Open Access

Condensation oscillations in the peptidization of phenylglycine

  • Mieczysław Sajewicz1,
  • Monika Gontarska1,
  • Dorota Kronenbach1,
  • Marcin Leda2, 3,
  • Teresa Kowalska1 and
  • Irving R Epstein2Email author
Journal of Systems Chemistry20101:7

DOI: 10.1186/1759-2208-1-7

Received: 9 April 2010

Accepted: 18 August 2010

Published: 18 August 2010


In earlier studies, we showed that certain low-molecular-weight carboxylic acids (profens, amino acids, hydroxy acids) can undergo spontaneous in vitro chiral conversion accompanied by condensation to from oligomers, and we proposed two simple models to describe these processes. Here, we present the results of investigations using non-chiral high-performance liquid chromatography with diode array detector (HPLC-DAD) and mass spectrometry (MS) on the dynamics of peptidization of S-, R-, and rac-phenylglycine dissolved in 70% aqueous ethanol and stored for times up to one year. The experimental results demonstrate that peptidization of phenylglycine can occur in an oscillatory fashion. We also describe, and carry out simulations with, three models that capture key aspects of the oscillatory condensation and chiral conversion processes.


The remarkable phenomenon of spontaneous in vitro oscillatory chiral conversion of selected profens, amino acids, and hydroxy acids has been the focus of our attention for some time. We first observed oscillatory chiral conversion in selected profens: S(+)-ibuprofen, S(+)-naproxen, S,R(±)-2-phenylpropionic acid, S(+)-flurbiprofen, R(-)-flurbiprofen, and S,R(±)-ketoprofen [13]. Later we described an analogous behavior in several amino acids: L-alanine, L-α-phenylalanine, and L-tyrosine [46]. We have characterized similar phenomena in selected hydroxy acids [7, 8] (L-lactic acid, R-α-hydroxybutyric acid, S-α-hydroxybutyric acid, R-mandelic acid, and S-mandelic acid) as well. Most of these oscillatory chiral conversions take place with the acid samples dissolved in 70% aqueous ethanol.

The general scheme of these chiral conversions can be simply summarized as
If we consider chiral conversion of selected carboxylic acids in aqueous solution in greater detail, then eq. (1) can be written as [9]:
In anhydrous media and in the presence of trace amounts of water, the probable mechanism of chiral conversion is given by eq. (1b) [10]:

where X = -NH2, -OH, -Ar, etc., and Y = -R, etc.

We have suggested two simple models of oscillatory chiral conversion [11]. The simpler model [5, 12] is based on autocatalytic dimerization. Oscillations appear in this model in both enantiomer subsystems. Racemization is a linear reversible reaction coupling the two oscillating subsystems. This model is based on the oscillatory Templator model of Peacock-López and collaborators [13, 14].

In the second approach [15], oscillations appear as the result of coupling between enantiomers. This model appears particularly relevant for systems involving condensation or peptidization in which the condensate (dipeptide) SR has different chemical properties than RS, e.g., where only the residue on the left undergoes epimerization.

In subsequent papers [1618], we demonstrated via the biuret test [16] and 13C NMR spectroscopy [17, 18] that profens, amino acids, and hydroxy acids can also undergo spontaneous condensation or peptidization when stored for sufficient time in 70% aqueous ethanol.

Ivanov et al. [19, 20] have convincingly documented the oscillatory condensation of organosilanols (e.g., R2Si(OH)2 or RR'Si(OH)2). There are several analogies between the results presented in their studies and those found in our own laboratory, which have inspired us to focus on the dynamics of condensation or peptidization of chiral low-molecular-weight carboxylic acids. For this reason, and because of the potential importance of this process in synthetic biology and chemical evolution, we have decided to focus on the issue of peptidization of amino acids coupled to their oscillatory chiral conversion [16]. More specifically, we scrutinize here the dynamics of peptidization of the low-molecular-weight amino acids, R-, S-, and rac-phenylglycine. The primary analytical tool that we employ to monitor the spontaneous peptidization of phenylglycine samples dissolved in 70% aqueous ethanol is a non-chiral high-performance liquid chromatographic system with diode-array detection (HPLC-DAD). We also supplement this technique with mass spectrometry (MS). In addition, we propose three models that go beyond the schemes developed earlier [11] to capture key aspects of the condensation and oscillatory chiral conversion processes.

