The Impact of Pyroglutamate: Sulfolobus acidocaldarius Has a Growth Advantage over Saccharolobus solfataricus in Glutamate-Containing Media
Microorganisms are well adapted to their habitat but are partially sensitive to toxic metabolites or abiotic compounds secreted by other organisms or chemically formed under the respective environmental conditions. Thermoacidophiles are challenged by pyroglutamate, a lactam that is spontaneously formed by cyclization of glutamate under aerobic thermoacidophilic conditions. It is known that growth of the thermoacidophilic crenarchaeon Saccharolobus solfataricus (formerly Sulfolobus solfataricus) is completely inhibited by pyroglutamate. In the present study, we investigated the effect of pyroglutamate on the growth of S. solfataricus and the closely related crenarchaeon Sulfolobus acidocaldarius. In contrast to S. solfataricus, S. acidocaldarius was successfully cultivated with pyroglutamate as a sole carbon source. Bioinformatical analyses showed that both members of the Sulfolobaceae have at least one candidate for a 5-oxoprolinase, which catalyses the ATP-dependent conversion of pyroglutamate to glutamate. In S. solfataricus, we observed the intracellular accumulation of pyroglutamate and crude cell extract assays showed a less effective degradation of pyroglutamate. Apparently, S. acidocaldarius seems to be less versatile regarding carbohydrates and prefers peptidolytic growth compared to S. solfataricus. Concludingly, S. acidocaldarius exhibits a more efficient utilization of pyroglutamate and is not inhibited by this compound, making it a better candidate for applications with glutamate-containing media at high temperatures.
Thermoacidophilic organisms are of high interest for biotechnology since the extreme culture conditions offer new possibilities for many different applications. Examples of such thermoacidophilic organisms are found within the Sulfolobaceae  growing aerobically on different kinds of carbon sources including tryptone and casamino acids  at pH 2-3 and temperatures around 75-80°C. However, most thermoacidophiles are restricted by very low biomass yields , prohibiting an efficient production of added-value products. One of the reasons is the accumulation of potentially growth-inhibiting ionic compounds of low molecular weight, which was observed during fermenter-based cultivation with Saccharolobus solfataricus . One of these compounds has been identified as pyroglutamate, which is spontaneously formed from glutamate and glutamine under high temperature and at low pH [4, 5].
So far, not much is known about the effect of pyroglutamate, neither on eukaryotes nor on prokaryotes. Humans with glutathione synthetase deficiency, leading to pyroglutamate accumulation in blood plasma (pyroglutamic acidemia) and urine (pyroglutamic aciduria), develop chronic metabolic acidosis . Yang and colleagues showed that pyroglutamate, produced from lactic acid bacterial strains, has antimicrobial properties against the investigated gram-negative bacterial strains . Already a pyroglutamate concentration of 0.3% () inhibited growth of some Pseudomonas and Enterobacter strains. Since a stronger inhibitory effect was detectable in liquid media than on agar plates, Yang and colleagues predicted that the antimicrobial effect depends on the undissociated form, which passes the membrane and partially destroys the proton gradient. Pyroglutamate also inhibits the growth of S. solfataricus and other thermoacidophiles, e.g., Metallosphaera sedula and Thermoplasma acidophilum [4, 8]. Park and colleagues showed that supplementation of pyroglutamate in glutamate-containing medium decreases the growth rate of S. solfataricus in a concentration range of 3.3-15.5 mM. The growth was decreased by 50% at a concentration of 12.1 mM and was completely abolished at a concentration of 15.5 mM pyroglutamate .
It is noteworthy that some hydrolysed proteins used as nutrients in microbial cultures such as casein hydrolysate, and yeast extract , contain glutamate as the main amino acid. Biotechnological processes often include complex media containing hydrolysed proteins. These proteins are obtained from animal-derived food waste such as skin or offal and play an important role as cheap carbon sources in biotechnology . Thermophilic organisms are often cultivated in media supplemented with amino acids as carbon sources [3, 10, 11]. However, glutamate is spontaneously converted into pyroglutamate in a pH range of 2 to 3.5 and at temperatures above room temperature [8, 12]. This makes many thermoacidophiles, like, for example, S. solfataricus, less suitable for a number of biotechnological approaches due to pyroglutamate-induced growth restriction.
