- Research article
- Open Access
Characterization of LrgAB as a stationary phase-specific pyruvate uptake system in Streptococcus mutans
BMC Microbiology volume 19, Article number: 223 (2019)
Our recent ‘-omics’ comparisons of Streptococcus mutans wild-type and lrgAB-mutant revealed that this organism undergoes dynamic cellular changes in the face of multiple exogenous stresses, consequently affecting its comprehensive virulence traits. In this current study, we further demonstrate that LrgAB functions as a S. mutans pyruvate uptake system.
S. mutans excretes pyruvate during growth as an overflow metabolite, and appears to uptake this excreted pyruvate via LrgAB once the primary carbon source is exhausted. This utilization of excreted pyruvate was tightly regulated by glucose levels and stationary growth phase lrgAB induction. The degree of lrgAB induction was reduced by high extracellular levels of pyruvate, suggesting that lrgAB induction is subject to negative feedback regulation, likely through the LytST TCS, which is required for expression of lrgAB. Stationary phase lrgAB induction was efficiently inhibited by low concentrations of 3FP, a toxic pyruvate analogue, without affecting cell growth, suggesting that accumulated pyruvate is sensed either directly or indirectly by LytS, subsequently triggering lrgAB expression. S. mutans growth was inhibited by high concentrations of 3FP, implying that pyruvate uptake is necessary for S. mutans exponential phase growth and occurs in a Lrg-independent manner. Finally, we found that stationary phase lrgAB induction is modulated by hydrogen peroxide (H2O2) and by co-cultivation with H2O2-producing S. gordonii.
Pyruvate may provide S. mutans with an alternative carbon source under limited growth conditions, as well as serving as a buffer against exogenous oxidative stress. Given the hypothesized role of LrgAB in cell death and lysis, these data also provide an important basis for how these processes are functionally and mechanically connected to key metabolic pathways such as pyruvate metabolism.
Development of a mature biofilm on the tooth surface is the central event in the pathogenesis of dental caries . This process primarily requires that cariogenic organisms, including Streptococcus mutans, withstand the limited resources or environmental fluctuations experienced in the oral cavity [2, 3]. An emerging concept for biofilm maturation is that the survival and persistence of these organisms during biofilm development may be mediated by regulated cell death and lysis processes, consequently eliminating bacterial cells damaged by adverse environments and benefiting the rest of the population within the biofilm [4, 5]. Toward this end, we have studied the S. mutans Cid/Lrg system, consisting of two dicistronic operons lrgAB (SMU.575c/574c) and cidAB (SMU.1701c/1700c) [6,7,8,9,10,11]. These operons are currently annotated as encoding holin- and antiholin-like proteins. The primary basis for these annotations came from the predicted structural similarities between CidA/LrgA and the bacteriophage-encoded holin family of proteins [4,5,6]. Bacteriophage holins are small membrane proteins, regulating the timing and lysis of the host cell during lytic infection with inhibitor holins (antiholins) . Further support was provided by previously-observed phenotypes of Staphylococcus aureus cid and lrg mutants [13,14,15,16]. Notably, in S. mutans, the Cid/Lrg system is also involved in comprehensive virulence traits, including antibiotic resistance, autolysis, biofilm development, genetic competence, oxidative and heat stress responses [6, 7, 9, 11], all of which are essential for successful colonization and persistence in the oral cavity. Nevertheless, the molecular details of how Cid and Lrg function to control cell death and lysis have not yet been completely elucidated in S. mutans and S. aureus. Direct evidence of their specific cellular functionality is still scarce.
A hallmark finding for the S. mutans Cid/Lrg system is that expression levels of lrg and cid are counterbalanced throughout the growth cycle and in response to the availability of oxygen and glucose [6, 8]. In fact, the lrg and cid operons were originally identified to be up- and down-regulated, respectively, in aerobically grown cells . The response of lrg and cid to glucose levels is particularly remarkable. The lrg genes are highly induced in cultures containing lower levels of glucose (≤ 15 mM) but almost completely repressed in cultures containing glucose at concentrations of 20 mM and higher . In contrast, cid expression is negligible when cells are cultured in the presence of lower glucose concentrations (≤20 mM) but increases at higher glucose concentrations (> 20 mM) . Our recent study further demonstrated that CcpA is a direct regulator of expression of cid and lrg , and lrgAB expression is also governed by the LytST two-component regulatory system (TCS), located immediately upstream of the lrgAB genes [6, 8]. These data suggest a functional linkage between the Cid/Lrg system and metabolic pathways. This idea was also reinforced by our recent omics studies of S. mutans wild-type and isogenic ΔlrgAB mutant strains, using RNA-seq and label-free quantitative mass spectrometry, showing that a large number of genes and/or proteins involved in carbohydrate metabolism, ABC transporters, and oxidative stress adaptation were significantly altered in the lrgAB mutant under stress inducing culture conditions (aerobic, heat and vancomycin treatment) [7, 11].
The fact that the lrgAB promoter is highly active only in cells entering stationary phase, but not in cells growing exponentially, in the low-glucose condition , implies that LrgAB may be important for survival of cells when exogenous carbohydrate has been depleted. This lrgAB induction pattern was also shown in our previous microarray data, comparing RNA expression profiles of wild-type and lytS-deficient strains between early- and late-exponential growth phases in BHI medium . When this expression data was reconstituted for comparison of early- vs. late-exponential growth phases in the wild type, it was shown that lrgAB (SMU.575c-574c) was dramatically upregulated (about > 900-fold) at late-exponential phase, compared to early-exponential growth phase . A four-gene operon (SMU.1421 to SMU.1424), encoding the components of the pyruvate dehydrogenase complex (PDH), was also remarkably upregulated (by > 284-fold) at late-exponential phase, compared to that of early-exponential phase , suggesting that LrgAB may be related to pyruvate metabolism. Coincidentally, PftAB (YsbAB), homologous to LrgAB, was recently reported to function as a pyruvate transporter in Bacillus subtilis [18, 19]. Similarly to the observations for the lrgAB genes in S. mutans [6, 9], expression of the ysbAB genes was regulated by LytSR/LytST, located upstream of ysbAB, as well as by CcpA [20, 21]. Expression of ysbAB was also maximal at stationary phase of growth [18, 19] and was reduced by glucose addition [20, 21]. Esherichia coli also has two TCS (BtsSR and YpdAB) homologous to LytST that have been shown to regulate expression of pyruvate transporters in response to extracellular pyruvate [22,23,24]. Interestingly, these TCS and BtsT (high-affinity pyruvate transporter regulated by BtsSR and YpdAB) have also been recently implicated in the ability of pyruvate to rescue E. coli from the viable but non-culturable (VBNC) state . Collectively these studies, combined with the functional and genetic similarities of LrgAB to YsbAB in B. subtilis, suggest that LrgAB may also function as a pyruvate transporter in S. mutans.
