
37), processes 1 and 3, which include the spinning sidebands, display a higher value
than process 2 or the elemental analysis results. Process 2 is the closest to the elemental
analysis data and is therefore the preferred NMR data processing method. Concerning
accuracy and lower overall error, the elemental method is probably better suited for
determining loading of bulk TFP resin preparations. The TFP resin was generated in
batches of 600 grams. Sending out 50 mg to a contract lab for fluorine analysis was not
a large concern as far as sample loss was concerned. An in-house method for quickly
checking TFP loading right after synthesis proved useful.
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Scheme 2 (page 48) is a summary of the methods for producing a variety of activated
carboxyl and sulfonate esters. These activated esters are then reacted with a variety of
amines to generate the desired amide libraries. The bottom of Scheme 2 (page 48)
shows the structure of two acids chosen to demonstrate TFP resin loading and product
formation. Typical l H NMR data of polystyrene resins in a Nano· nrm ™ probe are
displayed in Figure 9 (page 49). Spectra Band C correspond to acids 1 and 2 loaded
onto the TFP resin. Determining resin loading based on proton data alone would not be
an easy task. In Figure 10 (page 50), two new 19F NMR signals emerge at -141.7 and
152.0 ppm, which account for the acid loaded TFP resins. It is a simple matter to
compare the integrals of these new signals with the original TFP signals to determine
loading. In contrast to elemental analysis, 19F NMR can actually discriminate between
starting TFP resin and resins that have been loaded to form carboxylate esters 2 and
sulfonate esters 3 (Scheme 2, page 48). If a particular carboxylic acid loading reaction
only proceeds to 50%, the final product would be half of the expected amount.
Therefore, 19F NMR can be used to follow the entire reaction sequence. Another
advantage to using 19F NMR is the simplicity of the NMR data. By looking at a simple
1D 19F spectrum, a combinatorial chemist can quickly determine how well the reaction
has proceeded. An arbitrary loading value of 75% could be selected by the
combinatorial chemist as a minimum amount needed before the activated resin could be
used for further chemistry. If the loading was less than 75%. the resin could be exposed
to the loading reaction conditions again. in an effort to improve loading. or simply not
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Scheme 2- Activated Ester and Final Product Formation
ii
~N~)(A.. iv .. AF F 0 R'-N R
~2
~NH2 .. W"N ~-O OH
F F
~o0" ,,0
iii
~N ~-IJ O-~-Riv '8
• • R'-N" 'R
F F 0
3
Key: (i) 2,3,5,6-tetrafluoro-4-hydroxybenzoic acid (1.7 equiv), DIC (1.5 equiv),DMF, HOBt (1.5 equiv), 25° C, 16 h; (ii) acid (2 equiv), DIC (2 equiv), DMAP(0.2 equiv), DMF, 25° C, 3-22 h; (iii) sulfonyl chloride (2.0 equiv), DIEA (3.0equiv), DMF, 25° C, 2 h; (iv) amine (0.8 equiv), DMF, 25° C, 1-12 h.
Carboxyl (2) and sulfonyl (3) activated esters are prepared from TFPresin (Scheme 2). These activated esters are then reacted with avariety of amines to generate the desired amide libraries.
Acid 1
H s
~N\\~~ N
OH
o
Acid 2
48
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Figure 9: 'H NMR, nanoprobe on INOVA 500
A\;~N UOH TFP
F F
l----,- ~~U\JL-.l'\,
B I I I i I I I i I I I I i r-- I I I I -. I I I ,--- I I I I I I I I I I I I I I i I I i I I i I Iii I I I I
AI I Iii I I i I I i I I I i I I I I i I I i II I i I I I i I I Ii' iii i II I I I I I I I I I I I I I , I 4 3 2 1 ppm
10 9 8 • 7 6 5OF F
~N~O~;'>-~--COF F
TFP-Acid 1 (loading?).p.\0
AF
)=(~N Uo-CyV'
F F 0
10 9 8 7 6 5 4 3 2 ppm
TFP-Acid 2 (loading?)
