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Streptococcus mutans copes with heat stress by multiple transcriptional regulons modulating virulence and energy metabolism

Scientific Reports volume 5, Article number: 12929 (2015) | Download Citation

Abstract

Dental caries is closely associated with the virulence of Streptococcus mutans. The virulence expression of S. mutans is linked to its stress adaptation to the changes in the oral environment. In this work we used whole-genome microarrays to profile the dynamic transcriptomic responses of S. mutans during physiological heat stress. In addition, we evaluated the phenotypic changes, including, eDNA release, initial biofilm formation, extracellular polysaccharides generation, acid production/acid tolerance, and ATP turnover of S. mutans during heat stress. There were distinct patterns observed in the way that S. mutans responded to heat stress that included 66 transcription factors for the expression of functional genes being differentially expressed. Especially, response regulators of two component systems (TCSs), the repressors of heat shock proteins and regulators involved in sugar transporting and metabolism co-ordinated to enhance the cell’s survival and energy generation against heat stress in S. mutans.

Introduction

Streptococcus mutans, the major etiological agent in dental caries, colonizes the multispecies microbial biofilms that adhere to tooth surfaces1,2. Sophisticated environmental adaptation is critical for the survival and prevalence of S. mutans in the oral cavity, which is a dynamic habitat subject to a wide range of harsh and rapidly changing physiological conditions, including extreme acidity, fluctuation of nutrients, osmotic stress, shifts in temperature and reactive oxygen species, etc3.

The adaptation mechanism to heat stress in bacteria is one of the most conserved biological stress responses in bacteria as they adapt to changing environments4. Temperature shift signals feed into the transcriptional regulatory systems of bacteria, which affects the physiological changes that enable organisms to adapt and survive4. Within the process there are the phases of recognition and adjustment that are coordinated by enzyme and gene level regulation5. Alternative sigma factors play an important role in the adaptation process, which is mediated by complex regulatory networks6. The Escherichia coli heat shock response is highly specific and mediated by members of the sigma 32 regulon through two feedback loops: DnaK/J/GrpE and GroEL/S chaperone systems and inner membrane protease FtsH7. Conversely, although the heat stress response of the Gram-positive bacterium Bacillus subtilis partially overlaps with that of E. coli, it is mainly controlled by the sigma B and CtsR regulators8.

Over many years, the effect of environmental stimuli and the responses to them in streptococci, especially S. mutans, have attracted major research efforts3. S. mutans can resist acid stress through a variety of mechanisms including up-regulation of the proton-translocating F-ATPase3, elevation of cytoplasmic pH through the agmatine deiminase system (AgDS)9 or malolactic fermentation10 and reorganization of membrane fatty acid composition11. The inactivation of reactive oxygen species (ROS) via enzymes results in resistance to oxidative stress3,12. Molecular chaperones, the Clp proteolytic system, TCSs, CcpA-dependent and -independent carbon catabolite repression and quorum-sensing (QS) signalling function to facilitate the ecological fitness of S. mutans13. In addition, protein folding and degradation in S. mutans under heat stress are maintained via the involvement of HrcA and CtsR regulons8. Due to S. mutans lacking an alternative sigma factor14, the transcriptional regulatory responses of S. mutans to heat stress should be different from E. coli and B. subtilis. The current study used whole-genome microarrays, in combination with biological analyses, to investigate the transcriptional and metabolic alterations in S. mutans during heat stress. The aim was to explore how the metabolic pathway-related genes are regulated by the corresponding transcription factors, and how the metabolism of S. mutans changes in response to heat stress.

Results

S. mutans Shows Dynamic Transcriptomic Responses during Heat Stress

To profile the dynamic transcriptomic responses of S. mutans during heat stress, we employed whole-genome microarrays for S. mutans cells incubated at 37 °C versus 42 °C for 5 min, 10 min, 15 min, 30 min, 45 min and 60 min. This resulted in 694 genes that showed differential expression (34.8% of genomic genes) after heat stimuli in S. mutans, including many transcriptional regulators, heat shock-related proteins, ATP-binding cassette (ABC) transport family proteins and phosphoenolpyruvate-sugar phosphotransferase (PTS) system family proteins (Table S1). The levels of differentially expressed genes (DEGs) at each time point are shown in Fig. 1a. Between the six time-points, 75 genes in total were expressed differentially (Table S1). Genes involved in the regulation of transcription predominated the 75 “core DEGs”, such as smu_1027, smu_144c and rpoE, which were followed by members of heat shock regulons, including hrcA, groES, grpE, clpP and clpE. In addition, genes related to DNA metabolism and repair, specifically DNA topoisomerase I (smu_1002) and DNA mismatch repair protein (smu_44), were induced significantly (Table S1).