To date little is known about the role and regulation of pyruvate in S. mutans, as well as other oral streptococci. Pyruvate is the final product of glycolysis, as well as a major substrate for oxidative metabolism. Pyruvate is converted to acetyl-coenzyme (acetyl-CoA) by the Pdh complex or Pfl (pyruvate formate lyase), depending on the presence or absence of oxygen, or the limitation or excess of a preferred sugar (e.g. glucose) [25, 26]. Acetyl-CoA is subsequently converted to end-products of fermentative metabolism, such as lactate, acetate, acetoin and formate. By ultilizing these pathways, cells maintain redox balance (NAD+/NADH) and generate ATP, which promotes cell homeostasis. In this present study, we reveal that pyruvate is excreted during growth of S. mutans as an overflow metabolite, and is reimported into cells via LrgAB when the primary carbon source (i.e. glucose) becomes exhausted. We performed a series of pyruvate quantification and lrg promoter reporter assays in order to characterize the role and regulation LrgAB as a pyruvate uptake system. These experiments demonstrate that LrgAB expression and activity is tightly regulated at the transcriptional level and modulated by both external and internal metabolic conditions. We also show that due to the H2O2- scavenging activity of pyruvate, re-uptake of pyruvate by S. mutans may be influenced by interactions with H2O2-producing oral commensals, such as S. gordonii. Given the possible involvement of LrgAB in inducing cell death and lysis in a programed manner, the presented data provide a new basis for how cell death and lysis mechanisms in S. mutans may be functionally and mechanically connected to pyruvate, a metabolic signal which may modulate homeostasis and virulence of this organism.
Bacterial strains, plasmids, and growth conditions
Streptococcus mutans UA159 and its previously-constructed mutant derivatives [6, 9] were cultured in brain heart infusion (BHI) medium (Difco Laboratories, Detroit, MI) or chemically defined medium FMC  containing 11 mM (or 45 mM) glucose. The medium was supplemented by sodium pyruvate (Fisher Scientific), β-fluoropyruvic acid sodium salt monohydrate (3FP, Sigma-Aldrich), pyruvic acid (Sigma-Aldrich), carbonyl cyanide m-chlorophenyl hydrazine (CCCP, Sigma-Aldrich) and 2,4-dinitrophenol (DNP, Sigma-Aldrich) or hydrogen peroxide (H2O2, Fisher Scientific), as necessary. Antibiotics were used to supplement growth media in the following concentrations: spectinomycin (1 mg/ml), kanamycin (1 mg/ml), and erythromycin (10 μg/ml). Unless otherwise noted, cultures were grown at 37 °C in a 5% CO2, aerobic atmosphere. For aerobic growh, cultures were grown in an aerobic incubator. To achieve anaerobic conditions, sterile mineral oil was placed on top of the cultures [6, 17, 28]. For growth measurements, fresh medium was inoculated with 1 : 100 dilutions of overnight cultures of S. mutans. The optical density at 600 nm (OD 600) was measured at 37 °C at 30 min-intervals using a Bioscreen C growth curve analysis system.
Sequence analysis and alignments
Amino acid sequences for S. mutans UA159 LrgA/B (SMU.574/575c), B. subtilis 168 YsbA/B (BSU_28900/28910), S. aureus MRSA252 LrgA/B (SAR_0259/0260), S. gordonii DL1 LrgA/B (SGO_1268/1269), and E. coli K12 LrgA/B (YohJ/K, JW2129/2130) were retrieved from the National Center of Biotechnology Information (NCBI) Protein database or from Uniprot (www.uniprot.org). Alignments were then generated utilizing the T-COFFEE M-coffee protein alignment tool  with shading completed via BoxShade version 3.21 (https://embnet.vital-it.ch/software/BOX_form.html). Percent identity matrices were then produced using the same sequences using Clustal Omega .
Microplate reporter assay
GFP activities of the S. mutans strains harboring Plrg-gfp gene fusion, previously constructed , were observed using a Synergy microplate reader (BioTek) controlled by Gen5 software [10, 31, 32]. Overnight cultures were diluted 1:50 into 2 ml of FMC medium and grown to an OD600 = 0.5. At this point, these cultures were diluted 1:50 into 175 μl FMC in individual wells of a 96-well plate (black walls, clear bottoms; Corning). To evaluate the possible role of pyruvate as an antioxidant against H2O2 in the oral cavity, the reporter strain was also cultivated with Streptococcus gordonii DL1, a H2O2-producing oral commensal, at a ratio of 1:1. The optical density at 600 nm (OD600) and green fluorescence were monitored (sensitivity = 45; excitation = 485 nm; emission = 520 nm) at 30 min intervals. The fluorescence of wild-type harboring plasmid without the reporter gene fusion was subtracted from fluorescence readings of the S. mutans strains harboring Plrg-gfp gene fusion. The results are representative of at least three independent replicates, each performed in triplicate.
Measurement of extracellular pyruvate and glucose levels
S. mutans UA159 wild-type and isogenic mutants (ΔlrgAB, ΔlytS, ΔcidB, or UA159/184-cidAB) strains were grown in chemically defined FMC medium, supplemented with either 11 mM or 45 mM glucose. For time course measurements of extracellular pyruvate during growth, samples (200 μl) were taken at 1–2 h intervals and half of this volume (100 μl) was used to measure the OD600 in a spectrophotometer for monitoring growth. The other half (100 μl) was centrifuged for 2 min at 18,000 xg to remove the cells, and pyruvate and glucose concentrations of the supernatant were quantified with an EnzyChrom™ pyruvate assay kit (BioAssay Systems, Hayward, CA) or glucose (HK) assay kit (Sigma-Aldrich), respectively, according to the manufacturer’s instructions. The results are average or representative of at least two independent replicates, each performed in duplicate.
Sequence analysis of LrgA and LrgB homologues
To evaluate the possibility that S. mutans LrgAB functions as a pyruvate transporter, we performed multiple sequence alignments alongside B. subtilis YsbA and YsbB, recently reported to be putative pyruvate transporters [18, 19], as well as other LrgA and LrgB homologues from S. aureus, E. coli and S. gordonii (a non-cariogenic inhabitant of the oral cavity). In the alignment of LrgA homogues (Fig. 1a), the central portion of the proteins displayed many conserved residues while N- and C-teminal portions were quite variable. The size of the other LrgA homologues was relatively shorter than that of S. mutans LrgA. In contrast, LrgB homologues had a similar size and displayed more conserved residues throughout the sequence (Fig. 1b). We also generated percent identity matrices using the amino acid sequences of LrgA or LrgB homologues via Clustal Omega. As shown in the comparison look-up tables for LrgA (Fig. 1c) and LrgB (Fig. 1d) homologues, each pair-wise comparison displayed an identify value greater than 20%. In particular, S. mutans LrgA and LrgB proteins displayed high identify to B. subtilis YsbA (40.9%) and YsbB (30.0%), as well as to S. aureus LrgA (34.9%) and LrgB (30.0%), proposed to be involved in the regulation of cell death [4, 13,14,15]. The YsbA and YsbB proteins also displayed higher similarities (43.3 and 56.5%) to S. aureus LrgA and LrgB. It is also notable that S. mutans lytST, known to regulate lrgAB [6, 8], has a similar genomic organization to these operons in B. subtilis and S. aureus (Additional file 1: Figure S1). This conservation of genomic organization and amino acid similarities suggest that S. mutans LrgAB may function as a pyruvate transporter, as previously observed for YsbAB in B. subtilis [18, 19].