We note that Blackmond [21] has suggested a mechanism involving preferential catalysis by homochiral dimers to explain enantiomeric amplification in the Soai reaction, the autocatalytic alkylation of N-heterocyclic aldehydes by zinc dialkyls. Mickskei et al. [22] subsequently extended this idea to a detailed model and showed in numerical simulations that enantiomeric enrichment and oscillation can occur under appropriate conditions.



R-Phenylglycine and S-phenylglycine of analytical purity grade were purchased from Sigma-Aldrich (St Louis, MO, USA). Phenylglycine racemate was prepared by mixing optically pure R and S antimers in molar proportions of 1:1. For the spontaneous peptidization experiments, we used solutions of R-phenylglycine, S-phenylglycine, and rac-phenylglycine in 70% aqueous ethanol. The concentration of each optically pure enantiomer was 0.5 g L-1 (3.3 × 10-3 mol L-1). The racemic mixture contained each antimer at half the above concentration. Samples were stored in tightly stoppered colourless glass vials and allowed to age at 22°C. We also prepared analogous solutions of R-phenylglycine, S-phenylglycine, and rac-phenylglycine that were stored for one year at 22°C.


High performance liquid chromatographic analysis was carried out using a Gyncotek liquid chromatograph (Gyncotek, Macclesfield, UK) equipped with a Gyncotek Gina 50 model autosampler, Gyncotek P 580A LPG model pump, Gyncotek DAD UVD 340U model diode array detector, and Chromeleon Dionex v. 6.4 software for data acquisition and processing. The analyses were carried out in the isocratic mode, using an RP-18 (5 μm particle size) column (250 mm × 4.6 mm i.d.; Varian, Harbor City, CA, USA), and methanol-water (6:4, v/v) mobile phase at a flow rate of 0.6 mL min-1. The chromatographic column was thermostated at 35°C with a Varian Pro Star 510 model column oven.

Mass Spectrometric Analysis

Freshly prepared and aged phenylglycine samples were introduced into a Varian 500-MS model mass spectrometer and analyzed in the ESI mode (full ESI-MS scan, positive ionization, spray chamber temperature 45°C, drying gas temperature 150°C, drying gas pressure 25 psi, capillary voltage 70 V, needle voltage 5 kV). A Varian MS Workstation v. 6.9.1 software was used for data acquisition and processing.

Microbiological Tests

We tested for the presence of microorganisms in samples of R- and S-phenylglycine aged for one year using solid and liquid media. Composition of solid medium: meat extract, 2 g L-1; yeast extract, 2 g L-1, peptone, 5 g L-1, sodium chloride, 4 g L-1; agar, 15 g L-1, pH = 7.4. Composition of liquid medium: meat extract, 0.4 g L-1; enzymatic casein hydrolysate, 5.4 g L-1; yeast hydrolysate, 1.7 g L-1; peptone, 4.0 g L-1; sodium chloride, 3.5 g L-1.

With the solid medium, 100-μL aliquots of the samples to be tested were introduced and incubated for seven days at approximately the same temperature (ca. 21°C) at which the samples had been stored earlier. This experiment was repeated in triplicate. To 50 mL of the liquid medium, we added 100-μL aliquots and then incubated the samples for fourteen days at ambient temperature (ca. 21°C) with continuous shaking (260 rpm). This experiment was also repeated in triplicate. In none of the samples was growth of microorganisms observed. Longer incubation periods were not employed, due to the risk of sample infection.

