Skip to main content
PMC home page
Scientific Reports logoLink to Scientific Reports
. 2020 Nov 12;10:19661. doi: 10.1038/s41598-020-76744-5

Disruption of Streptococcus mutans and Candida albicans synergy by a commensal streptococcus

Joshua T Huffines 1, Jessica A Scoffield 1,✉
PMCID: PMC7661713  PMID: 33184348

Abstract

Polymicrobial interactions in dental plaque play a significant role in dysbiosis and homeostasis in the oral cavity. In early childhood caries, Streptococcus mutans and Candida albicans are often co-isolated from carious lesions and associated with increased disease severity. Studies have demonstrated that metabolic and glucan-dependent synergism between C. albicans and S. mutans contribute to enhanced pathogenesis. However, it is unclear how oral commensals influence pathogen synergy. Streptococcus parasanguinis, a hydrogen peroxide (H2O2) producing oral commensal, has antimicrobial activity against S. mutans. In this study, we utilized a three species biofilm model to understand the impact of S. parasanguinis on S. mutans and C. albicans synergy. We report that S. parasanguinis disrupts S. mutans and C. albicans biofilm synergy in a contact and H2O2-independent manner. Further, metabolomics analysis revealed a S. parasanguinis-driven alteration in sugar metabolism that restricts biofilm development by S. mutans. Moreover, S. parasanguinis inhibits S. mutans glucosyltransferase (GtfB) activity, which is important for glucan matrix development and GtfB-mediated binding to C. albicans mannan. Taken together, our study describes a new antimicrobial role for S. parasanguinis and highlights how this abundant oral commensal may be utilized to attenuate pathogen synergism.

Subject terms: Biofilms, Microbial communities, Fungi

Introduction

Early childhood caries (ECC) is a highly prevalent and costly biofilm-driven disease that disproportionately affects children of low socio-economic status1,2. Streptococcus mutans is commonly isolated from carious lesions of children with ECC, and as such, considered a primary etiological agent of dental caries. S. mutans is regarded as a highly cariogenic bacterium due to its ability to efficiently metabolize dietary carbohydrates into lactic acid, resist acid, and produce insoluble glucan, a sucrose-dependent exopolysaccharide (EPS) that is synthesized by glucosyltransferases (GTFs) and is a major virulence factor that permits the formation of robust biofilms and tooth adherence3–7. Although S. mutans is a primary cause of dental caries, oral plaque contains a consortium of microbes that interact synergistically or antagonistically8–12.

Candida albicans, an opportunistic fungal pathobiont residing throughout the body, is often co-isolated with S. mutans from carious lesions in children with severe ECC infections13–15. Several studies have reported mechanisms in which C. albicans and S. mutans display synergistic behavior. For example, S. mutans was found to significantly increase C. albicans colonization in a Drosophila melanogaster model. Moreover, co-infection with both species resulted in increased biofilm biomass and tooth decay compared to the single species infection in a rat caries model of infection11,16. Despite its involvement in ECC, C. albicans does not efficiently metabolize sucrose, but can readily utilize fructose and glucose17,18. Further, GTFs have been shown to bind to C. albicans mannans, thus promoting EPS production and incorporation of the fungus into the biofilm19. In addition, exogenous GTFs promote C. albicans growth17. Synergism between S. mutans and C. albicans has been well-documented11,16,17,19–21, however, the role of oral commensal streptococci in ECC microbial synergy is poorly understood.

Oral commensal streptococci are primary colonizers of the oral cavity and play a role in maintaining homeostasis by antagonizing oral pathogens via the production of hydrogen peroxide (H2O2). Streptococcus parasanguinis, a mitis group streptococcus and one of the most abundant (5–40% abundance) commensals on the tongue dorsum22–25, exhibits enhanced biofilm formation in a H2O2-dependent manner during co-culture with Aggregatibacter actinomycetemcomitans while simultaneously inhibiting growth of this periopathogen26. Furthermore, S. parasanguinis reduces S. mutans biofilm formation and pathogenesis in a rat caries model of infection in a nitrite and H2O2-dependent manner27–29. Due to the remarkable ability of S. parasanguinis to inhibit both cariogenic and periodontal pathogens, we questioned whether S. parasanguinis could potentially disrupt S. mutans and C. albicans synergy. Although commensal streptococci have been shown to co-aggregate and form biofilms with C. albicans30, there are no studies that dissect how streptococci, like S. parasanguinis, modulate the interaction between S. mutans and C. albicans. In this study, we tested the role of S. parasanguinis in a three species biofilm model containing S. mutans and C. albicans. Here, we report that S. parasanguinis significantly reduces S. mutans and C. albicans biofilm synergy. Interestingly, the reduction in S. mutans and C. albicans biofilm formation was H2O2-independent, and was the result of a disruption in S. mutans sucrose metabolism and a shift in the global metabolic signature by S. parasanguinis. Lastly, we show that S. parasanguinis prevents C. albicans from adhering to glucan and inhibits the formation of glucan by blocking GTF activity. Taken together, our study reveals a new mechanism by which S. parasanguinis safeguards against ECC pathogens, specifically by blocking S. mutans sucrose utilization, and indicates that this commensal could potentially be used as a preventative measure for oral microbial diseases.