lrgAB encodes a pyruvate uptake system in S. mutans
Pyruvate is excreted as an overflow metabolite and re-consumed after other favorable carbon sources (i.e. glucose) are exhausted . Many bacterial species, including B. subtilis [18, 19] and E. coli [22, 23] are able to utilize extracellular pyruvate as a sole carbon source, but this does not appear to be the case for S. mutans, as it is not able to grow in chemically defined FMC medium containing pyruvate as the sole carbon source (Additional file 2: Figure S2). Therefore, to determine whether LrgAB is involved in pyruvate transport, we first monitored extracellular pyruvate levels throughout planktonic culture growth of wild-type and ΔlrgAB mutant strains using a pyruvate assay kit. For this, we cultivated both strains in FMC medium, containing a low level of glucose (11 mM), allowing a strong stationary phase induction of lrgAB , at 5% CO2 atmosphere. As shown in Fig. 2a, the wild-type cells excreted pyruvate into the extracellular medium in a growth-phase dependent manner until late-exponential phase, at which point extracellular pyruvate concentration reached its maximum level (≈ 400 μM). Shortly afterwards, pyruvate concentrations rapidly dropped almost to zero within a hour after the onset of stationary phase (Fig. 2a). In contrast, in the stationary phase of ΔlrgAB cultures, the level of excreted pyruvate was only slightly decreased without dramatic change (Fig. 2b), suggesting that LrgAB may be responsible for uptake and further utilization of excreted pyruvate at stationary phase. However, the lack of LrgAB could not completely block pyruvate uptake (Fig. 2b), suggesting the presence of an additional pyruvate uptake system, likely in a Lrg-independent manner, in S. mutans. It is notable that pyruvate excretion throughout growth was not abolished in the ΔlrgAB strain, indicating that LrgAB is not likely involved in pyruvate export. The maximum level (approx. 600 μM) of pyruvate excreted during growth of the ΔlrgAB strain was about 50% elevated compared to wild type, and was reached after a delay to the onset of stationary phase, suggesting that lack of LrgAB may slow down pyruvate metabolism, consequently increasing the overflow of pyruvate. This is consistent with our recent RNA-seq data, showing that many metabolic pathway-related genes, including pfl, were significantly downregulated during growth of the ΔlrgAB strain . Inhibition of stationary phase pyruvate uptake was also observed in the ΔlytS strain (Fig. 2c), indicating that the function of LrgAB as a pyruvate uptake system, is under the tight control of lytST, located immediately upstream of lrgAB [6, 8]. Given the potential interaction between lrg and cid [6, 9], we also tested whether Cid could contribute to pyruvate uptake or utilization. To test this, we quantified extracellular pyruvate during growth of ΔcidB, previously shown to have a similar transcriptomic profile and phenotypes as those observed for the ΔlrgAB mutant, particularly in response to oxidative stress [6, 9, 11]. However, the ΔcidB strain behaved like wildtype in terms of pyruvate excretion and uptake (Additional file 3: Figure S3). Even in the cultures of strains lacking (ΔcidAB) or overexpressing cidAB (UA159/184-cidAB) , no obvious difference was observed (data not shown). Thus, we concluded that the Cid proteins are not likely involved in pyruvate uptake/utilization in S. mutans, thus no further investigation was performed on the cid operon in this study.
Glucose and oxygen levels are important for stationary-phase pyruvate uptake of S. mutans
We previously described that stationary phase expression of lrgAB was dramatically repressed in cultures containing glucose at concentrations of 20 mM and higher, although still detectable at concentrations of up to 45 mM . In accordance with this observation, stationary phase pyruvate uptake was profoundly inhibited, although pyruvate was excreted at much higher levels relative to low glucose cultures (Fig. 2a), when the wild-type strain was cultivated in FMC medium containing 45 mM glucose (Fig. 3a). This inhibition by high-glucose levels was even more pronounced in the ΔlrgAB culture (Fig. 3b), compared to that observed for the low-glucose culture of this mutant (Fig. 2b). These results suggest that LrgAB activity, as a pyruvate uptake system, is strongly repressed in high-glucose cultures, a phenotype which is regulated at the transcriptional level [6, 10]. We additionally measured the concentration of extracellular glucose in the same time-course samples taken for the above pyruvate assays, and observed that most of glucose was rapidly depleted during exponential growth in both wild type and ΔlrgAB cultures, even in the glucose-excess (45 mM) condition (Additional file 4: Figure S4), suggesting that the effect of LrgAB on pyruvate uptake is not a result of altered glucose depletion. Nevetheless, pyruvate accumulation during growth was moderately reduced at stationary phase (Fig. 3a), further supporting the idea that uptake of pyruvate can also occur in a LrgAB-independent manner, because expression of lrgAB is almost completely inhibited at stationary phase .
S. mutans metabolizes a large proportion of glucose only as far as pyruvate and acetyl CoA, and their subsequent metabolism depends on the availability of oxygen, particularly when the glucose concentration is limited [26, 34, 35]. Our previous data showed that expression of lrgAB was highly upregulated in response to oxygen, and its deficiency rendered the organism super-sensitive to oxygen [6, 11, 17], suggesting that oxygen availability may influence the efficacy of LrgAB to function as a pyruvate uptake system. To test this, we quantified extracellular pyruvate in both wild type and ΔlrgAB mutant cells, cultivated aerobically or anaerobically. To achieve anaerobic conditions, sterile mineral oil was placed on top of the cultures. All cultures were incubated in an aerobic incubator. The overall extracellular pyruvate profile during growth of both wild type (Additional file 5: Figure S5A and S5C) and ΔlrgAB (Additional file 5: Figure S5B and S5D) cultures were similar between the cells, grown aerobically and anaerobically. However, we found that pyruvate was about 50% more excreted during aerobic growth (Additional file 5: Figure S5A and S5B), relative to that observed during anaerobic growth (Additional file 5: Figure S5C and S5D) in both strains, respectively. We also found that the re-uptake of excreted pyruvate was somewhat inhibited during aerobic growth in both strains, relative to anaerobic growth, suggesting that pyruvate consumption may be decelerated during aerobic growth. Overall, these results suggest that LrgAB activity may be modulated by internal and external metabolic conditions of the cell.