I I I I I I I I I I I I , I I I l----r 1 ' I ,---1 I I--T---' I I '--T---' I I I I I I i I
10 9 8 7 6 5 4 3 2 I p~m
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A
Figure 10: 19F NMR, nanoprobe on INOVA 500
5e)=(~N UOH TFP
F F
'---- f\ .liill!!ll Ii I I Ii II Illli'j'llll'l II Ili-~l--'~-l~
-120 -125 -130 -135 -140 -145 -ISO -ISS -160 -165 -170 ppm
TFP-Acid I (35% loaded)
VIo
B
Jr)=(~N~}-~--CO
_ ,.,'." ~_ ....., ,,', "'" .,,~_L~~\ ......~,. "'I; 4tJ~r ""tt"1lI Iii I iii I I I Iii ]---,-------,----T -j----.-----r-l- I r-'-----,---l I ~T -, I iii r-- Iii I I I I I I I i I I i I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
TFP-Acid 2 (75% loaded)
c
jr)=(~NUO~
F F 0
I I I I T----.--. T 1 '---f I I I 1--' T I I I I I I I I I 1 I I, I I I 1 I I I i I
-120 -125 -130 -135 -140 -145 -150 -ISS -160 -165 -170 ppm
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be used. Because Acid 2 met the 75% loading criterion, it was carried on for amide
production.
By using the Nano· nmr ™ probe, the line widths of the 19F resonances were greatly
reduced and the signals were well resolved from one another. But, was the use of this
probe really necessary to determine the loading of the TFP resins? Compelled by the
thought of spending days manipulating tiny nanotubes and sitting under a magnet
removing and inserting the Nano . nmr ™ probe, a loaded resin was placed into a 5mm
sample tube, swelled with CDC!) and 19F NMR data were acquired on a Broker VXR
300. The 5 mm tube data, displayed in Figure 11 (page 52), are from the same three
samples in Figure 10, but at 300 MHz. The chemical shift dispersion for 19F NMR is
large enough to allow for a rough estimate of loading. The resin plug, swelled in
CDC!], can be floated into the receiver coil. The sample size ranges from 20-50 mg
depending on how well each resin sample swells. At 256 scans per sample, 50 to 60
samples were run using automation on an overnight basis.
The reaction kinetics, of TFP resin formation chcmistry, were also explorcd by using 19F
NMR observations. Typical loading rcaction conditions for estcr formation wcre
reproduced in a nanotube and 19F NMR data \\'ere collected. Thc results from this study
are displayed in Figure 12 (page 53). Thc reaction approaches complction after
approximately 100 minutes. Thc combinatorial chcmists wcrc under thc impression that
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Figure 11: 19F NMR, 5mm probe on VXR 300
JFH~NVOH
F F
TFP
VIN
A
B
.--1 I I I I I -, I I l"l~--r--' i I -,-- --~---l ~--, j----.----r-, -1--- l~---'---T ~---l 1 ~--l-- 1 l~-I I Tj
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
TFP-Acid 1
JF)={~N V~})-~--OO
F F
I I \ I I I I I T I I I---r---I-,--T--l '-1 i I I I I I I i [Ii I I , I I I I I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
/
TFP-Acid 2
c
IF)=(~NVO~
F F 0
I I I I I I .-.......,--------T--' ,-----,---, 1 I .------.----1 1 I I I I I I I iii I I I I I I I I' I I I I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
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Figure 12: Kinetics of Ester Formation on TFP R~sin
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these loading reactions could take several hours and were often done overnight. This
particular kinetic study was conducted in a single nanotube with an arrayed pre
acquisition delay and a 4 scan experiment every minute for several hours. These kinetic
data allowed the chemists to do the loading step in a couple of hours as opposed to
overnight. If there was any doubt of the success of the loading step, a 19F NMR
spectrum could be quickly obtained on the final product in a traditional 5 mm NMR
tube on an open access 300 MHz spectrometer. An effort was also made to investigate
the kinetics of amide product formation, but the reaction was too rapid to observe in the
time required to initiate data acquisition. By the time the Nano· nmr ™ probe was
inserted into the magnet, the reaction was complete. Salvino et al. [73] describe
detailed use of the TFP resin for producing a variety of structurally different amides and
sulfonamides. The products in that study were analyzed by HPLC-MS and found to
have a high level of purity with a single compound in each well.