In this study, growth behaviour of two closely related crenarchaea—S. acidocaldarius and S. solfataricus—on glutamate and pyroglutamate as a sole carbon source was examined. While S. acidocaldarius can utilize pyroglutamate even at high concentrations, S. solfataricus was inhibited by higher pyroglutamate concentrations even in the presence of other suitable carbon sources. During growth on glutamate and pyroglutamate, S. solfataricus exhibited less efficient pyroglutamate metabolization compared to S. acidocaldarius. Thus, pyroglutamate is less suitable as a carbon source for S. solfataricus since it accumulates inside the cell and inhibits growth at elevated concentrations.
2. Materials and Methods
2.1. Strain and Growth Conditions
Sulfolobus acidocaldarius MW001  and Saccharolobus solfataricus P2 [14, 15] were aerobically grown in Brock medium  at a pH of 3. The medium of S. acidocaldarius MW001 was supplemented with 20 μg/mL uracil. The growth cultures were supplemented by either 24 mM L-glutamate or 24 mM L-pyroglutamate. Both strains were adapted to growth on glutamate starting from a culture grown with casein hydrolysate in a single adaption cycle (5 days). The adaptation to pyroglutamate was performed using glutamate-adapted cells in two cycles (14 days and 4 days). Glycerol stocks of the adapted cells were used for all following experiments.
Four independent cultures were carried out for each condition. The cultures were inoculated (initial OD600: 0.05-0.06) with a preculture that was inoculated with an adapted glycerol stock of the same carbon source and were incubated in long neck flasks (500 mL flasks, medium volume 100 mL) at 75°C and 160 rpm (Thermotron, Infors AG, Switzerland). During growth, pH was regulated with 0.5 M H2SO4. Growth of cells was monitored by measuring optical density at 600 nm (OD600).
2.2. Quantification of Intracellular and Extracellular Amino Acid Concentration
To determine extracellular concentrations of amino acids, supernatant samples were taken in regular intervals during growth and centrifuged (20,000 ×g, 5 min, RT).
To determine intracellular concentration of amino acids, a culture volume corresponding to 2 mg cell dry weight was harvested at each timepoint by centrifugation (12,000 ×g, 5 min, 4°C). The used OD-biomass correlation was calculated for each carbon source individually. Cell lysis and preparation were performed as described previously  with minor modifications: cell pellet was resuspended in 5 mL 0.9% NaCl () and washed twice, metabolite extraction was performed with 1/3 volume of methanol (omitting ribitol), deionized water, and chloroform, the polar phase was dried overnight with rotation, and the dried samples were resuspended in 100 μL deionized water. Ammonium was removed from the samples as described previously .
Pyroglutamate was analysed after its conversion back to glutamate as described by Macpherson and Slater  with slight modifications. 30 μL of the ammonium-free sample was dried with rotation and resolved in 100 μL 6 M HCl followed by an incubation for at least 1.5 h at 95°C and a neutralization step. Afterwards, the sample was dried with rotation and resolved in 30 μL deionized water.
Samples were analysed by HPLC-FLD as described previously  with some modifications to focus on glutamate detection: the mobile phase A was changed to 25 mM sodium acetate (pH 6.5) and the gradient was altered for phase B to 3% for 5.3 min, 3-4% within 0.05 min, 4-7% within 4.65 min, 7-15% within 2 min, 15% for 6 min, 15-25% within 0.5 min, 25% for 1 min, 25-30% within 0.5 min, 30-100% within 1 min, and 100% for 2 min.
The pyroglutamate content was calculated as follows: the glutamate content in the sample without conversion was deducted from the glutamate content in the sample after conversion. The resulting concentration corresponds to the pyroglutamate content. The method was confirmed by measuring known concentrations of pyroglutamate and showed a quantitative conversion to glutamate (Figure S1a–b).