As a control, we carried out a protein determination by the Bradford method [23] and also measured the light absorbance at λ = 260 nm in order to check for the presence of DNA in the two samples. The Bradford test gave a negative result, and the spectrophotometric measurement revealed no DNA in our samples. We therefore concluded that no microorganisms were present.

Results and Discussion


In Fig. 1 we present two mass spectra of S-phenylglycine, the first of a freshly prepared solution in 70% aqueous ethanol and the second of an analogous sample after a one-year storage period. Both spectra were recorded for the total samples, i.e., without any preliminary separation by LC-MS.
Figure 1

Mass spectra of S -phenylglycine solution in 70% aqueous ethanol; (a) freshly prepared sample, and (b) sample after one year storage period. Both samples were stored at 22°C.

Considered as fingerprints, the two mass spectra shown in Fig. 1 are quite different. It is evident that fragmentation of the aged sample (Fig. 1b) results in a much richer pattern than that of the freshly prepared one (Fig. 1a). The aged sample apparently contains a wider variety of species. In the fresh sample, the predominant ion appears at m/z 304, which can be ascribed to the [Phg2 + He]+ cation (where Phg2 represents the cyclic associative dimer composed of two phenylglycine molecules coupled by a pair of hydrogen bonds), whereas in the aged sample the same cation makes a relatively small contribution to the recorded fingerprint. The disappearance of this cation supports the notion that the aged sample contains new species originating from S-phenylglycine. We note that a second cation (at m/z = 289) appears in both spectra. This signal can be attributed to [Phg2 - NH + He]+, and in the aged sample it apparently predominates. As this ion, which also seems to be associated with the phenylglycine dimer, still predominates in the sample stored for one year, we conclude that structural transformation due to aging consumes a relatively small portion of the starting material.

The aging of S-phenylglycine dissolved in 70% aqueous ethanol is also mirrored in the respective chromatograms. Based on the results of biuret test [16], it seems that oligopeptides are the most probable outcome of this process. We compare the chromatograms of the freshly prepared S-phenylglycine solution with those stored for nine days and for one year (Fig. 2a-c).
Figure 2

Chromatograms of S -phenylglycine solutions in 70% aqueous ethanol registered at 275 nm; (a) freshly prepared sample, (b) sample after nine days storage, and (c) sample after one year storage. All samples were stored at 22°C.

In the HPLC experiment, we employ a non-chiral chromatographic system and focus on monitoring the appearance and/or concentration changes of species that evolve during the S-phenylglycine aging process. Peaks 1 and 2, which are present in all the samples, with retention times, t R , of 5.2 and 5.4 min, respectively, can probably be attributed to phenylglycine in two different associative forms. We make this assertion because a) the two peaks appear at similar retention times, suggesting similar chemical properties; b) they predominate in the freshly prepared sample; and c) their intensities decrease with time. The mass spectrometric evidence of two species apparently derived from phenylglycine at m/z 289 and 304, which we ascribed earlier to the [Phg2 - NH + He]+ and [Phg2 + He]+ cations, respectively, also supports our identification. A key feature, seen in the mass spectra shown in Fig. 1, is that the peaks evolve at different rates, which supports our hypothesis that S-phenylglycine appears in the system in two different associative forms.

We attribute the peaks with higher retention times to larger oligopeptides generated in the course of the sample aging. The results of the biuret test performed with S-, R-, and rac-phenylglycine [16] also indicate the presence of oligopeptides in aged samples.

In Fig. 3, we present chromatograms of a freshly prepared S-phenylglycine solution and one stored for a year. The aim of this comparison is to emphasize the differences at higher retention times, where the higher oligopeptides (which are not abundant enough to be seen in the nine-day sample) are likely to be found.
Figure 3

Chromatograms of an S -phenylglycine solution in 70% aqueous ethanol registered at 300 nm. (a) freshly prepared sample; (b) sample after one year. Insets in (b) show UV spectra of the separated species recorded near the maxima of the respective peaks.