Diethylamine and benzylamine were selected to demonstrate amide product formation
using the TFP-Acid 2 resin (Figure 11, page 52). Separate samples of the TFP-Acid 2
resin were re-swelled in DMF containing 0.8 equivalents of diethylamine and
benzylamine. The formation of the amide product simultaneously cleaves the product
from the resin. The amide product was filtered from the resin and dried. The IH NMR
data of both products dissolved in CDCl) in 5 mm tubes run on a Varian INDVA 500
MHz spectrometer are displayed in Figure 13 (page 55). The amide products are very
clean and represent about 5 to 10 mg of each sample. The structures were also
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UIUI
Figure 13: IU NMR of amide products from Acid 2 (5mm probe INOVA 500)
Acid 2, diethylamine product
~~~N/'\
o ~
II I I I 1 I 1 I I I 1-- , I I ,-~--.- I I I,
9 8 7 6 5 4 3 2 ] ppm
Acid 2. benzylamine product
~~~~~
o V
f
~
I I I I [I I I I I I I I I I I I 1 I i I I I I 'I I I i I I i I I I
9 8 7 6 5 4 3 2 1 ppm
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confirmed by LC-MS. The ability to determine resin loading by 19F NMR was critical
for estimating final product yield. After amide product formation is complete, the 19F
NMR signals from the remaining resin will return to the original chemical shifts of the
TFP starting resin unless there is excess amine added and it forms an amine salt with the
TFP resin after the product amide is cleaved. This amine salt formation effect is
observed for the diethylamine product formation and is displayed in Figure 14 (page
57). By simply performing an Hel wash to remove the amine salt, the 19F NMR signals
return to the original chemical shifts of the starting TFP resin.
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lJl-...l
A
B
c
Figure 14: Acid 2-TFP resin after diethylamine amide product formation.
Starting TFP resin.
jr>=<trN VOHF F
I I 1 I I I 1 I I I I r r -T--'--r-'---' I I I I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
Acid 2-TFP resin after diethylamine product formation.
jtF)=( +
~N )..(0- (N1F F
1 1 1 1 1 1 r ' T H T --'--1 1 T' ,- 1 1 1 I I 'I
-120 -125 -130 -135 -140 -145 -ISO -155 -160 -165 -170 ppm
Acid 2-TFP resin after diethylamine product formation and Hel wash.
jr>=<trN VOHF F
11
I I I I i I I I 1 I I I IT 1 I I i I I Iii I I I I I I I iii I I I I I I i I
-120 -125 -130 -135 -140 -145 -150 -155 -160 -165 -170 ppm
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4.2 Fluorinated Chloromethlypolstyrene (FCP resin)
Because of the success of the TFP resin in monitoring solid phase reactions, new
methods were explored to make use of 19F NMR. Scheme 3 (page 59) represents the
synthesis of a fluorinated chloromethylpolystyrene resin 5. This Fluorinated resin is
prepared by copolymerization of styrene (1), 4-fluorosyrene (2), 4-vinylbenzyl chloride
(3), and 1,4-divinlybenzene. By selecting a fluorinated monomer, this particular resin
has an internal fluorine standard. Along with the previously mentioned advantages of
using 19F NMR to monitor solid-phase synthesis, the FCP resin allows for analysis
independent of the resin sample mass. Since non-fluorinated residual solvents are
transparent to 19F NMR, the product resin can be analyzed immediately after washing to
remove excess fluorine-containing reagents [74], eliminating the time needed to dry the
resin before analysis. As with the case of TFP resin, a traditional 5 mm probe could be
used to acquire the 19F NMR data. It should be noted that significantly more scans were
required to result in reasonable signal to noise. Therefore the use of the Nano· nmr ™
probe produced remarkably better sensitivity with significantly less sample (3 to 5 mg
compared to 30 to 50 mg for the 5 mm NMR tube) and much narrower line widths.