2.3. Monitoring of Pyroglutamate Conversion in Crude Cell Extract
Just before the cultures reached maximal optical density, a culture volume corresponding to 10 mg cell dry weight was harvested by centrifugation (12,000 ×g, 5 min, 4°C) and resuspended in 500 μL 10 mM HEPES buffer (pH 6.5). Cells were disrupted by sonication thrice with 1 min pulse and 2 min of cooling. Cell debris was removed by centrifugation, and the supernatant was used as crude cell extract. 100 μL of crude cell extract was heated at 65°C for 24 h in 10 mM HEPES buffer containing 2.2 mM L-pyroglutamate and 1 mM MgCl2 supplemented with or without 14 mM ATP (pH 6.5) (total volume of 1 mL). As control, 2.2 mM L-pyroglutamate and 14 mM ATP were heated at 65°C for 24 h in 10 mM HEPES buffer supplemented with 1 mM MgCl2 (pH 6.5). After heating, proteins were precipitated by chloroform and removed by centrifugation (20,000 ×g, 5 min, 4°C), and the supernatant was analysed for glutamate and pyroglutamate content. Protein concentration of the crude cell extract was determined using the Bicinchoninic acid Protein Assay Kit (Sigma-Aldrich, Germany) following the manufacturer’s instructions. Enzymatic activity was calculated based on the difference between the initial pyroglutamate concentration (added pyroglutamate and pyroglutamate of the cell crude extract (CE control)) and the pyroglutamate concentration after 24 h of incubation (CE –/+ ATP) and correlated to a control without cell crude extract (Glp control) and to the protein content of cell crude extract. Quantification of ATP was done using the BacTiter-Glo™ Microbial Cell Viability Assay from Promega (Madison, WI, USA).
2.4. Computational Analysis of 5-Oxoprolinase Candidates in S. acidocaldarius and S. solfataricus
The protein sequences of all 5-oxoprolinase candidates were identified using BLASTp  with the protein sequence of the OXP1 gene of Arabidopsis thaliana (UniProt: Q9FIZ7) . The sequences of experimentally verified 5-oxoprolinases were obtained from the UniProt database , and all sequences were aligned by using Clustal Omega . The genomic context of gene candidates was analysed using the Microbial Genomic Context Viewer .
3. Results and Discussion
3.1. Sulfolobus acidocaldarius Exhibits Faster Growth on Glutamate and Uses Pyroglutamate as a Sole Carbon Source
In the direct comparison of their growth behaviour, S. acidocaldarius grew faster and reached a higher maximum cell dry weight than S. solfataricus under the same cultivation conditions on glutamate (Figure 1(a); Table 1). Both strains entered the exponential growth phase and the stationary phase at a similar time after inoculation. S. solfataricus showed a reduced maximal growth rate and a lower biomass-related substrate uptake rate compared to S. acidocaldarius (Table 1). When the cultures reached the stationary phase, the medium contained 1-2 mM glutamate, which was then completely consumed during the stationary phase (Figure 1(b)).
Glutamate is not stable at 75°C and pH 3 , leading to pyroglutamate formation (Figure 1(b)) with a reaction rate constant of 0.0066 h-1. Therefore, during the cultivation of Sulfolobaceae on glutamate, formation of pyroglutamate in the medium was observed. As pyroglutamate was stable under the chosen cultivation conditions (Figure S1b), the decreasing content was the result of consumption. The highest detected concentration of pyroglutamate was almost identical in both cultures, approximately 6.5 mM at 48 h (Figure 1(b)). Afterwards, the pyroglutamate concentration decreased in both culture supernatants. After 48 h, a continuous decrease of glutamate and pyroglutamate was detectable in the supernatant of S. acidocaldarius without growth restriction. At the beginning of coutilization, 46% of the initial glutamate concentration was still detectable in supernatant. In the culture of S. solfataricus, a continuous pyroglutamate decline was observed after 75 h in the presence of 20% of the initial glutamate concentration. This uptake of pyroglutamate led to no further growth increase. At the end of cultivation, pyroglutamate was almost completely taken up by S. acidocaldarius whereas approximately 4 mM pyroglutamate was still detectable in the growth medium of S. solfataricus. Combining maximum cell dry weight and residual substrate at ODmax, both organisms showed a similar yield coefficient (Table 1) at ODmax.
S. solfataricus did not grow at all on 24 mM pyroglutamate as a sole carbon source and in the presence of 14 mM pyroglutamate, neither as supplement nor after addition to a growing culture (Figure 2(b)). S. acidocaldarius was able to grow on 24 mM pyroglutamate (Figure 2(a)), reaching a maximum cell dry weight of 0.64 g L-1 and a maximum growth rate of 0.055 h-1 within 96 h of cultivation (Table 1). S. acidocaldarius grew slower on pyroglutamate compared to glutamate (Figure 2(a)), but the maximum cell dry weight, maximal substrate uptake rate, and yield coefficient were similar (Table 1).