Figure 3, and the absence of long retention time peaks after nine days, demonstrate that the accumulation of higher oligopeptides is a relatively slow process that may take months to yield measurable amounts of these condensation products. In the insets of Fig. 3b, we examine the peaks corresponding to the three species with the highest retention times in more detail. The different shapes of the UV spectra at different wavelengths and the observed bathochromic shifts support our association of longer retention times with more monomer units in the oligopeptide.

One goal of this study is to establish if the condensation products, i.e., oligopeptides, in an S-phenylglycine solution arise in a monotonic or an oscillatory manner. To investigate this question, we monitored chromatographic peak heights in an aging sample, as registered at 275 nm. These peak heights are roughly proportional to the concentrations of the respective chemical species. In Fig. 4, we present the time courses of peaks 1-5, numbered as in Fig. 2.
Figure 4

Chromatographic peak heights for (a) peaks 1-3, and (b) peaks 4 and 5 for an S -phenylglycine solution stored at 22°C for nine days. Peak numbers as in Fig. 2. Retention times: peak 1, 5.2 min; peak 2, 5.4 min; peak 3, 5.6 min; peak 4, 6.0 min; peak 5, 6.9 min.

Clearly, the peak heights change in a non-monotonic fashion. The linear correlation coefficients r for calibration curves determined from the peak heights for stable reference compounds using the same chromatographic conditions (HPLC-DAD system, chromatographic column and mobile phase composition) and at least ten data points always exceeded r ≥ 0.99. Moreover, the percent error on each individual peak height never surpassed ±5%. Thus, the trends of the peak height changes in Figs. 4a, b seem to confirm the oscillatory nature of the condensation process, though the limited time resolution precludes our establishing whether the reaction is truly periodic.

The height of peak 1 initially rises in an erratic manner. This growth may arise from hydrolysis of trace amounts of oligopeptide impurities present in the commercial sample and visible in the chromatogram in Fig. 2a. After ca. 110 h, the mean abundance of peak 1 starts to decrease in an oscillatory fashion, which can be ascribed to consumption of the starting amino acid through peptidization. This effect correlates with the time-dependent fall of the intensity of peak 1 seen in Figs 2a-c.

The mean intensity of peak 2 grows during the nine day observation period. Again, this behavior may result from hydrolysis of trace oligopeptide impurities or perhaps from interconversion of the two types of H-bonded phenylglycine dimers represented by peaks 1 and 2. Although the intensity of peak 2 increases during this intial nine-day period (see Figs 2a, b), after one year the intensity of peak 2 becomes almost negligible (see Fig. 2c). This eventual lowering of the intensity of peak 2 may correspond to the consumption of the phenylglycine through peptidization.

Peaks 3-5 can be attributed to oligopeptides initially present in our samples. During the nine days of our experiment, the general trend in the height of peaks 3 and 5 is oscillatory yet growing, while peak 4 is nonmonotonically diminishing. The long-term history of peaks 3-5 confirms a slow concentration growth of the respective oligopeptides (see Figs 2a-c).

The results presented in Fig. 4 support the oscillatory nature of S-phenylglycine peptidization. This oscillatory process can be schematically described by the following equations:

R-Phenylglycine and rac-Phenylglycine

We repeated our experimental protocol with samples of R-phenylglycine and rac-phenylglycine, recording mass spectra for freshly prepared solutions in 70% aqueous ethanol and for the analogous samples after a one year storage period. All spectra were recorded for the total samples, i.e., without preliminary separation and identification of any of the aging products by LC-MS. The results obtained are shown in Figs. 5 and 6.
Figure 5

Mass spectra of R -phenylglycine solutions in 70% aqueous ethanol; (a) freshly prepared sample, and (b) sample after one year storage. Both samples were stored at 22°C.
Figure 6

Mass spectra of rac -phenylglycine solutions in 70% aqueous ethanol; (a) freshly prepared sample, and (b) sample after one year storage. Both samples were stored at 22°C.