Three FCP resins were produced using 5, 10, and 20% 4-fluorostyrene by weight.
Fluoride analyses were performed by Quantitative Technologies Inc.. in Whitehouse.
NJ. The fluorine was liberated by combustion with oxygen in a closed flask. The
resulting ionic fluoride was absorbed in total ionic strength buffer and subsequently
analyzed using a fluoride-ion specific electrode. The elemental analysis
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Scheme 3: FCP resin production.
1 2 3
+
4
suspensionpolymerization
~
CI
F
m
n
5
Scheme 4: Solid-phase Michael Addition Reactions
m
0
o>ryo
~~ R2
n
A,
Fm
8a,b7 a. R,=CF3, R2=H
7 b, R,=H. R2=F
Bases a-hSH THF. 20 C
n¢:1 72hrs+ ~
R2
A,
On, j=\
o ~
F
6
Bases: a, CS2C03; b. K2C03 ; C. NaOCHJ ; d. LiOH; e, (C2HshN; f, LiN[Si(CH3hb;g, , ,8-diazabicyclo[5.4.0jundec-7-ene; h, (n-C~H9)NOH.
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was replicated five times on each of three different days. By changing the 4
fluorostyrene content, it was discovered that an internal standard loading of 0.32 mmol
Fig resin was sufficient to give reasonable signal-to-noise (~ 15) in an acceptable
amount of NMR spectrometer time. Using approximately 50 mg of resin 5, with a
loading of 0.32 mmol Fig, swollen in CDC!] in a 5 mm NMR tube, the acquisition time
with a 200 MHz (188.23 MHz tuned to 19F) NMR spectrometer was approximately 6
minutes. At 500 MHz, using the Nano . nmr ™ probe with 3 mg of resin, the acquisition
time was 1 minute.
In order to demonstrate the utility of the FCP resin, a series of solid-phase Michael
addition reactions were investigated (Scheme 4, page 59). The thiophenols 7a and 7b
were reacted with a resin bound cinnamic acid ester 6 using parallel conditions. The
only difference between each reaction was the selection of the catalytic base. The
thiophenols that were used in this study have fluorine groups, which were used to
monitor reaction pro&ress by 19F NMR. The list of bases used include the following: a,
CS2C03; b, K2C03; C, NaOCH3; d, LiOH; e, (C2HhN; f. LiN[Si(CH3hh; g, 1,8
diazabicyclo[5.4.0]undec-7-ene (DBU); h, (Il-C4Hg)4NOH. All thc 19F NMR data wcrc
collected using thc Nano . nmr probc with rcsins swclled in DMF-d7. Reactions
occurred in a quantitativc manner for bascs d (lithium hydroxide) and f (lithium
hexamethlydisiylamide) (Figurc 15. pagc 61).
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Figure 15. Michael Addition Reaction Yields.
1.81.6
_1.4~ 1.2oE 1E- 0.8'tJQ) 0.6>= 0.4
0.2o
- -
....
....- ....
- - -
- - - 1- -
-
-+--1:- -+-~I~Lr-- rL 11..
a b c d e 9 h
Base cataIyst
Figure 15. Yields (mmol/g) of resin-bound adducts according to Scheme 2for 8a (black) and 8b (white). Base catalysts are as defined in Scheme 4(page 57).
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The 19F NMR data for the Michael addition product 8b resulting from base catalyst g
(OBU) is displayed in Figure 16, spectrum A (page 63). In Figure 16, two distinct 19F
NMR signals are observed. These signals are well resolved, further demonstrating the
utility of the Nano· nmr ™ probe. The internal standard 19F resonance is at -117.3 ppm
and the reaction product is at -111.9 ppm. In comparison to the internal standard of
0.32 mmol FIg resin, the 19F integration value of the product loading of 8b was
calculated to be 0.69 mmollg. The infrared spectrum of 8b is displayed in Figure 17
(page 64). An incomplete Michael addition reaction with base g (vc=o 6 at 1712 em-I
and Vc=o 8b at 1737 em-I) is indicated by the IR data. Unfortunately, the overlap of the
infrared signals makes it difficult to generate quantitative information based on infrared
data. If the reaction yield was below 0.25 mmollg, the product was not detectable by IR,
but was quantifiable by 19F NMR to a limit of approximately 0.05 mmollg. Figure 16
spectrum B (page 61) displays the 19F spectrum of resin 8b product from catalyst h.