Results

Streptococcus parasanguinis inhibits S. mutans and C. albicans biofilm synergy

Streptococcus parasanguinis has been shown to inhibit the virulence of S. mutans, however, the role of this commensal streptococcus on S. mutans and C. albicans synergy is not clearly defined. In an effort to elucidate the interaction between S. parasanguinis and the ECC pathogens, S. mutans and C. albicans, we developed a three species biofilm model. In agreement with previous studies, crystal violet biomass quantification showed that S. parasanguinis and C. albicans produced relatively modest single species biofilms compared to the single species S. mutans biofilm (Fig. 1A). The dual S. parasanguinis and C. albicans biofilm was comparable to a single species S. parasanguinis biofilm. As expected, both the single S. mutans and dual S. mutans–C. albicans biofilms produced robust biofilms (Fig. 1A). Although previous studies report a synergistic increase in biofilm mass31, the dual-species biofilm between C. albicans and S. mutans was not significantly increased compared to the single-species S. mutans biofilm (P > 0.05; Fig. 1A). Strikingly, the addition of S. parasanguinis resulted in a remarkable decrease in both two (S. mutans) and three species biofilms (P < 0.0001; Fig. 1A). This result indicated the possibility that S. parasanguinis dominates the overall biofilm despite the presence of S. mutans and/or C. albicans. In order to quantify the abundance of each species within the biofilm we enumerated colony forming units (CFUs). Surprisingly, S. mutans CFUs were modestly decreased during co-culture with C. albicans (P = 0.0448; Fig. 1B). Further, there was a 2-log reduction (P = 0.0007) in S. mutans CFUs in the presence of S. parasanguinis, regardless of whether C. albicans was present (Fig. 1B). In agreement with our previous study16, C. albicans CFUs were promoted (~ 1.5 log) in the dual biofilm with S. mutans (P < 0.0001; Fig. 1C), but this was abolished when S. parasanguinis was added to the biofilm (P < 0.0001; Fig. 1C). Intriguingly, S. parasanguinis biomass did not change when co-cultured in single, dual, or three species biofilms (Fig. 1D). To gain insight into the overall structure of the multi-species biofilms, we used fluorescently labeled bacterial strains to visualize the biofilm architecture. Using GFP-labeled S. mutans, mCherry-labeled S. parasanguinis, and calcofluor white stained C. albicans, biofilm images were obtained using confocal laser scanning microscopy (CLSM). As expected, the presence of S. parasanguinis decreased the size of the S. mutans microcolonies in both the dual and three-species biofilms compared to the control biofilm (Fig. 2). Taken together, these data demonstrate S. parasanguinis inhibits not only S. mutans biofilm development, but restricts the incorporation of C. albicans into multi-species biofilms.

Figure 1.

Figure 1

Open in a new tab

Streptococcus parasanguinis reduces S. mutans and C. albicans biofilm formation. (A) Crystal violet assay of single-, dual-, and tri-species biofilms (n = 9) ****P < 0.0001. Biofilm colony forming units (CFUs) of (B) S. mutans (Sm) *P = 0.0448 **P = 0.0015 ***P = 0.0007 (C) C. albicans (Ca) **P = 0.0012 ****P < 0.0001 (D) S. parasanguinis (Sp). All biofilms were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2. ns = not significant.

Figure 2.