As with the S- enantiomer, the mass spectrometric fingerprints of the freshly prepared and aged R- and rac-phenylglycine samples differ considerably. Again, both samples show peaks at m/z 289 and 301, which we attribute to two different dimeric forms of the starting material. Again, the relative intensities of these two signals change in the course of aging so that in the freshly prepared samples the peak at m/z 289 is lower than that of the heavier ion, while after one year the reverse proportion is observed.

The mass spectra of the aged R- and rac-phenylglycine samples (Figs. 5b and 6b) differ, however, in important ways from that of the aged S species (Fig. 1b). In the latter case, we find a much richer array of signals originating from heavier ions than in the mass spectrum of the freshly prepared sample (see Fig. 1b vs. 1a). In the first two cases, the spectrum of the aged solution contains fewer, better separated signals at m/z values above those attributed to the H-bonded dimers than in the starting solution. In the aged R-phenylglycine sample, for example, two such signals are perceptible at m/z 413 and 582 (Fig. 5b). The mass values suggest that all these signals might originate, e.g., from the fragmented tetrapeptide. The analogous signals found in the aged rac-phenylglycine sample appear at m/z 369, 413, and 542 (Fig. 6b) and hence an analogous conclusion as to a possible tetrapeptide origin can be drawn.

We also monitored the aging process with R-phenylglycine and rac-phenylglycine by means of HPLC-DAD using the same techniques we applied to S-phenylglycine. In qualitative terms, the behavior of all three sets of samples was very similar. Again, we observed the two peaks (1 and 2) at retention times (tR) of 5.2 and 5.4 min, respectively, which we ascribe to pure R- and rac-phenylglycine in the two different associative forms. However, more detailed scrutiny of the respective chromatograms reveals quantitative differences that point toward a different dynamics of aging, i.e., of peptidization, in each of the three samples. A comparison of the respective chromatograms is given in Fig. 7.
Figure 7

Chromatograms of S -phenylglycine, R -phenylglycine, and rac -phenylglycine solutions in 70% aqueous ethanol registered at 275 nm; (a) each sample after seven days storage; (b) each sample after one year storage. All samples were stored at 22°C.

Figure 7a demonstrates that the intensities of peaks 1 and 2 differ among the three samples after seven days of aging. These intensities and their ratios are, respectively, 112 and 75 mAV (1.49:1), 97 and 54 mAV (1.80:1). and 81 and 29 mAV (2.79:1) for S-phenylglycine, R-phenylglycine, and rac-phenylglycine, respectively. We find that the lowest concentrations of species 1 and 2, and hence the highest peptidization rate, occur in the case of the racemic mixture. This observation is in good agreement with the results of biuret test [16] performed on three different phenylglycine samples after a storage period of a few days, which also pointed to rac-phenylglycine as the sample with the highest peptidization yields.

The chromatograms obtained after a one year storage period (Fig. 7b) present a somewhat different picture. The intensities of peaks 1 and 2 and their ratios with S-phenylglycine, R-phenylglycine, and rac-phenylglycine, respectively, are now 65 and 11 mAV (ratio 5.91), 155 and 50 mAV (3.10), and 169 and 19 mAV (8.63). Clearly, the long term dynamics differ from what was observed after seven days. To highlight the differences in the long term peptidization process with the three samples, in Fig. 8 we expand the chromatograms shown in Fig. 7b in the 6-12 min retention time range.
Figure 8

Chromatograms of S -phenylglycine, R -phenylglycine, and rac -phenylglycine solutions in 70% aqueous ethanol at 275 nm.

Figure 8 demonstrates that after one year higher molecular weight products, presumably oligopeptides, which cannot be detected during the short term storage period, appear. The peak numbering corresponds to that used in Fig. 2, but we now see the additional aging products numbered 6 to 9. Each one year old sample yields different amounts of the respective products, and in the aged R-phenylglycine sample peaks 4 and 5 are no longer visible.