The yield of the Michael adduct was determined to be 0.08 mmollg.
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0\w
A
B
Figure 16: 19F NMR Spectra of Michael Additions.
Nanoprobe 19F NMR spectrum of product resin 8b from basecatalyst g (DBU). Integration values (ppm): 216 (-111.8);100 (-117.3).
f
I I I I --T--~ I --,-----,--- I I T- -T---I I -r----, I ,- -----,--- I I
-95 -100 -105 -110 -115 -120 -125 -130 ppmy
215.77100.00
Nanoprobe 19F NMR spectrum of product resin 8b from basecatalyst h. Product yield determined to be 0.08 mmol/g.
I Iii Ii, I i I Iii I i I
-95 -100 -105 -110 -115 -120 -125 -130 ppmy
25.77
100.00
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Figure 17. IR Data of Michael Addition
Figure 17. Ester carbonyl stretching absorption of product resin 8b from basecatalyst g (OBD).
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5. Conclusions
Fluorine-19 NMR is a versatile technique in the study of resin-bound molecules. The
advantages of 19p NMR include: high sensitivity, high natural abundance (no isotope
labeling required) and a large spectral dispersion when compared to I H NMR. Pluorine
19 NMR was used to study the preparation of Tetrafluorophenol resin. A 19p NMR
method was demonstrated for quantifying the reaction of aminomethyl resin with 4
hydroxy-2,3,5,6-tetrafluorobenzoic acid using 3-fluorobenzamide as an internal
standard. The use of the Varian Nano· nmr TM probe was essential in developing this
method because the entire sample is represented in the active volume of the received
coil of the probe [66]. This internal standard quantitation method compared well with
established elemental analysis methods. This internal standard method could also be
applied to any resin chemistry in which a fluorine containing reactant was involved.
The acid loading reaction chemistry was also investigated using 19p NMR. The ester
formation reaction between the TFP resin and the acid group causes a distinct chemical
shift change of the fluorine signals. The chemist could simply measure the integrals
between the loaded and starting TFP resin 19F NMR signals. If the acid loading reaction
did not produce a desired percentage of loading, the loading reaction could be repeated
before amide library production commenced. This NMR method of measuring acid
loading on TFP resin was transferred to an ARX Bruker 300 and run in traditional 5mm
NMR tubes using oyernight automation. The automation allowed to chemists to
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optimize the TFP loading reaction step of the amide library production in an efficient
manner compared to running 50 to 60 samples per day using the Nano· nrnr TM probe.
Tetrafluorophenol resin loading kinetics were also investigated using 19F NMR. These
studies afforded the chemists with reliable information regarding time constraints for
loading reaction chemistry. This information allowed the combinatorial chemists to set
up more reactions in a shorter period of time rather than assuming they would need to
set up reactions over night. Fluorine-19 NMR was also used to observe amide product
formation. The TFP 19F NMR signals would return to their original chemical shifts
after the libraries were produced.
A slightly different approach in the use of 19F NMR to quantitate reaction yield was
developed by utilizing the fluorinated chloromethlypolystyrene resin. The fluorine
"'---,containing standard was copolymerizedJnto the backbone of the resin. An accurate
resin mass was no longer needed to determine reaction yield. FIourine-containing
reactants were used with the fluorinated cloromethylpolystrene resin to optimize a series
of Michael addiction reactions with a variety of catalytic bases. Lithium hydroxide and
LiN[Si(CH3)3h were determined to catalyze quantitative yields of this particular
reaction.
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As seen in several examples, the 19F NMR spectra of resin-bound organic molecules are
easy to interpret and relatively simple. Fluorine-19 NMR is a powerful tool for
optimizing reactions on solid-supports and is suitable for quantitation of reaction yields.