Figure 1: Transcriptional response pattern of S. mutans during heat shock.
Figure 1

(a). Amount of significantly up- and/or down-regulated genes within different heat shock (42 °C) durations. (b). Transcriptional patterns of S. mutans that had been exposed to heat stress showing clear divergence as determined by principle component analysis (PCA). (c). Validation of microarray data by qRT-PCR. The expression of eight genes were validated by qRT-PCR (n ≥ 3, *P < 0.05).

Principal component analysis (PCA) was used to determine the distance of transcriptomes corresponding to the six time points. Samples marked with distinct colours were projected to a three-dimensional space (Fig. 1b), and the first principle component (PC1) which had the largest variance (35%) separated the samples the most. The samples spread out into three directions (except for one sample in 42 °C at 45 min), demonstrating most of the differences between the gene expression patterns of S. mutans at the six time points. Interestingly, distances from samples in 37 °C increased with the increment of heat stimuli duration. For example, samples grown at 42 °C for 45 min and 60 min were further from ones at 37 °C relative to samples at 42 °C for 5 min and 15 min. Taken together, the PCA plot further demonstrated the dynamic transcriptomic responses of S. mutans during heat stress.

To further validate the reliability of the microarray data, the expression of eight genes during heat stress was determined by qRT-PCR analysis (Fig. 1c). Most of the genes exhibited consistent patterns of differential expression in both the qRT-PCR and microarray, indicating a good concordance of both methods. It should be noted that dnaK and groEL, which showed near 1.2 fold changes under heat stress based on the microarray data, were up-regulated more than 1.5-fold according to the qRT-PCR analysis (Table S1 and Fig. 1c). This could be caused by the underestimation of the fold changes by microarray analysis and the higher sensitivity of qRT-PCR15. In addition, we further examined the expression of these genes in another S. mutans strain (ATCC 55677TM) by qRT-PCR. Both strains (UA159 and ATCC 55677TM) showed similar expression pattern among those selected genes (Fig. S1).

To obtain an overall insight into the impact of heat stress on S. mutans, the DEGs from each time point were assigned a function based on a gene ontology (GO) classification. We obtained 52 significantly changed GO terms (P < 0.01) (Table S2). The majority of DEGs with annotated function were related to regulation and metabolic processes. A significant part of these GO terms showed time dependency (Fig. 2), which is related to the amount and distribution of DEGs at each time point.

Figure 2: Gene ontology (GO) analysis of differentially expressed genes under heat stress.
Figure 2

The significant GO groups were plotted. The dotted line corresponds to a P value of 0.01. The mapping colours indicate GO categories with their names corresponding to the GO group number of the z-coordinate. The number of DEGs included is represented by the circle sizes.

GO analysis indicated the essential functional gene groups at each time point; however, it only provides the broad gene functional categories. Therefore, to further analyse the induced genes during the early and late heat stress responses in S. mutans, subsequent DEGs analysis was performed (Table S3). We noted 22 genes that showed elevated expression only at the 5 min exposure to heat stimuli. These included ComE, superoxide dismutase and 12 hypothetical proteins, which suggested their potential role in sensing the environmental signals. In addition, the expression of 33 and 25 genes was significantly induced from 10 and 15 min, respectively. Limitations in the ability of the microarray to detect the gene expression, so genes with volatile expression were not taken into consideration here.

Multiple Transcription Regulators are Induced in S. mutans Exposed to Heat Stimuli

Gene expression in response to changes in the environment is regulated by a wide range of regulatory proteins in bacteria. Among these, two major types of regulators of transcription are the alternative sigma factors and TCSs6. A possible alternate sigma factor, i.e. ComX, and more than 100 transcriptional regulators have been identified in the genome of S. mutans14. A list of 130 transcriptional regulators and their expression in S. mutans in response to heat stress are shown in Table S4, including 40 regulators embodied in the RegPrecise database16, 15 response regulators of TCSs and 75 other genes annotated as transcriptional regulators in the KEGG database or reported in a previous study17. Of these, 66 were observed in this study to have differential expression when exposed to heat stress. These contained 36 transcriptional regulators that showed significantly differential expressions at more than three time points, including alternative sigma factor (comX), response regulators of TCSs (vicR, ciaR and scnR) and global regulators (rpoE and fruR). In parallel with the induction of these global regulators, we also observed an up-regulation of gene encoding autolysin (smu_704c) (Table S1) and an increase of eDNA released by S. mutans (Fig. 3), indicating an enhanced autolysis during heat stress.