Figure 2

Open in a new tab

Streptococcus parasanguinis alters the structure of mixed biofilms. Confocal scanning laser microscopy images of wild-type S. mutans, C. albicans, and S. parasanguinis single and mixed biofilms at 60X magnification. S. mutans was labeled with green fluorescent protein (GFP), C. albicans was stained with calcofluor white, and S. parasanguinis was labeled with mCherry. All biofilms were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2. Scale bar: 25 µm. Images were acquired using the Nis Elements 5.0 Imaging Software (https://www.microscope.healthcare.nikon.com/products/software/nis-elements).

Inhibition of S. mutans biofilm is H2O2 and contact-independent

Oral commensal streptococci produce H2O2 to antagonize other bacteria28,32–35. The primary enzyme responsible for H2O2 production in S. parasanguinis is pyruvate oxidase, which is encoded by the poxL gene27,28,35,36. To investigate the potential mechanism of biofilm inhibition by S. parasanguinis and determine whether H2O2 production mediates this interference, both S. mutans and dual C. albicans–S. mutans biofilms were grown with wild-type S. parasanguinis or a pyruvate oxidase deficient mutant (∆ poxL) in transwell plates to physically separate S. parasanguinis from S. mutans and C. albicans. As shown in Fig. 3, the S. mutans single and dual (C. albicans) biofilms were reduced (P < 0.0001) at comparable levels by the presence of wild-type S. parasanguinis or the ∆poxL mutant in the transwell insert. These data indicate that the inhibition by S. parasanguinis was independent of physical contact and H2O2 production.

Figure 3.

Figure 3

Open in a new tab

Inhibition of S. mutans single and dual biofilms with C. albicans by S. parasanguinis is contact and H2O2-independent. Quantification of single and dual species biofilms exposed to wild-type or pyruvate oxidase (poxL) deficient S. parasanguinis in transwells. ns = not significant; ****P < 0.0001. All biofilms were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2.

Metabolomics reveals S. parasanguinis-altered sugar metabolism in multi-species biofilms

Streptococcus mutans biofilm development is driven by carbohydrate metabolism and the synthesis of a glucan matrix from sucrose3–5,11,17,37. To probe how S. parasanguinis impacts sugar metabolism, we conducted global, untargeted metabolic profiling on dual- and three-species combined planktonic and biofilm cultures as well as single species S. parasanguinis cultures to delineate how S. parasanguinis modulates the multi-species biofilm metabolome (Fig. 4A). Principle component analysis revealed the dual C. albicans–S. mutans group to be vastly different than biofilms cultured with S. parasanguinis, with PC1 accounting for 39.6% of the variance (Fig. 4B). Shifts in the metabolic signatures of dual and three species biofilms were largely driven by S. parasanguinis, as the metabolome profiles of multi-species cultures closely resembled a single species S. parasanguinis biofilm. The dual C. albicans and S. mutans biofilm revealed an enriched presence of broad classes of metabolites, including lipids, peptides, cofactors, and amino acids compared to single or dual species biofilms containing S. parasanguinis, including compounds such as tyrosol and glycerol, both of which are indicated in biofilm development for C. albicans38,39 (Figs. S1–S4). Further, the dual C. albicans and S. mutans biofilms had elevated concentrations of sugar alcohols, fructose, glucose, and fructose compared to single and dual species biofilms containing S. parasanguinis, (Fig. 5A), suggesting that S. parasanguinis potentially consumes these sugars. Notably, sucrose consumption was drastically reduced in all biofilms containing S. parasanguinis compared to the dual-species S. mutans–C. albicans biofilm. (Fig. 5A).

Figure 4.

Figure 4

Open in a new tab

Streptococcus parasanguinis dominates the metabolic profile in dual- and tri-species cultures. (A) Global metabolomics profiling of dual- and tri-species cultures and single-species S. parasanguinis cultures. (B) Principle Component Analysis. Sp: S. parasanguinis; Sm: S. mutans; Ca: C. albicans. Metabolomics data were collected for 5 replicates in each group. All cultures were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2.

Figure 5.

Figure 5

Open in a new tab

Presence of S. parasanguinis reduces sucrose utilization by S. mutans (A) Heatmap of carbohydrate metabolites (Value is median normalized) (B) Sucrose assay of single-, dual-, and tri-species cultures. Sp: S. parasanguinis; Sm: S. mutans; Ca: C. albicans. Metabolomics data were collected for 5 replicates in each group. ns = not significant; **P = 0.0096; ****P < 0.0001. All cultures were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2.