Although the tetrafluorophenol resin has found utility in amide library production, it is
this author's opinion that the fluorinated chloromethylpolystyrene resin offers the
greatest potential for future use. Most combinatorial libraries contain several if not
many members with 19F incorporated into their structure. These 19F nuclei can afford
almost a limitless potential for reaction condition optimization. Considering that a
majority of the time in any combinatorial effort is spent optimizing chemistry and not
actual library production, the potential impact of the fluorinated
chloromethylpolystyrene resin and reaction monitoring using 19F NMR and the Varian
Nano· nmr ™ probe as a combinatorial library development tool is significant.
Compared to 'cleave and analyze' methodologies, 19F NMR provides an excellent
nondestructive alternative to investigate and optimize solid-phase reactions.
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6. References
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[3] Lam KS, l..ebl M, Krchnak V. (1997) The "One-Bead-One-Compound"Combinatorial Library Method. Chem Rev. 97: 411-448.
[4] Fruchtel JS, Jung G. (1996) Organic Chemistry on Solid Supports. Angew. Chem.Int. Ed. Engl. 35: 17-42.
[5] Egner B, Bradley M. (1997) Analytical Technniques for Solid-phase Organic andCombinatorial Synthesis. Drug Dis. Tech. 2: 102-109.
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[7] Fitch WL. (1999) Analytical Method for Quality Control of CombinatorialLibraries. Mol. Div. 4: 39-45.
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[9] Van B. (1998) Monitoring the Progress and the Yield of Solid-phase OrganicReactions Directly on Resin Supports. Acc. Chem. Res. 31: 621-630.
[10] Van B, Liu L, Astor CA, Tang Q. (1999) Determination of the Absolute Amountof Resin-bound Hydroxyl or Carbonyl Groups for the Optimization of Solid-phaseCombinatorial and Parallel Organic Synthesis. Anal. Chcm. 71: 4564-4571.
[II] Van B, Martin PC, Lee J. (1999) Single-bead Fluorescence Microspectroscopy:Detection of Self-quenching in Fluorescence-labeled Resin Beads. J. Comb.Choll. I: 78-81.
[12] Yan B. Gremlich HU, ~Ioss S. Coppola G~1. Sun Q. Liu L. (1999) A Comparisonof Various FTIR and FT Raman Methods: Applications in the ReactionOptimization Stage of Combinatorial Chemistry. .T. Comb. Choll. I: 46-54.
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[13] Yan B, Li W. (1997) Rapid Fluorescence Detennination of the Absolute Amountof Aldehyde and Ketone Groups on Resin Supports. J. Org. Chem. 62: 93549357.
[14] Russell K, Cole DC, Mclaren FM, Pivonka DE. (1996) Analytical Techniques forCombinatorial Chemistry: Quantitative Infrared Spectroscopic Measurements ofDeuterium-Labeled Protecting Groups. J. Am. Chem. Soc. 118: 7941-7945.
[15] Submuth R, Trautwein A, Richter H, Nicholson G, lung G. (1999) CombinatorialChemistry Synthesis, Analysis, Screening. G. lung Editor, VCH Publishers Inc.,New York NY. 499-532.
[16] Fitch WL, BaerTA, Chen W, Holden F, Holmes CP, Maclean D, Shah N, SullivanE, Tang M, Waybourn P. (1999) Improved Methods for Encoding and DecodingDialkylamine-Encoded Combinatorial Libraries. J. Comb. Chem. 1: 188-194.
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[18] Wang T, Zeng L, StraderT, Burton L, Kassel DB. (1998) A New Ultra-highThroughput Method for Characterizing Combinatorial Libraries Incorporating aMultiple Probe Autosampler Coupled with Flow Injection Mass SpecrometryAnalysis. Rapid COmm1l11. Mass Spectrom. 12: 1123-1129.
[19] Zeng L, Burton L, Yung K, Shushan B, Kassel DB. (1998) Automated Analytical/ Preparative High-Perfonnance Liquid Chromatography-Mass SpectrometrySystem for the Rapid Characterization and Purification of Compound Libraries. J.ofChromo A. 794: 3-13.