Figure 3: Measurement of eDNA in the planktonic culture of S. mutans.
Figure 3

eDNA release was significantly induced at 42 °C relative to 37 °C at corresponding time points. *P < 0.05.

The smu_2027, which was reported as a LexA-like regulator being induced under different stresses including heat, oxidation and ofloxacin antibiotic and responsible for regulating tolerance toward DNA damage in a noncanonical SOS mechanism18, was also observed significantly up-regulated in the current study (Table S1). In addition, smu_1027 and smu_144c which were annotated as response regulators in the KEGG database also up-regulated upon heat stress (Table S1). Via sequence blast analysis, smu_144c were determined to be conserved in most Streptococci, while smu_1027 was unique in S. mutans.

Classic Molecular Chaperones and Proteases Facilitate Heat Fitness of S. mutans

A set of genes that are all regulated by a specific transcription factor are referred to as a regulon, and these are known to control the responses of bacteria to environmental changes19. To further decipher how the metabolic pathway genes are regulated by the corresponding transcription factors, we analysed the target genes of these differentially expressed transcriptional regulators. From this, the regulon information of nine differentially expressed transcriptional regulators was obtained (Table S5). Of the regulons, two (HrcA and CtsR) have been previously determined to have critical functions in modulating protein folding and degradation pathways in Gram-positive bacteria under environmental stress20,21. They control the expression of members of two well-defined families of heat shock proteins, i.e. molecular chaperones and proteases21,22. Our microarray data showed that the HrcA and CtsR regulons were induced in S. mutans under heat stress (Fig. 4a, b). Up-regulated operons controlled by HrcA under heat stress included grpE-dnaK, groEL-groES and smu_100–103 (Fig. 4a). Although microarray analysis showed no significant change in expression of dnaK and groEL during heat stress, the expression of these genes were demonstrated to be up-regulated by qRT-PCR analysis. The expressions of both dnaK and groEL were also demonstrated to be up-regulated after heat stress in S. mutans by slot blot analysis in previous studies20,22. Unlike most Gram-positive bacteria, in S. mutans the HrcA and CtsR repressors dually control the transcription of the groE operon23. In addition, other genes regulated by CtsR are up-regulated after exposure to 42°C, including gene encoding ATP-dependent protease (clpE), ATP-dependent Clp protease proteolytic subunit (clpP)21,24 and genes related to DNA mismatch repair (smu_43 and smu_44) (Fig. 4b). ClpP is proteolytic subunit of Clp functional complex, which specifically targets damaged and misfolded proteins. ClpP alone can also degrade proteins that might be toxic for the bacteria but with relatively lower efficiency21,24. Recent study showed that deletion of clpP in S. mutans resulted in a sensitive phenotype to heat stress24. Hence, the up-regulation of ClpE and ClpP is believed to be a defensive mechanism adopted by the bacterium to clear damaged or misfolded proteins under heat stress. Heat shock proteins and proteases were also reported to be related to acid tolerance in S. mutans20,24. We thus examined whether pre-adaptation to heat stress would affect bacterial survival under acid challenge. We observed that pre-adaptation to heat stress had no significant effect on cell survival under acid challenge (Fig. S2), as also being reported by others25.

Figure 4: Transcriptional profiles of genes modulated by selected transcription factors under heat stress in S. mutans.
Figure 4

Line graphs show the normalized expression profiles of DEGs regulated by HrcA (a), CtsR (b), TCS response regulator VicR (c) and global regulator FruR (d) at 5, 10, 15, 30, 45, and 60 min at 42 °C relative to 37 °C.

Essential Response Regulators of TCSs in S. mutans upon Heat Stress

Bacterial TCS transduction systems play important roles for many bacteria by enabling them to detect and respond to diverse changes/stresses in the environment. TCS response regulators have been shown to be involved in regulating target genes in S. mutans under acid stresses26.