Characterization of lrgAB expression and pyruvate uptake in response to extracellular pyruvate
The similar regulatory trend between pyruvate uptake (Fig. 2 and 3) and lrgAB expression [6, 10] suggests that re-uptake of excreted pyruvate likely depends on the level of lrgAB expression. However, the observation that stationary phase pyruvate uptake was not triggered by glucose depletion, prompted us to test whether the level of accumulated pyruvate is the primary stimulus for lrgAB induction and subsequent pyruvate uptake. To assess the pyruvate concentration dependence of lrgAB induction, we evaluated how lrgAB reponds to different concentrations of external pyruvate during growth, using the PlrgA-gfp reporter strain from our recent study . Because growth in high levels of glucose abrogates stationary phase induction of lrgAB, the strain was cultivated under a low-glucose (11 mM) condition, and under aerobic conditions leading to higher induction. We initially added 1 mM pyruvate into the medium at the beginning of growth, because about 400–800 μM pyruvate would be excreted in the same growth condition in the absence of pyruvate (Figs. 2, Additional files 2 and 4: Figure S2, and Figure S4). We further reasoned that supplying extracellular pyruvate in excess may lead to early induction of lrgAB, which is normally induced at stationary growth phase [6, 10]. Supplementation of 1 mM exogenous pyruvate at time of inoculation elevated the lrgAB induction level by about 3-fold, but this induction still occurred at stationary growth phase (Fig. 4b). The induction level of lrgAB increased linearly with increasing concentrations of pyruvate up to 10 mM (Figs. 4b-4e). The increment was somewhat alleviated at 20 mM and further increase of supplemented pyruvate (40 and 80 mM) led to a drastic decrease of lrgAB expression (Figs. 4f-4h). These results suggest that the magnitude of stationary phase lrgAB expression is modulated by levels of extracellular pyruvate but this metabolite does not alter the timing of lrgAB expression during growth. To evaluate whether the transcriptional response of lrgAB is correlated with the capacity of the organism to take up pyruvate, we monitored the level of extracellular pyruvate during growth in a low-glucose FMC medium supplemented by additional pyruvate of 1, 5, 10 and 40 mM. When the cell was cultivated in the presence of 1 mM pyruvate, the re-uptake of pyruvate normally occurred at stationary phase (Fig. 5a). Notably, however, supplying ≥5 mM pyruvate at the time of inoculation remarkably reduced the re-uptake of extracellular pyruvate with considerable amounts of pyruvate left in the media (Figs. 5b-5d). S. mutans cells grown at pyruvate concentrations of 10 mM or lower (Figs. 5a-5c), excreted pyruvate in a growth-dependent manner until late-exponential growth phase, but the magnitude of changes in the increment was several-fold greater than that of cells cultivated in the absence of pyruvate. For example, maximum increments (reached at 4 h) of pyruvate excreted in the pyruvate supplemented cultures (~ 600 μM in Fig. 5a, ~ 2.0 mM in Fig. 5b, and ~ 4 mM in Fig. 5c) were much higher than no pyruvate cultures (~ 400 μM in Fig. 2a), suggesting that extracellular pyruvate can stimulate excretion of intracellular pyruvate. When cells were cultivated in the presence of 40 mM pyruvate, no profound change was observed in the pyruvate flux during growth and in stationary phase (Fig. 5d), which is in accordance with reduced lrgAB expression in the same culture condition (Fig. 4g). Collectively, these results suggest that extracellular pyruvate triggers expression of lrgAB, leading to re-uptake of pyruvate by LrgAB. These data also suggest that lrgAB induction can be negatively regulated by high levels of extracellular pyruvate.
The toxic pyruvate analogue 3FP interferes with the response of lrgAB to extracellular pyruvate
It is likely that the stationary phase induction of lrgAB occurs through the activation of LytS in response to pyruvate, excreted during growth, because expression of lrgAB is under tight control of LytST . Thus, to test if lrgAB is specifically induced in response to pyruvate, we cultivated the PlrgA-gfp reporter strain in low glucose media, containing non-inhibitory levels (0, 0.01, 0.1, 1 mM) of the pyruvate analog 3-fluoropyruvate (3FP), previously shown to compete with pyruvate and inhibit cell growth by binding to PDH complex in the cell [36,37,38]. As shown in Figs. 6a-6d, stationary phase induction of lrgAB was reduced in a dose-dependent manner by 3FP. Expression of lrgAB was obviously reduced in the presence of 0.01 mM 3FP (Fig. 6b), and expression was almost completely inhibited at 1 mM 3FP (Fig. 6d), likely due to 3FP outcompeting excreted pyruvate. This competition was more evident when cells were grown in the presence of pyruvate and 3FP (Additional file 6: Figure S6). This observation also indicates that the inhibitory effect of 3FPs can be diluted by the addition of an excess of pyruvate. Somewhat surprisingly, supplementation of 0.01 mM 3FP completely inhibited re-uptake of excreted pyruvate, and additional excretion was triggered at stationary growth phase (Fig. 6e). The same result was observed when cells were grown in the presence of 1 mM 3FP (Fig. 6f) but more pyruvate was excreted during growth, compared to the observation for the absence of 3FP, suggesting that part of 3FP was taken up into the cell in a Lrg-independent manner, likely affecting the normal utilization of pyruvate. This is further supported by the fact that S. mutans was unable to normally grow in the presence of 10 mM 3FP (Additional file 7: Figure S7). It seems that pyruvate is an effective overflow metabolite to induce the lytST-lrgAB circuit for pyuvate uptake, even though it may not be the only inducer of pyruvate uptake system.
High concentrations of extracellular pyruvate can delay the stationary phase, regardless of LrgAB
The measurements of lrgAB expression in the culture containing 3FP, a synthetic analogue of pyruvate, implied that pyruvate may be able to enter the cell, independently of LrgAB (Fig. 6). Increased levels of intracellular 3FP exert a negative effect on the metabolic pathways linked to the pyruvate node and eventually cell viability. We also observed prolongation of the exponential phase of growth when cells were grown in the presence of ≥40 mM pyruvate that was able to almost completely block the uptake of pyruvate (Fig. 5d). To verify this observation and further evaluate the effect of accumulated pyruvate on S. mutans cell growth, we monitored the growth of wild-type and ΔlrgAB mutant strains in FMC medium supplemented with increasing amounts of pyruvate (from 0.01 mM up to 80 mM) using a Bioscreen C plate reader. As shown in Fig. 7a, all supplemented pyruvate had no impact on the growth rate of the wildtype cells but prolonged the exponential phase of growth, delaying stationary phase, at concentrations of 4 mM or higher, which is consistent with the observation for the stationary phase uptake of pyruvate. Importantly, similar growth trends were also observed in the ΔlrgAB strain, showing a more evident elongation of exponential phase of growth (Fig. 7b). These results are consistent with the observation that accumulated pyruvate is taken up into the cell only at stationary phase (Fig. 2a) and inactivation of LrgAB does not completely block uptake of pyruvate (Fig. 2b). Collectively, these results further suggest the presence of another pyruvate uptake system, likely acting in a Lrg-independent manner and when concentrations of pyruvate are relatively high. The uptaken pyruvate could contribute to the survival and persistence of cells when the primary carbon source is completely consumed.