Since a major focus of this study is on establishing whether the peptidization process is monotonic or oscillatory, we used the HPLC data to follow the concentrations of the various species originating from R-phenylglycine and rac-phenylglycine in time. The results for peak heights 1-5, which should be roughly proportional to the concentrations of the corresponding species are shown for R-phenylglycine and rac-phenylglycine in Figs. 9 and 10, respectively. Although the long times between measurements make it difficult to obtain a characteristic frequency of oscillation, it is clear that the behavior is not monotonic.
Figure 9

Chromatographic peak heights for (a) peaks 1 and 2, and (b) peaks 3-5 for an R -phenylglycine solution stored at 22°C for nine days. Peak numbers as in Fig. 2. Retention times: peak 1, 5.2 min; peak 2, 5.4 min; peak 3, 5.6 min; peak 4, 6.0 min; peak 5, 6.9 min.
Figure 10

Chromatographic peak heights for (a) peaks 1 and 2, and (b) peaks 3-5 for a rac -phenylglycine solution stored at 22°C for nine days. Peak numbers as in Fig. 2. Retention times: peak 1, 5.2 min; peak 2, 5.4 min; peak 3, 5.6 min; peak 4, 6.0 min; peak 5, 6.9 min.

Theoretical Models

We present here three models derived from existing schemes in the literature that capture the key features of the processes studied here: chiral conversion and condensation occurring in an oscillatory fashion.

Model 1

We wish to describe a chiral system in which association can occur. Suppose that enatiomeric monomers S and R can form dimers (S2, R2), trimers and higher oligomers (Si, Ri i = 4,...). Including all possible association and dissociation reactions generates a very complicated network, but it is possible to choose a subsystem that gives temporal oscillation. One such possibility (for an achiral system) has been proposed by Hyver [24], and we modify his scheme to include chirality.
Reaction (8) represents racemization, which is assumed to be first order and slow with respect to the other reactions. This scheme contains no autocatalytic steps. The system is open by virtue of the pool of higher oligomers (X), which dissociate to create lower oligomers. This pool of oligomers need not contain equal amounts of enantiomers, so the rate constants kr and ks can be different. To take into account the condensation of monomers, we add to Hyver's scheme the additional steps
where S2', R2' and RS denote condensates of enantiomers S and R. We assume that reactions involving condensates (9) are much slower than dissociations (3-7). As Fig. 11 shows, oscillations are easily obtained in such a model.
Figure 11

(a) Simulated concentration profiles of S (solid line), S 2 (dashed line), S 4 (solid gray line) and S 8 (dashed gray line) for model (3-9) k 1 = k 2 = k 3 = k 4 = 1, k 5 = k -5 = 0.1, k 6 = 0.001, k s = 80 and k r = 40; (b) enantiomeric excess, ee = ([S] + 2[S 2 ] + 4[S 4 ] + 8[S 8 ] - [R]-2[R 2 ] - 4[R 4 ] - 8[R 8 ])/([S] + 2[S 2 ] + 4[S 4 ] + 8[S 8 ] + [R] + 2[R 2 ] + 4[R 4 ] + 8[R 8 ]). Initial conditions: [S] = 18, concentrations of other compounds equal to 6. Time and concentration units are dimensionless.

Model 2

In an alternative approach, the condensation step itself can be the source of nonlinearity. In the model shown below [25] formation of activated monomers S* and R* occurs autocatalytically (reaction 11).

This scheme is closed with respect to mass exchange, i.e., the total concentration of monomers c = [S] + [S*] + 2[S2] + 3[S3] + [R] + [R*] + 2[R2] + 3[R3] is constant.