VicR is the response regulator of the vicKR TCS system, which is essential for the survival of S. mutans and plays a major role in the stress response, competence development, sugar metabolism and biofilm formation27. A previous study found that vicR was an essential response regulator of S. mutans upon treatment with carolacton (a biofilm inhibitor) by regulating the expression of gtfB, gtfD and gbpB28. In this work, we observed a set of genes, including gene encoding glucosyltransferase-SI (gtfC), transcriptional regulators (malR and smu_439), gene encoding endolysin (smu_707c) and UDP-N-acetylglucosamine 2-epimerase (epsC), were regulated by vicR in S. mutans under heat stress (Fig. 4c).

Of the TCSs, CiaR is a global regulator involved in multiple stress responses, biofilm formation and bacteriocin production in S. mutans19. Genes such as smu_139, smu_239 and smu_739 have previously been reported as potential targets of CiaR19. Under heat stress, a significant continuous up-regulation of smu_139 was observed, along with increased expression of ciaR at multiple time points (5 min, 15 min and 45 min) after exposure to heat stimuli (Table S5). The smu_139 gene and its role in S. mutans stress response should be further investigated as it has been predicted to encode a protein associated with carbohydrate metabolism in the KEGG database29.

Heat Stimuli Induce Specific Sugar Transport Regulons and Glucans Synthesis

The regulons of the sugar-specific transcriptional regulators were significantly induced upon heat stress in S. mutans, such as the repressors FruR, GalR, MalR and LacR (Fig. 4d and Table S5). Although DEGs were enriched in these predicted regulons, only two genes encoding the EII loci (fructose-1-phosphatate kinase and galactose-6-phosphate isomerase subunit LacA) were induced significantly, indicating that heat may induce other biological processes controlled by these sugar-specific transcriptional regulators. This confirms previous studies in which PTSs were shown to be related to transcriptional regulation, catabolite repression and enzyme activity as well as sugar transport and phosphorylation30. Instead, heat activated the expression of smu_100–103, which were predicted to be the target genes of HrcA. A previous study has shown that this operon was a sucrose-inducible PTS and it might transfer carbohydrates synthesized by glucosyltransferase-I (GtfB) and glucosyltransferase-SI (GtfC) of S. mutans31. Their transcriptional regulator, smu_105, was not affected by heat stress. Collectively, the results indicated that this sucrose-inducible PTS could also be induced and might be involved in glycogen uptake under heat stress. In S. mutans, sugar substrates can also be taken up by ABC transporters. Under heat stress, we observed the up-regulation of two members of sugar ABC transporter systems, i.e. polysaccharide ABC transporter permease (smu_827) and the multiple sugar-binding ABC transporter permease MsmF (smu_879) (Table S1).

Sugars are microbial substrates for the synthesis of glucan, which is required for adherence and biofilm formation in S. mutans32. Under heat stress, gtfC and gbpC, but not gtfB, gtfD, gbpB, gbpD and ftf, were identified to be up-regulated by more than 1.5 fold from 10 min to 60 min (Table S1). Further investigation of the adherence and biofilm formation of S. mutans by fluorescent live/dead staining showed that the initial attachment was significantly impaired during heat stress (Fig. 5a,b). SEM analysis further confirmed that biofilm formation was compromised, as the 6 h biofilms showed more channel-like structures at 42 °C relative to those at 37 °C (Fig. 5c). As S. mutans GtfC can produce both water-insoluble and water-soluble glucans33, the up-regulation of gtfC may compensate the compromised sugar-dependent biofilm formation under heat shock. We thus quantified the extracellular polysaccharides (EPS) synthesized by S. mutans UA159, gtfB- and gtfC-deficient mutants with fluorescence-labelled dextrans. We found that EPS generation by S. mutans UA159 strain was not significantly impaired at 42 °C relative to 37 °C (Fig. 5d,e), indicating possible compensatory mechanisms of this bacterium under heat stress. The gftC-deficient mutant, but not the gtfB-deficient mutant, showed significantly impaired EPS production at 42 °C relative to 37 °C (Fig. 5d,e), further supporting our speculation that up-regulation of gtfC may involve the compensatory EPS-generation by S. mutans after heat shock.

Figure 5: Sucrose-dependent initial attachment and biofilm architecture of S. mutans during heat shock.
Figure 5

(a). Representative images of S. mutans (live: green; dead: red) grown on the glass surface after 2 h and 4 h incubation at 37 °C and 42 °C, respectively. (b). Quantitative analyses of coverage area (μm2) of S. mutans grown on the glass surface. (c). Representative SEM images from 6 h S. mutans biofilms at 37 °C versus 42 °C. (d). Representative confocal laser scanning microscopy images of EPS (red) produced by S. mutans UA159 and its gtf-mutants (green) under heat stress. (e). Quantitative analyses of normalized EPS (EPS/bacteria) produced by S. mutans UA159 and its gtf-mutants. Data were obtained from an average of three independent experiments and shown as mean ± standard deviation. *P < 0.05, **P < 0.01 compared with 37 °C controls at corresponding time points. N.S.: no significant difference.