Overflowed pyruvate can modulate the level of environmental hydrogen peroxide
It has been reported that some organic keto acids, including pyruvate, show antioxidant activity, e.g. by neutralizing oxidants such as H2O2 [39,40,41,42]. Therefore, it is possible that the induction of lrgAB may be influenced by interspecies interactions, especially with H2O2-producing oral commensals, including S. gordonii. To explore this possibility, we evaluated how lrgAB responds to H2O2 over growth using the PlrgA-gfp reporter strain, as described above. The reporter strain was cultivated in low-glucose FMC medium supplemented by 0.002% (≈0.588 mM) or 0.004% (≈1.176 mM) H2O2, and its GFP production was monitored during growth. The strain displayed an expected increased lag phase in the presence of 0.002% H2O2 (Fig. 8b) relative to that in the absence of H2O2 (Fig. 8a) but a similar stationary phase induction of lrgAB. At 0.004% H2O2, the strain did not grow well (Fig. 8c). Notably, the stationary phase lrgAB induction observed in cultures supplemented with 1 mM pyruvate and 0.002% H2O2 (Fig. 8e) was substantially reduced relative to 1 mM pyruvate alone (Fig. 8d) and without an increased lag phase (Fig. 8e), suggesting that pyruvate was used to scavenge H2O2. This H2O2-scavenging effect was more evidently observed when the strain was cultivated in the presence of 0.004% H2O2, because the strain was able to grow normally in this condition (Fig. 8f). These results suggest that pyruvate may serve S. mutans as a carbon source, as well as an antioxidant against H2O2, consequently contributing to ecological fitness of this organism in the oral cavity. To reinforce this conclusion, we cultivated the reporter strain with S. gordonii DL1, known to secrete substantial amounts of H2O2, in the absence and presence of 1 mM pyruvate, a concentration that has no effect on the growth of S. mutans (Fig. 7a) and S. gordonii (data not shown) but triggers lrgAB induction at the stationary phase. The expression of lrgAB was remarkably reduced by co-cultivation with S. gordonii (Fig. 8g) but the negative effect was almost completely complemented by exogenously adding pyruvate into the culture (Fig. 8h). These results suggest that re-uptake of accumulated pyruvate by S. mutans may be affected by interspecies competition, especially with H2O2-producing oral commensals, consequently altering the metabolic status of the organism .
The S. mutans Cid/Lrg system represents an excellent model to study how this organism withstands various stressors encountered in the oral cavity. Our previously-published “-omics” data suggested that the adaptation process to adverse environments requires metabolic remodeling [7,8,9, 11], which is in accordance with the fact that (i) lrgAB is specifically induced at stationary phase and (ii) is tightly regulated by glucose and oxygen levels [6, 8, 17]. The primary finding of this current study is that LrgAB is important to initiate the rapid re-uptake of pyruvate, excreted during growth, when cells confront carbon starvation/nutrient limitation in stationary growth phase. The excretion (overflow) of pyruvate is a common feature of many bacterial species when cultivated under a carbon-excess condition, contributing to metabolic balancing between carbon uptake and consumption [33, 43,44,45]. Because of its central role in metabolism, it is not surprising that excretion and re-uptake of pyruvate are tightly regulated at multiple levels, and the three main enzymes that utilize pyruvate as a substrate, Pdh, Pfl and Ldh, are accordingly modulated to the cell’s metabolic status and environmental condition [25, 46]. We have previously shown that the pdh and pfl genes, responsible for the conversion of pyruvate to acetyl-CoA, were highly upregulated at late-exponential phase , suggesting that their gene expression is linked with the uptake of pyruvate, functionally and metabolically. Given that the pdh genes were commonly upregulated in response to three stress conditions (aerobic, heat and vancomycin challenge) previously tested , pyruvate uptake and metabolism should affect the ability of S. mutans to adapt to suboptimal conditions. Pyruvate is likely a common nutrient in the microbiome environment, such as oral cavity. But its utilization and regulation in S. mutans have been poorly characterized, especially with respect to how they are connected to the virulence network of this organism.
It seems that the re-uptake of pyruvate is tightly regulated by glucose levels and stationary growth phase lrgAB induction. Growth in high levels of glucose abrogates stationary-phase response of lrgAB to extracellular pyruvate, suggesting that the response of lrgAB to extracellular pyruvate is subject to carbon catabolite repression. Supplementation of exogenous pyruvate was unable to induce earlier induction of lrgAB (normally occurring at stationary phase), reinforcing that uptake of pyruvate occurs only under limited growth, and is subject to tight metabolic control. Given that lrgAB expression requires activation by LytST TCS , repression of lrgAB may be primarily due to inaccessibility of LytT to the promoter region of lrgAB. In our recent study, we found that the cre site for CcpA binding overlapped, in part, with a potential LytT binding site in the promoter region of lrgAB , suggesting that activation of lrgAB by LytT may be prevented by CcpA binding to the promoter region of lrgAB. However, repression of lrgAB was not released even in the absence of CcpA when the cell was cultivated in high-glucose medium , suggesting that additional regulation(s) may be involved in the expression of lrgAB. In fact, CcpA often works together with CodY to sense changes in nutrient availability and coordinate, directly and indirectly, the expression of hundreds of genes involved in carbon and nitrogen metabolism of Gram-positive bacteria [45, 47,48,49]. CodY acts mainly as a repressor, and many genes encoding metabolic pathway components are repressed during growth in the presence of excess nutrients and involved in adaptation to poor growth conditions . Accordingly, we also observed that the codY gene was several-fold upregulated at early-exponential phase, compared to late-exponential growth phase . Thus, it is possible that these two global regulators (CcpA and CodY) interact and modulate lrgAB expression in response to environmental conditions and nutritional needs, which is currently under investigation.
The specific response of lrgAB to extracellular pyruvate was supported by the observation that supplementation of 10 μM 3FP had a profound effect on repressing the expression of lrgAB, likely by interfering with activation of the LytS sensor kinase by pyruvate. These results suggest that LrgAB may be responsible for facilitating the recovery from carbon starvation when concentrations of pyruvate are low. On the contrary, the finding that the stationary phase induction of lrgAB was alleviated by high concentrations of extracellular pyruvate (approx. > 20 mM), revealed the existence of a negative feedback regulation acting on LytST by the presence of high levels of extracellular pyruvate. This feedback regulation may contribute to balanced extracellular and intracellular pyruvate levels, although it remains to be elucidated. Given that the re-uptake of accumulated pyruvate is subject to a tight metabolic control, pyruvate may play a role as a potential metabolic signal to determine cellular fate under limited nutrient conditions. However, this regulatory model does not account for the observation that cells were still capable of utilizing extracellular pyruvate even in the absence of LrgAB, resulting in prolonged exponential growth, suggesting the existence of an additional pyruvate uptake system that operates in a LrgAB-independent manner and preferably when pyruvate concentrations are relatively high (at several mM levels). Indeed, it has been suggested that E. coli uses one exporter and two uptake transporters to modulate the level of intracellular pyruvate . However, uptake of pyruvate does not appear to be attributed to diffusion, because the cell displayed the same growth rate even in the presence of high concentrations of pyruvate. It is also supported by the observation that S. mutans was also unable to grow in a medium containing high concentrations of pyruvate (up to 80 mM) as sole carbon source (Additional file 2: Figure S2). These multiple pyruvate uptake systems and feedback regulations may ensure a tight management of pyruvate homeostasis which in turn may facilitate cellular adaptation.