[20] Ventura MC, Farrell WP, Aurigemma CM, Greig MJ. (1999) Packed ColumnSupercritical Fluid ChromatographylMass Spectrometry for High-ThroughputAnalysis. Anal. Chem. 71: 2410-2416.
[21] Ventura MC, Farrell WP, Aurigemma CM, Greig MJ. (1999) Packed ColumnSupercritical Fluid ChromatographylMass Spectrometry for High-ThroughputAnalysis. Part 2. Anal. Chon. 71: 4223-4231.
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[22] Taylor EW, Qian MG, Dollinger GD. (1998) Simultaneous On-LineCharacterization of Small Organic Molecules Derived form CombinatorialLibraries for Identity, Quantity, and Purity by Reverse-Phase HPLC withChemiluminescent Nitrogen, UV, and Mass Spectrometric Detection. Anal.Chem. 70: 3339-3347.
[23] Hsu BH, Orton E, Tang SY, Carlton RA. (1999) Application of Evaporative LightScattering Detection to the Characterization of Combinatorial and ParallelSynthesis Libraries for Pharmaceutical Drug Discovery. J. Chrom. B. 725: 103112.
[24] Kiplinger JP, Cole RO, Robinson S, Roskamp EJ, Ware RS, O'Connell HJ,Brailsford A, Batt 1. (1998) Structure-Controlled Automated Purification ofParallel Synthesis Products in Drug Discovery. Rapid COm11lWl. Mass Spectrom.12: 658-664.
[25] Kibbey CEo (1997) An Automated System for the Purification of CombinatorialLibraries by Preparative LCIMS. Lab. Rob. Auto. 9: 309-321.
[26] Zeng L, Kassel DB. (1998) Development of a Fully Automated ParallelHPLClMass Spectrometry System for the Analytical Characterization andPreparative Purification of Combinatorial Libraries. Anal. Chem. 70: 4380-4388.
[27] Kaur S, McGuire L, Tang D, Dollinger G, Huebner V. (1997) Affinity Selectionand Mass Spectrometry-Based Strategies to Identify Lead Compounds inCombinatorial Libraries. J. Prot. Che11l. 16: 505-511.
[28] Hsieh YF, Gordon N, Regnier F, Afeyan N, Martin SA, Vella GJ. (1997) J. Mol.Diversity. 2: 189-196.
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Biography
I was born at the Grand View Hospital in Perkasie PA, USA, on February 17,1968. Myparents are Stanley P. Krolikowski and Barbara J. Krolikowksi of Souderton, PA. Iwas raised in Souderton, PA. My wife is Rhonda L. Krolikowski (Reichard) and I have2 children: Ethan - 3 and Abigail - 3.
I graduated from North Penn High School in Lansdale, PA in 1986 and from LibertyUniversity in Lynchburg, VA with a Bachelor of Science Degree in Chemistry andEducation in 1991. I have also been seen at Villanova University, St. Joseph University,and Temple University before getting lost in Bethlehem, PA and winding up at LehighUniversity. Despite the hard work, my experience at Lehigh has been very rewardingfor me. In a strange way, I really do not want this chapter of my life to come to a close.
I have worked for 12 years as an NMR Spectroscopist in the pharmaceutical industry atRhone-Poulenc Rorer (now call Aventis after its merger with Hoechst Marion Roussel)and most recently at Merck and Co. Inc. at West Point, PA. in the Preclinical DrugMetabolism Department. I study the structure of metabolites and try to understand theamazing mechanisms which enzymes use to generate them.
My interests include: automobiles (often mistaken for an obsession), backpacking,fishing, physics and astronomy and last but not least my faith in Jesus Christ. I live inPA, but my heart is in the Rocky Mountains and i can often be found daydreamingabout them. I am beginning to wonder what the heck I am going to do with myself oncethis paper is finished! Thanks again for your help Dr. Roberts. I am sure you are just asglad as I am to see this paper finished.
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