S. mutans Up-regulates ATP Turnover to Counter Heat Stress

To survive under heat stress, S. mutans up-regulated genes encoding ATP-dependent transporters together with heat-triggered proteins and genes related to DNA-repair machinery (Table S1). All these biological processes require increased ATP turnover during the heat shock process. Here we observed an increase of intracellular ATP levels in S. mutans during heat stress (Fig. 6a). In parallel with increased intracellular ATP, glycolysis by S. mutans, as reflected by a pH drop and the amount of lactic acid produced in the sucrose-rich medium, was also significantly enhanced during heat shock (Fig. 6b,c). In addition, genes encoding fructose-1-phosphate kinase (smu_871) and NADH oxidase (nox), respectively, were continuously up-regulated under heat stress (Table S1). Fructose-1-phosphate kinase, also known as phosphofructokinase, is one of the three regulated enzymes in glycolysis34, and NADH oxidase is an enzyme critical for the maintenance of the NADH+:NAD+ ratios during active glycolysis35. That glycolysis is increased under heat stress in S. mutans is further shown by these two genes being up-regulated.

Figure 6: Effect of heat stress on metabolism in S. mutans.
Figure 6

(a). Time-course of intracellular ATP level of S. mutans incubated at 37 °C versus 42 °C. (b). Glycolysis-induced pH drop by S. mutans grown in sucrose-rich medium incubated at 37 °C versus 42 °C. (c). Quantification of lactic acid generated by S. mutans incubated at 37 °C versus 42 °C. Results are presented as mean ± standard deviations (n = 3). *P < 0.05 level compared with 37 °C controls at corresponding time points.

Discussion

The ability to respond to environmental perturbation is critical for bacteria to colonise new areas and survive36. The strategy employed by bacteria to tolerate heat stress is highly conserved36, and the accumulation of unfolded polypeptides as well as impairment of DNA act as triggers that lead to various changes in the global transcriptional profiles at different time points4. The specific mechanisms in the heat stress response differ between Gram-positive and Gram-negative bacteria8,37. Unlike the classic Gram-positive model bacterium B. subtilis, S. mutans is characterized by a host-associated lifestyle, non-sporulating phenotype and lower GC content (less than 40%). This has led to the recent proposal to consider S. mutans as a new Gram-positive paradigm2. Considering its ‘feast or famine’ lifestyle, strong aciduricity and relatively small genome, S. mutans has most likely developed unique measures to cope with heat stress. Our data showed that S. mutans had a dynamic transcriptional response to heat shock.

S. mutans has an even and steady response to heat shock as indicated by a balanced distribution of DEGs at multiple time points. This pattern of response is distinct from that of E. coli, whose DEGs peaked within 10 min upon heat shock38. The mild heat shock response (42 °C) of E. coli is almost entirely regulated by the amount and activity of the alternative sigma factor (Sigma 32, RpoH)39. Conversely, B. subtilis responds to general stress including heat stress via sigma B40. In addition, B. subtilis also possesses multiple sigma factors to cope with various environmental stimuli41. Unlike E. coli and B. subtilis, S. mutans UA159 possesses only one copy of a possible alternate sigma factor, i.e. ComX14. However, more than 100 transcriptional regulators (whole genome of 2 Mb with 1900 genes) and 14 TCSs, as well as one orphan response regulator have been identified in the genome of this bacterium14,42. In this work, 66 transcriptional regulators (including comX) were induced under heat stimuli in S. mutans. Moreover, the regulons analysis showed significantly induced target genes of multiple transcriptional regulators upon heat shock. Our data indicated that many transcriptional regulators coordinate the fitness of S. mutans to heat stress, possibly due to the lack of alternative sigma factors in the bacteria. In addition, the up-regulated expression of comX and comYABCD at multiple time points may increase the natural competence of S. mutans under heat stress. The heat-induced up-regulation of comX and comYABCD may justify the rationale of a heat shock method for bacterial transformation43.