To confirm the altered sucrose metabolism, we quantified the sucrose concentrations from biofilm supernatants of single, dual, and three-species cultures (Fig. 5B). Compared to the un-inoculated media control, S. parasanguinis utilized a small fraction of sucrose, S. mutans single and dual biofilms with C. albicans utilized all of the sucrose, but C. albicans did not utilize sucrose when grown alone, as previously reported17. There was no significant difference between a single species S. parasanguinis or dual culture with C. albicans (Fig. 5B), suggesting that any sucrose consumption in these dual biofilms is solely attributed to the presence of S. parasanguinis. In agreement with our metabolomics findings, S. parasanguinis reduced sucrose utilization in the dual (S. mutans) and three-species biofilm cultures (P < 0.0001). Overall, these data show that S. parasanguinis drives metabolism in polymicrobial cultures and may restrict S. mutans and C. albicans synergy by blocking sucrose utilization.

Streptococcus parasanguinis blocks C. albicans glucan binding and impairs S. mutans GTF activity

GtfB-mediated glucan production and binding to C. albicans mannan is considered to be a central mechanism of synergy between the two species17,19. Therefore, we tested whether S. parasanguinis diminishes the ability of C. albicans to adhere and form biofilms with glucan that is synthesized from cell-free S. mutans GTFs. First, to confirm that a single C. albicans biofilm is indeed promoted by the addition of exogenous GTFs from S. mutans, we cultured C. albicans with ethanol precipitated supernatants from wild-type and gtfB deficient S. mutans cultures. As shown in Fig. 6A, the addition of 25 µL supernatant from wild-type S. mutans increased the C. albicans biofilm by approximately 3.5 fold compared to the C. albicans control (P < 0.0001). Supernatant harvested from the gtfB mutant showed defects in the ability to promote C. albicans biofilm compared to wild-type S. mutans. Next, we wanted to determine if S. parasanguinis blocks the ability of GTFs to enhance the C. albicans biofilm. To test this we added varying concentrations (25, 50, and 100 µL) of GTF supernatant to single C. albicans biofilms (+ /− S. parasanguinis). As shown in Fig. 6B, the addition of all concentrations significantly increased C. albicans biofilm, but S. parasanguinis dramatically reduced the ability of C. albicans to increase its biofilm for both the 50 µL and 100 µL groups (P < 0.0001). Finally, to verify this finding, we visualized C. albicans using calcofluor white and CLSM in biofilms containing 100 µL of GTFs and S. parasanguinis. Imaging confirmed that S. mutans supernatant containing exogenous GTFs do indeed promote the C. albicans biofilm, and this promotion is ablated by S. parasanguinis (Fig. 6C).

Figure 6.

Figure 6

Open in a new tab

Streptococcus parasanguinis blocks synergy between GTFs and C. albicans. (A) Crystal violet assay of C. albicans biofilms with supernatant from wild-type or the gtfB mutant strain of S. mutans. (B) Crystal violet assay of C. albicans and C. albicans–S. parasanguinis biofilm with purified GTFs from overnight S. mutans cultures. *P = 0.0246 ****P < 0.0001; (C) Confocal laser scanning microscopy images of C. albicans biofilm stained with calcofluor white with GTFs or GTFs and S. parasanguinis. Scale bar: 50 µm. All cultures were grown in tryptic soy broth containing 0.5% yeast extract (TSBYE) and 1% sucrose for 16 h at 37 °C with 5% CO2.

Due to the ability of S. parasanguinis to induce dramatic shifts in S. mutans sugar utilization, particularly sucrose, and inhibit C. albicans from forming optimal biofilms with GTFs, we reasoned that this result could potentially be due to impaired GTF activity by S. parasanguinis since GTFs convert sucrose to glucan. It is well established that glucan plays a critical role in the formation of a mature S. mutans biofilm and the establishment of mixed species biofilms37,40. To investigate whether altered sucrose utilization was driven by a reduction in GTF activity by S. parasanguinis we purified GTFs from the supernatant of S. mutans cultures. Using a Cascade blue glucan probe, we used confocal microscopy to detect modifications in the ability of purified GTFs to synthesize glucan from sucrose when S. parasanguinis was present. In our positive control, purified GTFs produced copious amounts of glucan with the addition of sucrose compared to GTFs that received no sucrose (negative control) (Fig. 7A). Although GTFs that did not receive sucrose produced a marginal amount of glucan compared to our positive control, we suspect this minor increase was due to carbohydrates in the growth media that permitted a small amount of glucan to be synthesized by purified GTFs. Remarkably, the addition of S. parasanguinis-conditioned, filtered-sterilized supernatant dramatically reduced the formation of glucan, therefore resulting in a drop in fluorescence intensity (Fig. 7A,B). S. parasanguinis also decreased glucan formation in single and mixed species biofilms containing S. mutans (Fig. S5). Overall, these data demonstrate that S. parasanguinis not only shifts carbohydrate metabolism during multi-species biofilm development, but can directly inhibit GTF activity through an unknown secreted factor.