The dimer and trimer concentrations in Fig. 12 oscillate with small amplitude. In such a system, it is likely that only oscillations in the monomer concentrations would be observable.
Figure 12

(a) Simulated concentration profiles of S (solid line), S* (dashed line), R (solid gray line) and R* (dashed gray line) for model (10-16) k 1 = 0.02048, k -1 = 8.1k 1 , k 2 = 1, k 3 = 10 -8 , k -3 = 10 -8 , k 4 = 10 -4 , k -4 = 0.2479k 4 , k 5 = 10 -8 , k 6 = 10 -8 , k 7 = k -7 = 10 -8 . Initial conditions: [S] = 0.25, [S*] = 0.5, [S2] = [S3] = 0.05, [R] = 0.7, [R*] = 0.05, [R2] = [R3] = 0.04 and [SR] = 0.

Model 3

In our final model, oscillations appear as result of coupling between enantiomers[15]. This model is especially appropriate for systems in which the condensate SR has different chemical properties than RS.

Oscillations appear in this scheme only if the rate constant for formation of heterodimers in steps (20) and (21) is greater than that for homodimers in step (18). The system is closed with respect to mass exchange: c = [R] + [S] + [R*] + [S*] + 2([R2] + [S2] + [RS] + [SR]) = const.

In the general case, RS and SR different chemically, so we have: k4 ≠ k5, k6 ≠ k7 ≠ k12 ≠ k13, k8 ≠ k9 ≠ k14 ≠ k15 and k10 ≠ k11. Damped oscillations in a closed system occur for a broad range of parameters. The dynamics contain a stationary state, which is a stable focus with a negative eigenvalue whose real part is small in magnitude. Such dynamical behavior leads to damped oscillations whose amplitude decreases slowly in time. Results of some simulations are shown in Fig. 13. Concentrations of activated forms of monomers S* and R* (not shown) are about 40 times smaller than concentrations of other species. Generally, activated forms can be detected only in situ because they exist only in the reacting mixture.
Figure 13

(a) Simulated concentration profiles of S (solid line), R (dashed line) (a); S 2 (solid line) R 2 (dashed line) (b); and RS (solid line) and SR (dashed line) (c); for model (17-27). Enantiomeric excess ee = ([R] - [S] + [R*] - [S*] + 2[R2] - 2[S2])/c for c = 2, k1 = k2 = k3 = k6 = k7 = 1, k-1 = k8 = k9 = k10 = k11 = 0.1 and k4 = k5 = 100. Initial conditions: [S] = 1.9, [R] = 0.1 and concentrations of other compounds equal to zero.


The experimental results presented here demonstrate that phenylglycine, which exists largely in the form of hydrogen-bonded dimers, can undergo a condensation reaction in ethanol-water solution to produce higher oligomers. The reaction occurs in a nonmonotonic fashion and is apparently linked with the oscillatory chiral conversion of amino acids reported previously [46]. The S- and R- enantiomers appear to differ somewhat in their dynamics, a phenomenon that may arise from the presence of different amounts of trace impurities in the commercial samples. Our observations also suggest that there are two different dimeric aggregates, with one being more reactive with respect to peptidization than the other.

We have briefly presented three approaches to modeling such systems, and in particular to obtaining oscillatory behavior in oligomer populations and enantiomeric excesses. More sophisticated models will need to integrate the various aspects of these processes more seamlessly, but until more detailed kinetic data and rate parameters are available, it seems unwise to attempt to build more specific models.

The phenomena we have described may be of considerable importance in processes of chemical self-organization and evolution. While the results and models presented here are relatively crude, they should lay the groundwork for further studies of these fascinating systems.



M.G. and D.K. were partially supported by PhD scholarships within the framework of the "University as a Partner of the Economy Based on Science" (UPGOW) project, subsidized by the European Social Fund (EFS) of the European Union. I.R.E. was supported by the U.S. National Science Foundation grant CHE-0615507.

Authors’ Affiliations

Institute of Chemistry, University of Silesia
Chemistry Department, MS 015, Brandeis University
Institute of Physical Chemistry, Polish Academy of Sciences


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