Heat shock proteins (HSPs), which are similar in both eukaryotic and prokaryotic cells, are vital for cells to survive heat stress44,45. Members of two well-defined families of heat shock proteins, i.e. molecular chaperones and proteases, were induced during heat shock in S. mutans. Specifically, the genes encoding ClpE and ClpP were significantly induced in the current study. The ClpP protease is associated with ClpE to form a functional complex that is critical for the survival of S. mutans under environmental stress, including acid, temperature, and oxidative stresses by degrading denatured proteins or stabilizing native proteins21,24,46. S. mutans that was deficient in clpP was more sensitive than the wild-type to environmental stimuli47. Hence, the observed up-regulation of ClpE and ClpP during heat stress may contribute to the fitness of S. mutans under this harsh condition.

Notably, the proper function of these heat shock proteins will inevitably consume extra energy during heat stress. To cope with the energy demand, S. mutans may increase production of ATP. Here we observed an elevated level of intracellular ATP, similar to that reported in Staphylococcus aureus during heat shock48. Elevation of intracellular ATP may be the consequence of either enhanced bacterial energy-generation or energy-sparing adaptations (e.g. growth arrest). The observed enhanced microbial glycolysis, lactic acid production and up-regulation of genes encoding NADH oxidase and sugar transporters in the current study suggest that S. mutans may more likely up-regulate energy generation to cope with heat shock.

Heat stress also attenuated the initial attachment of S. mutans and led to the formation of a biofilm that contained more channels. The sucrose-dependent attachment of S. mutans was mediated by two major types of adhesions, i.e. cell-surface proteins and sucrose-derived glucans49. GtfB predominately generates water-insoluble polysaccharides, which act as the major components of the extracellular matrix (ECM) and mediate cellular adherence and biofilm formation of S. mutans50. On the contrary, GtfC is related to the synthesis of a glucan that has a low-molecular-mass and is partially water-soluble, and this can be either used to produce energy via being metabolized or to form part of a biofilm50. Here we observed that gtfC but not gtfB was up-regulated during heat shock. The up-regulation of gtfC may metabolize carbohydrate substrates for both energy-generation and EPS generation. Our data that gtfC-mutant instead of gtfB-mutant demonstrated significantly impaired EPS generation at 42°C relative to 37 °C further support the compensatory role of gtfC in EPS generation during heat stress. The up-regulation of gtfC may further help to offset damaging stresses via molecular machinery (e.g. HSPs) that consumes ATP. In addition, GtfC can be directly embedded in the acquired pellicle with enzymatic activity51. The partially soluble glucans can be recognized by other subtypes in the cell surface, such as glycosyltransferases (Gtfs) or glucan binding proteins (Gbps), thus contributing to cell attachment51. In addition to gtfC, gbpC was also up-regulated by heat stress. This may also compensate for the compromised biofilm formation under heat shock by forming a less energy consuming structure of GtfC-glucan-GbpC.

Taken together, by using whole-genome microarrays to profile the transcriptomic responses of S. mutans during heat shock, we have demonstrated that S. mutans acts as a new paradigm of a Gram-positive bacterium that responds to heat stress in a distinct pattern. The dynamic transcriptional alterations of multiple regulators and functional genes, together with enhanced glycolytic activity, attenuated sucrose-dependent initial attachment and impaired biofilm architecture, indicate metabolic adaptations by this bacterium to compensate for the extra energy demand required to counter adverse environmental stimuli.

Materials and Methods

Bacterial Strains and Growth Conditions

The S. mutans UA159 and S. mutans ATCC 55677TM strains were obtained from the American type Culture Collection (ATCC, Manassas, VA, USA). The gtfB- and gtfC-deficient mutants were kindly provided by Robert A. Burne (Department of Oral Biology, College of Dentistry, University of Florida, Gainesville, FL). S. mutans was routinely grown in brain heart infusion broth (BHI; Difco, Sparks, MD, USA) at 37 °C anaerobically52. To enable the sucrose-dependent initial attachment and biofilm assay, the BHI broth was supplemented with 1% sucrose. For the exposure to heat stress, cultures of S. mutans (OD600 nm = 0.5) were transferred from 37 °C to a 45 °C water bath, and the temperature of each culture was raised to 42 °C in <4 min. Then the cultures were transferred to a 42 °C water bath for 5 min, 10 min, 15 min, 30 min, 45 min and 60 min. The control was a cell culture grown at 37 °C and collected before the transfer to the 45 °C water bath.