As stated earlier, we observed a growth-inhibiting effect of pyroglutamate in cultures with S. solfataricus (Figure 2(b)). This effect has been previously reported in other studies [4, 8]. Furthermore, we confirmed that the growth-inhibiting effect of pyroglutamate in our experimental set-up is not only due to the loss of available carbon, because its addition to a growing culture can lead to cell death. However, Park and colleagues  proposed that pyroglutamate is a competitive inhibitor for glutamate transport in S. solfataricus. In contrast, our results show a complete glutamate uptake even in the presence of elevated pyroglutamate concentration which implies that glutamate uptake is rather independent of pyroglutamate occurrence. Moreover, the structures of the two metabolites are very different, thus, we assume that both metabolites may be taken up by different transport systems. For bacteria, it was proposed that pyroglutamate may also passively diffuse through the membrane  which may especially occur under acidic cultivation conditions.
3.2. Computational Analysis Revealed That Both Sulfolobaceae Have at Least One Promising Candidate for Pyroglutamate Degrading Enzymes
To investigate the pyroglutamate degradation capability of both species, we decided to perform a computational analysis of enzyme candidates. The only enzyme found in BRENDA  to degrade pyroglutamate was a 5-oxoprolinase (EC 126.96.36.199). This enzyme catalyses the ATP-dependent hydrolysis of pyroglutamate to glutamate. We chose the protein sequence belonging to the OXP1 gene from Arabidopsis thaliana as reference because it is the best studied eukaryotic 5-oxoprolinase . We performed a BLAST search to identify gene candidates in S. acidocaldarius and S. solfataricus. The six identified candidates were Saci_0368, Saci_0369 in S. acidocaldarius, and SSO2008, SSO2010, SSO2934, and SSO2936 in S. solfataricus. The length of each protein and all sequence identities are shown in Table 2.
A closer look at the genomic context  revealed that all genes occurred as gene pairs, coding for two subunits of the protein (Figure S2). A multiple sequence alignment with 5-oxoprolinases from all three domains of life showed that the candidates from Sulfolobaceae show high homology to eukaryotic 5-oxoprolinases, with sequence identities between 29 and 40%. We found no satisfying homology to any candidate from Bacteria (maximum 18% sequence identity). However, the 5-oxoprolinases from Eukaryota and Bacteria are encoded by one and three genes, respectively. Contrastingly, the predicted 5-oxoprolinases in Sulfolobaceae are encoded by two genes that are in direct genomic context (Figure S3). All seven archaeal 5-oxoprolinases in Swiss-Prot  belong to the members of the Euryarchaeota. They show high sequence identities with Sulfolobaceae candidates between 49 and 54%. The gene candidates SSO2008 and SSO2010 show the highest homology to the 5-oxoprolinase of Methanocaldococcus jannaschii (Table 2). Additionally, they consist of two subunits as well. Only members of the family Methanosarcinaceae have 5-oxoprolinases that are coded by a single gene. Unfortunately, no crystal structure for any of the 5-oxoprolinases is known; thus, no comparison of the substrate-binding sites was possible.
In summary, we predict that S. acidocaldarius has a functional 5-oxoprolinase, consisting of two subunits, and S. solfataricus has two copies of this enzyme. Moreover, the 5-oxoprolinase candidates from Sulfolobaceae are more homologous to eukaryotes than to bacteria.
For further investigation of the predicted 5-oxoprolinases, we looked at differences in transcription of the gene candidates that could explain the observed phenotypes. Therefore, we analysed published transcriptome data of both members of the Sulfolobaceae on different substrates [26–29]. The relative expression levels compared to the median of the whole transcriptome were compared to the presence of glutamate (and accordingly pyroglutamate) in the medium and is shown in Table 3. Although the culture conditions and medium composition differed among the studies, we found a noticeable correlation between the presence of glutamate in the medium and an enhanced expression (up to 5-fold) of the 5-oxoprolinase candidates in S. acidocaldarius [27–29]. Contrastingly, the expression of all gene candidates in S. solfataricus was remarkably low and did not increase when glutamate was present in the medium .
3.3. Saccharolobus solfataricus Accumulates High Levels of Pyroglutamate and Shows Lower 5-Oxoprolinase Activity
As the growth behaviour showed a strong difference with respect to the usage of the formed pyroglutamate in the later growth state, we further investigated whether both strains metabolise the incorporated pyroglutamate. Therefore, intracellular pyroglutamate and glutamate concentrations during stationary phase were determined.