Figure 7.

Figure 7

Open in a new tab

Streptococcus parasanguinis blocks glucan formation by GTFs. Confocal laser scanning microscopy of purified GTFs from S. mutans culture and cascade Blue-labeled dextran in (A) TSBYE, TSBYE + 1% Sucrose, or TSBYE + 1% sucrose with 100 µL of S. parasanguinis supernatant (SN). (B) Fluorescence intensity of each biofilm. ****P < 0.0001 Scale bar: 50 µm. All cultures were grown for 16 h at 37 °C with 5% CO2.

Discussion

Early childhood caries is a biofilm driven disease with S. mutans and C. albicans playing a considerable role9,10,13,15. Previous studies have demonstrated synergistic activity to either S. mutans or C. albicans when cultured together11,17,19–21,40. In addition, C. albicans and oral commensal streptococci have been shown to physically interact and display synergistic behavior within biofilms30,41, however, the impact of oral commensal streptococci in the S. mutans–C. albicans interaction is unclear. In this study, we demonstrate that S. parasanguinis, one of the most prominent commensals in the oral cavity22,23, interferes with S. mutans and C. albicans biofilm synergy in a H2O2 and contact independent manner. Supporting this observation, CLSM analysis revealed a reduction in the size of S. mutans microcolonies in the presence of S. parasanguinis. Remarkably, S. parasanguinis altered the global metabolic signature of the S. mutans–C. albicans cultures. Further, we provide evidence that S. parasanguinis blocks C. albicans from binding glucan, presumably by directly restricting GTF activity, which is essential for C. albicans binding and incorporation into the S. mutans biofilm, as well as robust S. mutans biofilm development. Numerous studies have reported that H2O2 production by commensal streptococci is the main virulence determinant that antagonizes S. mutans28,35,42. Paradoxically, we found that H2O2 had no role in the interference of S. mutans–C. albicans biofilm synergy as the level of biofilm inhibition by H2O2-deficient S. parasanguinis was comparable to wild-type. Overall, our studies highlight a new antimicrobial function for S. parasanguinis and illustrates how this commensal may potentially be used to target S. mutans glucan production, which is critical for not only S. mutans pathogenesis, but synergism with C. albicans.

Our global metabolomics analysis revealed that S. parasanguinis dominated the metabolic profile of dual and tri-species biofilms. Sucrose has consistently been recognized as the primary substrate that governs S. mutans virulence due to the ability of GTFs to synthesize glucan and establish a resilient biofilm3–6,8. C. albicans does not efficiently metabolize sucrose, but instead metabolizes intermediates released from the breakdown of sucrose by S. mutans, such as fructose and glucose43. In our study, fructose and glucose concentrations were elevated in the dual S. mutans and C. albicans biofilm, but the addition of S. parasanguinis severely reduced the levels of these substrates. Fructose, glucose, and sucrose are critical sugars in a recently proposed model of synergism between S. mutans and C. albicans17. Tyrosol, known for stimulating hyphae formation in C. albicans38, was found to be elevated in the C. albicans–S. mutans culture, but was largely absent from biofilms containing S. parasanguinis even though we observed more hyphae formation in the three species biofilms and in single species C. albicans cultures that were incubated with cell-free, purified GTFs. Although it is unclear as to how hyphae formation impacts synergistic biofilm formation, the GTF-dependent synergism is independent of hyphae formation19. Glycerol, indicated as an important regulator for biofilm formation by C. albicans39, was also higher in the dual species biofilm with C. albicans and S. mutans. One limitation of our study is that the metabolomics findings are representative of both planktonic and biofilm cultures. Although the majority of S. mutans cells commit to biofilm formation in the presence of sucrose rather than a planktonic mode of growth, understanding how commensals impact the metabolome of planktonic versus biofilm cells in mixed cultures would be beneficial. It is also important to note that the reduction in sugar metabolism cannot be completely explained by a reduction in S. mutans CFUs. S. parasanguinis reduces S. mutans CFUs by approximately 2-log. However, S. parasanguinis reduced S. mutans sucrose consumption by approximately 15-fold and inhibited the ability of GTFs to utilize sucrose in the cell-free assay when there were no S. mutans cells present. Overall, our findings indicate that S. parasanguinis may consume substrates that are essential for pathogen synergy and possibly sequester nutrients from C. albicans, thus making this fungus less competitive in a polymicrobial environment where it is unable to take advantage of cross-feeding from S. mutans.