Microarray Procedures

Immediately after heat stress, all cell cultures were collected and treated with RNA protect reagent (Qiagen, Valencia, CA, USA). A previously described RNA extraction method was used52. In brief, RNA was extracted and purified using RNeasy Mini kits (Qiagen) and digested with RNase-free DNase I (Qiagen). The concentration of RNA was measured by a Nanodrop ND 1000 spectrophotometer (Thermo Fisher Scientific, Pittsburgh, PA, USA). Agarose electrophoresis was then used to determine the integrity and quality of RNA.

S. mutans UA159 whole-genome arrays (8 × 15 K) were obtained from Agilent and included 1997 probes for S. mutans transcripts. RNA samples were labelled with cyanine 3 or cyanine 5 (GE Healthcare), and the labelled RNA was hybridized to the microarray at 45 °C overnight. The arrays were scanned with an Agilent G2562CA Microarray Scanner, and an Agilent Feature Extraction Software (Version 11.0.1.1) was used to analyse the acquired images. A range of R/Bioconductor packages were used with the raw data to normalize and annotate it. DEGs were identified by the Rank Product method, with fold changes >1.5 and P < 0.0553. Gene set enrichment analysis (GSEA) was employed to determine the significant GO terms of the DEGs54. The microarray data were confirmed using qRT-PCR with the expression of eight transcripts using a previously published method and the primers in Table S652,55. By integrating the transcript units information56, promoter binding motifs28, and experimental validation, we summarized heat stress-induced regulons of S. mutans (see Table S5 for details).

Microarray Data Accession

All data obtained from the microarray analysis have been added to the NCBI Gene Expression Omnibus database with an accession number GSE59302 (http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?token=abetgqeadtavhcv&acc=GSE59302).

ATP Determination, Glycolytic pH Drop Assay, Lactic Acid and eDNA determination

To measure the influence of heat stress (42 °C) on intracellular ATP levels, mid-logarithmic phase (OD600 nm = 0.5) cell cultures of S. mutans were collected after exposure to heat stimuli at 0 min, 5 min, 10 min, 15 min, 30 min, 45 min and 60 min. ATP levels were quantified by a luminometric ATP detection assay with BacTiter-GloTM kit from Promega as described in a previous study48. To determine the effect of heat stress on the glycolysis of S. mutans, the decrease in the pH over 75 min in a sucrose solution (1%, wt/vol) was recorded57. For lactic acid determination, supernatants of S. mutans cultures were collected by centrifugation (4000 rpm, 10 min) after incubation at 37 °C or 42 °C for 5 min, 10 min, 15 min, 30 min, 45 min and 60 min, respectively. Lactate concentrations in the supernatants were determined using an enzymatic (lactate dehydrogenase) method previously described58. The absorbance at 340 nm (OD340 nm) before and after the reaction was measured by a microplate reader (Gene, Hong Kong, China). Standard curves were plotted using a lactic acid standard (Supelco Analytical, Bellefonte, PA).

eDNA in planktonic cultures was measured by a spectrofluorometry method as previously reported with minor modifications59. Briefly, cell cultures of S. mutans UA159 with an OD600 nm value of 0.5 were collected and incubated in a water bath (37 °C or 42 °C). At the indicated time points, 4.5 ml of supernatant were collected by centrifugation (12,000 rpm, 1 min) and filtered by DNA purification columns (Qiagen). eDNA was then eluted by 210 μl H2O and labelled with 2.5 μl of 50 μM cell-impermeant fluorescent dye SYTOX Green (Invitrogen) for 10 min. 200 μl of stained samples were transferred to a 96-well plate (Corning, Inc., NY, USA) and eDNA was quantified by measuring the intensity of fluorescence (excitation at 485 nm, and emission at 535 nm) using a BioTek Synergy 2 HT microplate reader (Biotek Instruments, Winooski, VT, USA).