We observed a large difference in the intracellular content of glutamate and pyroglutamate at the end of cultivation (Figure 3). In S. acidocaldarius, both amino acids are present in low levels (less than 1 μg mg-1 cell dry weight) whereas the intracellular concentration of glutamate was 10-fold higher and the concentration of pyroglutamate was 17-fold higher in S. solfataricus. The intracellular content of pyroglutamate decreased from 72 h to 120 h in both cultures, whereas an accumulation occurred at 144 h. We predict that the cells reached the end of the stationary phase associated with ceased metabolic processes leading to accumulation.
Regarding the differences in intracellular pyroglutamate content, we performed crude cell extract assays to examine differences in the enzymatic activity based on pyroglutamate consumption. Additionally, we detected the formation of glutamate in this assay (Table S1). However, a quantitative evaluation of glutamate production is hampered by a possible further conversion of glutamate by other enzymes in the crude cell extract.
We detected 5-oxoprolinase activity in crude cell extracts of both strains (Figure 4). The enzymatic activity was strongly enhanced in the presence of ATP and was 1.7-fold higher in the crude cell extract of S. acidocaldarius compared to S. solfataricus. A control without cell crude extracts did not show a spontaneous degradation of pyroglutamate in the presence of ATP (Table S1).
In summary, in the cells of S. acidocaldarius, glutamate and pyroglutamate were both detected in substantially lower concentrations than in S. solfataricus, indicating a rapid conversion of the carbon source for metabolic processes. The data suggest that pyroglutamate is a higher burden for S. solfataricus than for S. acidocaldarius since it accumulates in the cells to more than 0.7% () of the cell dry weight. Taken into account that microorganisms typically contain approximately 3% () low molecular weight metabolites , this indicates a strong accumulation. We see a cooccurrence of enhanced intracellular pyroglutamate levels and growth inhibition in S. solfataricus. In this context, the previously stated role of pyroglutamate as a classical protonophore with cycles of passive uptake in the protonated and an active export in the deprotonated form with a comparable low intracellular concentration [4, 8] is not supported by our data. We showed a strong intracellular accumulation in S. solfataricus indicating an active energy-demanding import without subsequent energy-producing catabolic reactions. Inside the cell, the accumulation of an acid may lead to severe alterations of the metabolism, e.g., by decreased protein stability or inhibitory effects, and may serve as an explanation for the toxic effect. Finally, performed crude cell extract assays revealed a more effective conversion of pyroglutamate in S. acidocaldarius. Therefore, S. acidocaldarius took advantage of using pyroglutamate as a carbon source for anabolic processes and respiration.
In this study, we examined the effect of pyroglutamate on the thermoacidophilic crenarchaea Sulfolobus acidocaldarius and Saccharolobus solfataricus. During glutamate cultivation, we observed spontaneous pyroglutamate formation from glutamate and improved growth of S. acidocaldarius. Analysis of intracellular glutamate and pyroglutamate concentrations shows that S. solfataricus accumulates much higher levels of both amino acids in the cytoplasm upon reaching the steady state, while the levels in S. acidocaldarius remain low. A computational analysis of several gene candidates revealed that both strains contain gene candidates for 5-oxoprolinases capable of degrading pyroglutamate, but we detected a lower 5-oxoprolinase activity in crude cell extracts of S. solfataricus. Our data imply that pyroglutamate is a higher burden for S. solfataricus, because it leads to complete growth inhibition at higher concentrations. This is further supported by the fact that only S. acidocaldarius grew on pyroglutamate as a sole carbon source.
To our knowledge, the growth of thermoacidophilic archaea on pyroglutamate as a sole carbon source has not been reported before. This ability of S. acidocaldarius makes it into a highly suitable candidate for high temperature biotechnological applications, including the degradation of glutamate-rich media without any negative effect of spontaneously formed pyroglutamate.
The data used to support the findings of this study are included within the article and the supplementary information files.
Conflicts of Interest
The authors declare that there are no conflicts of interest regarding the publication of this paper.
Anna M. Vetter and Julia Helmecke contributed equally to this work.
We thank Sabine Kaltenhäuser for excellent technical assistance. This work was funded within the e:Bio initiative, HotSysAPP (031L0078E).