A surprising result in our study was that S. parasanguinis inhibited the ability of GTFs to synthesize glucan, which could explain why C. albicans biofilm formation was reduced when this organism was cultured with GTF supernatant and the commensal. Alternatively, since C. albicans has been shown to coaggregate with oral streptococci30,41, S. parasanguinis may also obstruct the ability of GTFs to access mannans on the C. albicans cell surface. It is unlikely that S. parasanguinis and C. albicans compete for GTFs or glucan binding. Although S. parasanguinis surface adhesins have been shown to enhance biofilm formation by binding to biofilm matrix polysaccharides produced by Pseudomonas aeruginosa44, there is no evidence that demonstrate that exogenous GTFs can promote S. parasanguinis biofilm formation. Given that GTFs, particularly GtfB, are critical for biofilm formation, adherence of S. mutans to the tooth surface, and C. albicans–S. mutans synergy, the development of GtfB inhibitors is viewed as a viable strategy to target S. mutans pathogenesis. Structure-based screening has identified small molecules that have demonstrated efficacy against GTF activity45–47. Ideally, GTF targets should display selective activity against S. mutans, but not disturb the composition or function of the oral microbiota, especially commensals. Our findings suggest that commensal-mediated inhibition of S. mutans GTF activity may serve as a novel strategy to hinder S. mutans pathogenesis while preserving the integrity of the oral microbiome. Further dissection of the exact mechanism or molecule (s) involved in S. parasanguinis-mediated inhibition of S. mutans GTF activity is warranted and will be the focus of future studies.

To our knowledge, S. parasanguinis is the only oral commensal that has demonstrated broad antimicrobial and anti-biofilm effects against diverse pathogens, including cariogenic, periodontal, and respiratory pathogens. For example, the S. parasanguinis biofilm is promoted in a H2O2-dependent manner during co-culture with the periopathogen A. actinomycetemcomitans, yet this pathogen loses viability in this model26. In addition, S. parasanguinis has been shown to inhibit S. mutans pathogenesis in a H2O2 and nitrite-dependent manner in a rat caries model of infection42. Moreover, the translocation of S. parasanguinis into the cystic fibrosis (CF) lung has been associated with improved lung function in CF patients48, presumably by antagonizing the major CF pathogen P. aeruginosa. S. parasanguinis reduces viability and pathogenesis of the respiratory pathogen P. aeruginosa in vitro and in a D. melanogaster infection model via reactive nitrogenous intermediate production34. Lastly, a S. parasanguinis surface adhesin (BapA1) facilitates the enhancement of commensal biofilm formation while P. aeruginosa biofilm development is restricted during co-culture44. Taken together, these studies exhibit that the oral commensal S. parasanguinis has the potential to be used as a therapeutic to combat a variety of microbial infections.

In summary, this study provides new insight into how S. parasanguinis disrupts synergy between S. mutans and C. albicans by interfering with GTF activity. The observation that S. parasanguinis hinders GTF activity requires future investigation to identify the specific molecule (s) that mediates this inhibition and test whether it can be harnessed for the development of improved therapeutics. Our present study, as well as previous studies, signifies that S. parasanguinis is a unique commensal that may be suitable for prebiotic or probiotic use. Future studies that explore the molecular mechanisms of S. parasanguinis microbial antagonism will strengthen our understanding of the complexities involved in polymicrobial relationships and aid in the development commensal-derived therapies that are active against oral infections.