Although the data herein suggest that LrgAB is primarily responsible for uptake of pyruvate in S. mutans, it remains to be elucidated how LrgAB mechanistically mediates the uptake (transport) of pyruvate. In a preliminary experiment, we found that stationary phase lrgAB induction was significantly inhibited by two hydrophobic protonophores, CCCP (carbonyl cyanide m-chlorophenyl hydrazine) and DNP (2,4-dinitrophenol) at 1 μM and 100 μM, respectively (Additional file 8: Figure S8), suggesting that a pH gradient between interior and exterior of cell may be involved in the activation of LrgAB. Accordingly, a recent study showed that BtsT (also named YjiY) functions as a specific pyruvate/H+ symporter in E. coli . This aspect is being further investigated in LrgAB. It is also noteworthy that lrgAB is induced by pyruvic acid, which still occurs at stationary growth phase (Additional file 9: Figure S9). Although pyruvate could freely diffuse through the lipid bilayer of the cell membrane in its protonated form , most of pyruvic acid should be in a dissociated, charged state (pyruvate), due to acidity of pyruvic acid (pKa = 2.5), suggesting that LrgAB may not be energized only by a proton gradient. Thus, in order to metabolize pyruvate, the uptake systems, including LrgAB, would be required for internalizing pyruvate. It also appears that other metabolic intermediates with structural similarity with pyruvate are transported by LrgAB. In our preliminary experiment using the PlrgA-gfp reporter strain, we observed that lrgAB did not repond to α-ketoglutarate, malate, oxaloacetate, and succinate, but citrate could trigger lrgAB induction (data not shown), suggesting that LrgAB may be specifically responsible for uptake of pyruvate. This theory is also supported by the observation that a synthetic analogue of pyruvate (3FP) effectively competed with pyruvate. This specificity also reinforces the role of pyruvate as a potential metabolic signal, because pyruvate is excreted together with other metabolic compounds. The detailed mechanism for how pyruvate is transported via LrgAB through the cell membrane is an important part of understanding the Cid/Lrg system and warrants further investigation.
Another important finding of this study was that pyruvate directly reacts with H2O2, suggesting that the re-uptake of pyruvate may be influenced by interspecies interactions, especially with H2O2-producing oral commensals, such as S. gordonii and S. sanguinis [53, 54]. The reaction of H2O2 with pyruvate is presented as CH3-CO-COOH+H2O2 → CH3-COOH+H2O + CO2 . Indeed, acetate and CO2 are the major by-products of pyruvate reaction with H2O2, with pyruvate being produced and excreted during exponential growth while glucose is converted to biomass. Acetate would be presumably also taken up into the cell in parallel with pyruvate under nutrient limited growth condition [33, 55]. Intriguingly, the pta-ackA pathway which generates acetate and ATP was reported to cause cell death in S. aureus , and to be regulated by CcpA and CodY in S. mutans  and B. subtilis . Therefore, these observations further suggest a potential connection between pyruvate metabolism and cell death, hypothesized to be induced by the Cid/Lrg system . It is also noteworthy that another organic keto acid, e.g. α-keto glutarate, can effectively scavenge H2O2 [39,40,41,42], suggesting that the level of H2O2 could be modulated by multiple metabolic products. It is an on-going study how the levels of H2O2 and pyruvate (or other organic acids) are changed in the interaction between S. mutans and S. gordonii (or S. sanguinis), and how the LrgAB pyruvate uptake system contributes to the protection from environmental H2O2 challenge.
The results of this study demonstrate that LrgAB is the first identified pyruvate uptake system in S. mutans, and provide an important new basis for how the hypothesized role of LrgAB in modulating cell death and lysis are mechanistically connected to key metabolic pathways. Overall, excreted pyruvate may play several important roles in S. mutans physiology, such as a carbon source and/or metabolic precursor for amino acid/fatty acid biosynthesis under nutrient-limited and/or stationary phase growth conditions, as well as by buffering external sources of oxidative stress, such as H2O2, which primarily appears to be modulated by LytST-LrgAB. Therefore, it is possible that the trafficking and utilization of pyruvate may significantly contribute to shaping a homeostatic mechanism and composition of oral microflora, consequently influencing the development of caries. Nevertheless, due to highly variable in vivo conditions especially in respect to nutrient availability and unknown host factors, the actual effect and role of pyruvate remain to be elucidated and are currently under investigation. This study also opens the possibility of searching for additional pyruvate uptake system as well as examining the relationship between metabolite fluxes and ecological fitness. This will be important as we explore the possible mechanisms underlying stress tolerance and programmed cell death as a bacterial survival strategy at the community level.
Availability of data and materials
The datasets analysed during the current study are available from the corresponding author upon reasonable request.
Loesche WJ. Role of Streptococcus mutans in human dental decay. Microbiol Rev. 1986;50(4):353–80.
Lemos JA, Burne RA. A model of efficiency: stress tolerance by Streptococcus mutans. Microbiology. 2008;154(Pt 11):3247–55.
Smith EG, Spatafora GA. Gene regulation in S. mutans: complex control in a complex environment. J Dent Res. 2012;91(2):133–41.
Bayles KW. The biological role of death and lysis in biofilm development. Nat Rev Microbiol. 2007;5(9):721–6.
Bayles KW. Bacterial programmed cell death: making sense of a paradox. Nat Rev Microbiol. 2014;12(1):63–9.
Ahn SJ, Rice KC, Oleas J, Bayles KW, Burne RA. The Streptococcus mutans Cid and Lrg systems modulate virulence traits in response to multiple environmental signals. Microbiology. 2010;156(Pt 10):3136–47.
Ahn S-J, Gu T, Koh J, Rice KC. Remodeling of the Strpetococcus mutans proteome in response to LrgAB and external stresses. Sci Rep. 2017;7(1):14063.
Ahn SJ, Qu MD, Roberts E, Burne RA, Rice KC. Identification of the Streptococcus mutans LytST two-component regulon reveals its contribution to oxidative stress tolerance. BMC Microbiol. 2012;12(1):187.
Ahn SJ, Rice KC. Understanding the Streptococcus mutans Cid/Lrg system through CidB function. Appl Environ Microbiol. 2016;82(20):6189–203.
Kim HM, Waters A, Turner ME, Rice KC, Ahn SJ. Regulation of cid and lrg expression by CcpA in Streptococcus mutans. Microbiology. 2019;165(1):113–23.
Rice KC, Turner ME, Carney OV, Gu T, Ahn SJ. Modification of the Streptococcus mutans transcriptome by LrgAB and environmental stressors. Microb Genom. 2017;3(2):e000104.
Wang IN, Smith DL, Young R. Holins: the protein clocks of bacteriophage infections. Annu Rev Microbiol. 2000;54:799–825.
Groicher KH, Firek BA, Fujimoto DF, Bayles KW. The Staphylococcus aureus lrgAB operon modulates murein hydrolase activity and penicillin tolerance. J Bacteriol. 2000;182(7):1794–801.
Ranjit DK, Endres JL, Bayles KW. Staphylococcus aureus CidA and LrgA proteins exhibit holin-like properties. J Bacteriol. 2011;193(10):2468–76.
Rice KC, Firek BA, Nelson JB, Yang SJ, Patton TG, Bayles KW. The Staphylococcus aureus cidAB operon: evaluation of its role in regulation of murein hydrolase activity and penicillin tolerance. J Bacteriol. 2003;185(8):2635–43.