Figure S1: evaluation of pyroglutamate measurement procedure. (a) Conformity of appointed and measured pyroglutamate concentrations. Pyroglutamate content in supernatant at a timepoint 0 h and 24 h of the S. acidocaldarius growth curve supplemented with 24 mM pyroglutamate (see Figure 2(a)). (b) Pyroglutamate stability at thermoacidophilic conditions. 22 mM pyroglutamate was cultivated in Brock Medium at 75°C and pH 3 for 144 h. Values represent the average of four independent cultivations, and error bars represent the standard error. Figure S2: genomic context of all 5-oxoprolinase candidates from Sulfolobus acidocaldarius and Saccharolobus solfataricus. This figure was created using the Microbial Genomic Context Viewer. Figure S3: fingerprint of the multiple sequence alignment of 5-oxoprolinases from all three domains of life. Blue sequence names indicate the 5-oxoprolinase candidates from Sulfolobus acidocaldarius and Saccharolobus solfataricus. Light grey shadings indicate the nonconserved regions, blue shading shows over 30% conservation, and red shading indicates similar regions. Organisms: BACSU = Bacillus subtilis 168, ECOLI = Escherichia coli K12, METJA = Methanocaldococcus jannaschii JAL-1, SULAC = Sulfolobus acidocaldarius DSM 639, SULSO = Saccharolobus solfataricus P2, METBF = Methanosarcina barkeri DSM 804, ARATH = Arabidopsis thaliana, and HUMAN = Homo sapiens. Table S1: content of glutamate and pyroglutamate in crude cell extract assay of Sulfolobus acidocaldarius and Saccharolobus solfataricus. Crude cell extracts (CE) of S. acidocaldarius MW001 (Saci) and S. solfataricus P2 (Sso) were incubated with 2.2 mM L-pyroglutamate (Glp) in presence and absence of 14 mM ATP (+ATP/-ATP) at 65°C for 24 h. Afterwards, glutamate (Glu) and pyroglutamate content were determined. Values represent the average of four independent cultivations. Errors represent the standard error between the four experiments. (Supplementary Materials)
C. B. Park, S. U. N. B. O. K. Lee, and D. D. Y. Ryu, “L-Pyroglutamate spontaneously formed from L-glutamate inhibits growth of the hyperthermophilic archaeon Sulfolobus solfataricus,” Applied and Environmental Microbiology, vol. 67, no. 8, pp. 3650–3654, 2001.View at: Publisher Site | Google Scholar
A. Kumar and A. K. Bachhawat, “Pyroglutamic acid: throwing light on a lightly studied metabolite,” Current Science, vol. 102, 2012.View at: Google Scholar
M. H. Creer, B. W. Lau, J. D. Jones, and K. M. Chan, “Pyroglutamic acidemia in an adult patient,” Clinical Chemistry, vol. 35, no. 4, pp. 684–686, 1989.View at: Google Scholar
H. J. Chae, H. Joo, and M. J. In, “Utilization of brewer’s yeast cells for the production of food-grade yeast extract. Part 1: effects of different enzymatic treatments on solid and protein recovery and flavor characteristics,” Bioresource Technology, vol. 76, no. 3, pp. 253–258, 2001.View at: Publisher Site | Google Scholar
D. G. G. Hatzinikolaou, E. Kalogeris, P. Christakopoulos, D. Kekos, B. J. J. Macris, and Z. Campus, “Comparative growth studies of the extreme thermophile Sulfolobus acidocaldarius in submerged and solidified substrate cultures,” World Journal of Microbiology and Biotechnology, vol. 17, no. 3, pp. 229–234, 2001.View at: Publisher Site | Google Scholar
H. D. Sakai and N. Kurosawa, “Saccharolobus caldissimus gen. nov., sp. nov., a facultatively anaerobic iron-reducing hyperthermophilic archaeon isolated from an acidic terrestrial hot spring, and reclassification of Sulfolobus solfataricus as Saccharolobus solfataricus comb. nov. and Sulfolobus shibatae as Saccharolobus shibatae comb. nov,” International Journal of Systematic and Evolutionary Microbiology, vol. 68, no. 4, pp. 1271–1278, 2018.View at: Publisher Site | Google Scholar
F. Sievers and D. G. Higgins, “Clustal Omega, accurate alignment of very large numbers of sequences,” in Multiple Sequence Alignment Methods, D. Russell, Ed., vol. 1079 of Methods in Molecular Biology (Methods and Protocols), pp. 105–116, Humana Press, Totowa, NJ, USA, 2014.View at: Publisher Site | Google Scholar
F. C. Neidhardt, J. L. Ingraham, and M. Schaechter, Physiology of the Bacterial Cell: A Molecular Approach, Sinauer Associates Inc, 1990.