Sucrose-dependent Initial Attachment and Biofilm Assay

The effect of heat stress on the attachment of S. mutans’ cells was determined using a previously described method60. S. mutans was collected at mid-log phase, washed twice with PBS, and then re-suspended in BHI medium containing 1% sucrose to a level of 1 × 106 CFU/ml. After 2 h or 4 h incubation on saliva pre-coated coverslips, biofilms were collected and stained with the fluorescent Live/Dead BacklightTM stain (Molecular Probes Inc., Eugene, Oregon, USA), and observed with a Leica TCS SP2 confocal laser scanning microscope (Leica, Germany). Images were analysed by Image-pro Plus 6.0 (Media Cybernetics Inc., Bethesda, MD, USA) to quantify the amount of initially attached bacteria. The heat stress effect on the biofilm structure was further determined using a scanning electron microscope (SEM) as described previously52. To further investigate the EPS synthesis of S. mutans under heat stress, 12 h biofilm of S. mutans UA159, and its gtfB-/gtfC-deficient mutants grown on saliva pre-coated coverslips were double-labelled with 2.5 μmol L−1 of Alexa Fluor 647-labelled dextran conjugate (10000 MW; absorbance/fluorescence emission maxima of 650/668 nm; Molecular Probes Inc., Eugene, OR, USA) and a SYTO 9 green fluorescent nucleic acid stain (2.5 μmol L−1, 480/500 nm; Molecular Probes Inc.) as described previously52.

Cross-protection assay

Cross-protection experiments were performed to determine whether pre-adaption to heat stress (42 °C, 2 h) could affect the survival of S. mutans challenged at acidic condition (pH = 2.8, 2 h). Briefly, S. mutans cells at mid-exponential phase (OD600nm = 0.5) were incubated in BHI medium (pH = 7) at either 37 °C or 42 °C for 2 h, and then re-suspended in 0.1 M sodium citrate buffer (pH = 2.8, 2 h). 200 μl of cell suspend before and after acid challenge were diluted and plated on BHI agar plates (pH 7.5). The viable cells were counted after 48 h incubation (37 °C) and the survival rate after acid challenge was calculated.

Statistical Methods

Microarray data were analysed using the R Project for Statistical Computing. A two-tailed paired Student’s t test was used for qRT-PCR, metabolite determination and biomass assay. Data in the graphs are expressed as the mean ± standard deviation and P values < 0.05 were considered significantly different.

Additional Information

How to cite this article: Liu, C. et al. Streptococcus mutans copes with heat stress by multiple transcriptional regulons modulating virulence and energy metabolism. Sci. Rep. 5, 12929; doi: 10.1038/srep12929 (2015).

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Acknowledgements

We thank Nicholas Short for critical reading of the manuscript. This work was supported by grant from the Science and Technology Department of Sichuan Province, China (grant number: 2013HH0009 to XX), the National Science & Technology Pillar Program during the 12th Five-year Plan Period (grant number: 2012BAI07B03 to JL), National Natural Science Foundation of China (grant number: 81200782 to XX; 81170959 to XZ). Yulong Niu was supported by China Scholarship Council. We thank Robert A. Burne’s laboratory for providing gtfB-/gtfC-deficient mutants.

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Author notes

    • Chengcheng Liu
    •  & Yulong Niu

    These authors contributed equally to this work.

Affiliations

  1. State Key Laboratory of Oral Disease, West China Hospital of Stomatology, Sichuan University, Chengdu, PR China

    • Chengcheng Liu
    • , Xuedong Zhou
    • , Xin Zheng
    • , Shida Wang
    • , Qiang Guo
    • , Yuqing Li
    • , Mingyun Li
    • , Jiyao Li
    • , Yi Ding
    •  & Xin Xu
  2. Department of Operative Dentistry and Endodontics, West China Hospital of Stomatology, Sichuan University, Chengdu, PR China

    • Xuedong Zhou
    • , Xin Zheng
    • , Jiyao Li
    •  & Xin Xu
  3. Key Lab of Bio-resources and Eco-environment of Ministry of Education, College of Life Sciences, Sichuan University, Chengdu, PR China

    • Yulong Niu
    •  & Yi Yang
  4. Department of Periodontics, West China Hospital of Stomatology, Sichuan University, Chengdu, PR China

    • Chengcheng Liu
    •  & Yi Ding
  5. Center for Oral Health and Systemic Disease, School of Dentistry, University of Louisville, Louisville, Kentucky, USA

    • Chengcheng Liu
    •  & Richard J. Lamont

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Contributions

C.L. and Y.N. performed the majority of the experiments, analysed the data and drafted the manuscript. X.Z. helped with the measurement of lactic acid. X.Z. helped to design the study and draft the manuscript. S.W., Q.G., Y.L., M.L., J.L., Y.Y., Y.D. and R.L. provided suggestions for the project and critically reviewed the manuscript. X.X. supervised the project and wrote most of the manuscript. All authors read and approved the final manuscript.

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The authors declare no competing financial interests.

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Correspondence to Xin Xu.

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