Chaudhari SS, Thomas VC, Sadykov MR, Bose JL, Ahn DJ, Zimmerman MC, Bayles KW. The LysR-type transcriptional regulator, CidR, regulates stationary phase cell death in Staphylococcus aureus. Mol Microbiol. 2016;101(6):942–53.
Ahn SJ, Wen ZT, Burne RA. Effects of oxygen on virulence traits of Streptococcus mutans. J Bacteriol. 2007;189(23):8519–27.
Charbonnier T, Le Coq D, McGovern S, Calabre M, Delumeau O, Aymerich S, Jules M. Molecular and Physiological Logics of the Pyruvate-Induced Response of a Novel Transporter in Bacillus subtilis. MBio. 2017;8(5):e00976–17.
van den Esker MH, Kovacs AT, Kuipers OP. YsbA and LytST are essential for pyruvate utilization in Bacillus subtilis. Environ Microbiol. 2017;19(1):83–94.
Marciniak BC, Pabijaniak M, de Jong A, Duhring R, Seidel G, Hillen W, Kuipers OP. High- and low-affinity cre boxes for CcpA binding in Bacillus subtilis revealed by genome-wide analysis. BMC Genomics. 2012;13:401.
Moreno MS, Schneider BL, Maile RR, Weyler W, Saier MH Jr. Catabolite repression mediated by the CcpA protein in Bacillus subtilis: novel modes of regulation revealed by whole-genome analyses. Mol Microbiol. 2001;39(5):1366–81.
Behr S, Kristoficova I, Witting M, Breland EJ, Eberly AR, Sachs C, Schmitt-Kopplin P, Hadjifrangiskou M, Jung K. Identification of a high-affinity pyruvate receptor in Escherichia coli. Sci Rep. 2017;7(1):1388.
Kristoficova I, Vilhena C, Behr S, Jung K. BtsT - a novel and specific pyruvate/H(+) symporter in Escherichia coli. J Bacteriol. 2017;200(2):e00599–17.
Vilhena C, Kaganovitch E, Shin JY, Grunberger A, Behr S, Kristoficova I, Brameyer S, Kohlheyer D, Jung K. A Single-Cell View of the BtsSR/YpdAB Pyruvate Sensing Network in Escherichia coli and Its Biological Relevance. J Bacteriol. 2017;200(1):e00536–17.
Abbe K, Carlsson J, Takahashi-Abbe S, Yamada T. Oxygen and the sugar metabolism in oral streptococci. Proc Finn Dent Soc. 1991;87(4):477–87.
Colby SM, Russell RR. Sugar metabolism by mutans streptococci. Soc Appl Bacteriol Symp Ser. 1997;26:80S–8S.
Terleckyj B, Shockman GD. Amino acid requirements of Streptococcus mutans and other oral streptococci. Infect Immun. 1975;11(4):656–64.
Ahn SJ, Burne RA. Effects of oxygen on biofilm formation and the AtlA autolysin of Streptococcus mutans. J Bacteriol. 2007;189(17):6293–302.
Moretti S, Armougom F, Wallace IM, Higgins DG, Jongeneel CV, Notredame C. The M-Coffee web server: a meta-method for computing multiple sequence alignments by combining alternative alignment methods. Nucleic Acids Res. 2007;35(Web Server issue):W645–8.
Larkin MA, Blackshields G, Brown NP, Chenna R, McGettigan PA, McWilliam H, Valentin F, Wallace IM, Wilm A, Lopez R, et al. Clustal W and Clustal X version 2.0. Bioinformatics. 2007;23(21):2947–8.
Kaspar J, Shields RC, Burne RA. Competence inhibition by the XrpA peptide encoded within the comX gene of Streptococcus mutans. Mol Microbiol. 2018;109(3):345–64.
Kaspar J, Underhill SAM, Shields RC, Reyes A, Rosenzweig S, Hagen SJ, Burne RA. Intercellular communication via the comX-inducing peptide (XIP) of Streptococcus mutans. J Bacteriol. 2017;199(21):e00404–17.
Paczia N, Nilgen A, Lehmann T, Gatgens J, Wiechert W, Noack S. Extensive exometabolome analysis reveals extended overflow metabolism in various microorganisms. Microb Cell Factories. 2012;11:122.
Kodama T, Fukui K, Shimamoto T, Ohta H, Kokeguchi S, Kato K. Effects of oxygen on glucose-limited growth of Streptococcus mutans. Infect Immun. 1987;55(1):169–73.
Takahashi N, Abbe K, Takahashi-Abbe S, Yamada T. Oxygen sensitivity of sugar metabolism and interconversion of pyruvate formate-lyase in intact cells of Streptococcus mutans and Streptococcus sanguis. Infect Immun. 1987;55(3):652–6.
Apfel MA, Ikeda BH, Speckhard DC, Frey PA. Escherichia coli pyruvate dehydrogenase complex. Thiamin pyrophosphate-dependent inactivation by 3-bromopyruvate. J Biol Chem. 1984;259(5):2905–9.
Flournoy DS, Frey PA. Inactivation of the pyruvate dehydrogenase complex of Escherichia coli by fluoropyruvate. Biochemistry. 1989;28(25):9594–602.
Lang VJ, Leystra-Lantz C, Cook RA. Characterization of the specific pyruvate transport system in Escherichia coli K-12. J Bacteriol. 1987;169(1):380–5.
Giandomenico AR, Cerniglia GE, Biaglow JE, Stevens CW, Koch CJ. The importance of sodium pyruvate in assessing damage produced by hydrogen peroxide. Free Radic Biol Med. 1997;23(3):426–34.
Nath KA, Ngo EO, Hebbel RP, Croatt AJ, Zhou B, Nutter LM. alpha-Ketoacids scavenge H2O2 in vitro and in vivo and reduce menadione-induced DNA injury and cytotoxicity. Am J Phys. 1995;268(1 Pt 1):C227–36.
Long LH, Halliwell B. Artefacts in cell culture: alpha-ketoglutarate can scavenge hydrogen peroxide generated by ascorbate and epigallocatechin gallate in cell culture media. Biochem Biophys Res Commun. 2011;406(1):20–4.
Long LH, Halliwell B. The effects of oxaloacetate on hydrogen peroxide generation from ascorbate and epigallocatechin gallate in cell culture media: potential for altering cell metabolism. Biochem Biophys Res Commun. 2012;417(1):446–50.
Poole P, Allaway D. Carbon and nitrogen metabolism in rhizobium. Adv Microb Physiol. 2000;43:117–63.
Shimizu K. Metabolic regulation and coordination of the metabolism in Bacteria in response to a variety of growth conditions. Adv Biochem Eng Biotechnol. 2016;155:1–54.
Shivers RP, Dineen SS, Sonenshein AL. Positive regulation of Bacillus subtilis ackA by CodY and CcpA: establishing a potential hierarchy in carbon flow. Mol Microbiol. 2006;62(3):811–22.
Wang Q, Ou MS, Kim Y, Ingram LO, Shanmugam KT. Metabolic flux control at the pyruvate node in an anaerobic Escherichia coli strain with an active pyruvate dehydrogenase. Appl Environ Microbiol. 2010;76(7):2107–14.
Fujita Y, Satomura T, Tojo S, Hirooka K. CcpA-mediated catabolite activation of the Bacillus subtilis ilv-leu operon and its negation by either CodY- or TnrA-mediated negative regulation. J Bacteriol. 2014;196(21):3793–806.
Santiago B, Marek M, Faustoferri RC, Quivey RG Jr. The Streptococcus mutans aminotransferase encoded by ilvE is regulated by CodY and CcpA. J Bacteriol. 2013;195(16):3552–62.
Gorke B, Stulke J. Carbon catabolite repression in bacteria: many ways to make the most out of nutrients. Nat Rev Microbiol. 2008;6(8):613–24.
Sonenshein AL. Control of key metabolic intersections in Bacillus subtilis. Nat Rev Microbiol. 2007;5(12):917–27.
Kreth J, Lengeler JW, Jahreis K. Characterization of pyruvate uptake in Escherichia coli K-12. PLoS One. 2013;8(6):e67125.
Benning C. Evidence supporting a model of voltage-dependent uptake of auxin into Cucurbita vesicles. Planta. 1986;169(2):228–37.
Zhu L, Kreth J. The role of hydrogen peroxide in environmental adaptation of oral microbial communities. Oxidative Med Cell Longev. 2012;2012:717843.
Barnard JP, Stinson MW. Influence of environmental conditions on hydrogen peroxide formation by Streptococcus gordonii. Infect Immun. 1999;67(12):6558–64.
Jolkver E, Emer D, Ballan S, Kramer R, Eikmanns BJ, Marin K. Identification and characterization of a bacterial transport system for the uptake of pyruvate, propionate, and acetate in Corynebacterium glutamicum. J Bacteriol. 2009;191(3):940–8.
Sadykov MR, Thomas VC, Marshall DD, Wenstrom CJ, Moormeier DE, Widhelm TJ, Nuxoll AS, Powers R, Bayles KW. Inactivation of the Pta-AckA pathway causes cell death in Staphylococcus aureus. J Bacteriol. 2013;195(13):3035–44.
Kim JN, Burne RA. CcpA and CodY Coordinate Acetate Metabolism in Streptococcus mutans. Appl Environ Microbiol. 2017;83(7):e03274–16.
We thank Professor Robert A. Burne (Department of Oral Biology, University of Florida) for providing all the resources needed.
This work was supported by the National Institutes of Health (NIH)- National Institute of Dental and Craniofacial Research (NIDCR) grant R01 DE025237 (S.-J. A.).
Ethics approval and consent to participate
No human/animal experiment is involved in this study.
Consent for publication
The authors declare that there are no conflicts of interest.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Additional file 2: Figure S2. Growth of S. mutans wild type in chemically defined FMC medium containing increasing concentrations of pyruvate as the sole carbon source. Growth was monitored during growth in a Bioscreen C system that was set to shake for 15 s every 30 min. The results are representative of two independent experiments.
Additional file 3: Figure S3. Measurement of extracellular pyruvate during growth of S. mutans ΔcidB mutant strain in low-glucose FMC medium. The strain was grown in a chemically defined medium (FMC) supplemented by 11 mM glucose. For time course measurements of extracellular pyruvate and growth, samples were taken at 1 or 2 h intervals (see Materials and Methods for details). The concentration of pyruvate was determined using an EnzyChrom™ pyruvate assay kit, and growth was measured by the optical density at 600 nm (OD600). Bar indicates the concentration of extracellular pyruvate; line indicates growth curve. The results are average of two independent experiments.
Additional file 4: Figure S4. Measurement of extracellular glucose during growth of S. mutans wild type and ΔlrgAB strains in the high-glucose media. The strains were grown in a chemically defined medium (FMC) supplemented by 45 mM glucose. For time course measurements of extracellular pyruvate and growth, samples were taken at 1 or 2 h intervals (see Materials and Methods for details). The concentration of glucose was determined using an Glucose (HK) assay kit, and growth was measured by the optical density at 600 nm (OD600). Bar indicates the concentration of extracellular pyruvate; line indicates growth curve. The results are representative of two independent experiments.
Additional file 5: Figure S5. Measurement of extracellular pyruvate during aerobic (A and B) or anaerobic (C and D) during growth of S. mutans wild-type (A and C) and ΔlrgAB (B and D) in the low-glucose media. The strains were grown in a chemically defined medium (FMC) supplemented by 11 mM glucose. For anaerobic growth, sterile mineral oil was placed on top of cultures. For time course measurements of extracellular pyruvate and growth, samples were taken at 1 or 2 h intervals (see Materials and Methods for details). The concentration of pyruvate was determined using an EnzyChrom™ pyruvate assay kit, and growth was measured by the optical density at 600 nm (OD600). Bar indicates the concentration of extracellular pyruvate; line indicates growth curve. The results are average of two independent experiments.
Additional file 6: Figure S6. The effect of 3-fluoropyruvate (3FP; pyruvate analogue) on lrg promoter (PlrgA) activity in the presence of pyruvate. The PlrgA-gfp reporter strain was grown in a low-glucose (11 mM) FMC medium supplemented by 0 (A), 0.01 (B), 0.1 (C) or 1 mM (D) 3FP. Pyruvate was added into the medium at the concentration of 1 mM. Relative gfp expression (green square) and OD600 (grey circle; OD) were monitored on a plate reader (see Materials and Methods for details). The results are representative of two independent experiments.
Additional file 7: Figure S7. The effect of 3FP on the growth of S. mutans wildtype. The strain was cultivated in 11 mM glucose FMC media containing different concentrations (0, 1, 2, and 10 mM) of the pyruvate analog 3-fluoropyruvate (3FP). Growth was monitored during growth in a Bioscreen C system that was set to shake for 15 s every 30 min. The results are representative of two independent experiments.
Additional file 8: Figure S8. The effect of protonophores CCCP and DNP on lrg promoter (PlrgA) activity. The PlrgA-gfp reporter strain was grown in a low-glucose (11 mM) FMC medium (A), supplemented by 1 μM CCCP (carbonyl cyanide m-chlorophenyl hydrazine, B) and 0.1 mM DNP (2,4-dinitrophenol, C). Relative gfp expression (green square) and OD600 (grey circle; OD) were monitored on a plate reader (see Materials and Methods for details). The results are representative of two independent experiments.
Additional file 9: Figure S9. Change of lrg promoter (PlrgA) activity during growth in FMC medium supplemented by different concentrations of extracellular pyruvic acid. The PlrgA-gfp reporter strain was grown in a low-glucose (11 mM) FMC medium supplemented by 0 (A), 1 (B), and 2 mM (C) pyruvic acid (PA). Relative gfp expression (green squares) and OD600 (grey circles; OD) were monitored during growth on a plate reader (see Materials and Methods for details). The results are representative of two independent experiments.
About this article
Cite this article
Ahn, S., Deep, K., Turner, M.E. et al. Characterization of LrgAB as a stationary phase-specific pyruvate uptake system in Streptococcus mutans. BMC Microbiol 19, 223 (2019) doi:10.1186/s12866-019-1600-x
- Streptococcus mutans
- Oxidative stress
- Glucose metabolism