Materials and methods

Microbial strains and growth conditions

C. albicans SC5314, S. mutans UA159, S mutans ∆gtfB, S. parasanguinis FW213, and S. parasanguinis ∆poxL34 strains were used in this study. SC5314 was grown in Yeast Peptone Dextrose (YPD) whereas UA159 and FW213 were grown in Tryptic Soy Broth + 5% (w/v) Yeast Extract (TSBYE).

Biofilm and transwell assays

Overnight cultures were grown to mid-exponential phase (OD600 = 0.5) and approximately 1 × 104 colony forming units per milliliter (CFU/mL) were seeded into the biofilm for each species. All single, dual, and three-species biofilms were grown in TSBYE + 1% (w/v) sucrose for 16 h at 37 °C + 5% CO2. For all transwell experiments, a 6-well transwell insert system with a 0.4 μm pore polycarbonate membrane (Corning) was used to grow S. parasanguinis and the poxL mutant in the upper chamber and S. mutans and C. albicans biofilms in the lower well and incubated as described above. Microtiter plates were gently washed 2 times, blotted, and stained with 0.1% crystal violet. Following crystal violet staining, biofilms were washed, dried, and dissolved with 30% acetic acid as described previously49. To quantify biofilms to obtain values in the linear range of the Biotek plate reader, a standard curve was generated by serially diluting acetic acid dissolved biofilms and measuring the OD562 for each dilution. Using a standard curve, the µg of crystal violet was calculated using a trendline of the linear portion (R2 = 0.9966). All dilutions were measured in 96-well plates. Each assay was performed in triplicate wells and repeated three times.

Quantification of colony forming units (CFUs)

All biofilms were gently washed with sterile PBS twice before adding 200 µL of sterile PBS for plating. The biofilms were scraped up with a 200 µL tip, vortexed for 10 s, and were serially diluted. All dilutions were plated on Todd-Hewitt Broth or blood agar plates and were incubated at 37 °C + 5% CO2 for a minimum of 16 h before counting.

Confocal laser scanning microscopy (CLSM)

GFP-labeled UA159 and mCherry-labeled FW213 were used to visualize biofilms. All biofilms for confocal were grown in Ibidi µ-Slide 8 well slides (Cat #: 80826). Wells were gently washed with phosphate-buffered saline (PBS). Wells with C. albicans were stained with calcofluor white in PBS for 15 min before imaging. Biofilms were visualized on a Nikon A1 + confocal laser scanning microscope (CLSM) (Nikon Instruments Inc.) using a 60 × oil immersion lens. Three dimensional biofilm images were acquired using the Nis Elements 5.0 Imaging Software. All images are representative of biofilms from 3 independent experiments.

Metabolomics analysis and sucrose quantification

Single, dual, and three species cultures were grown overnight in 20 mL of TSBYE + 1% sucrose in 50 mL conical tubes. Cells from the entire culture (planktonic and biofilm) were harvested to ensure at least 100 µL of packed cells were available for each of the 5 replicates to meet Metabolon’s processing criteria. Samples were stored in the − 80 °C freezer prior to shipment on dry ice to Metabolon, Inc (Durham, NC). All samples were processed and analyzed for raw counts by Metabolon using liquid chromatography-mass spectrometry (LCMS) methods optimized for positive ions, negative ions, and polar compounds. Raw counts provided by Metabolon were median scaled with missing values imputed with the lowest value. Principal component analysis (PCA) was calculated and graphed using R. Heatmaps of the median scaled data was made using GraphPad Prism.

To measure sucrose concentrations single, dual, and three species cultures were grown and harvested as described above for the metabolomics samples. Samples were stored overnight at − 80 °C prior to quantification. Sucrose concentrations were measured using the Glucose and Sucrose Assay Kit (Sigma Aldrich; Cat No. MAK013).

GTF precipitation, cell-free glucan formation, and glucan quantification

S. mutans proteins from overnight culture supernatants were ethanol precipitated at a 1:1 ratio of 100% ethanol to precipitate extracellular S. mutans GTFs. The ethanol/proteins were incubated at − 80 °C for 1 h, pelleted, and re-suspended in fresh TYE (± 1% sucrose). To test the role of S. parasanguinis supernatant on S. mutans glucan formation, 100 µL of cell-free GTFs were added to 1 mL of TSBYE media that contained no sucrose, 1% sucrose, or 1% sucrose with the additional of 100 µL of filtered-sterilized spent S. parasanguinis media from overnight cultures. Samples were dispensed in polystyrene dishes and incubated for 16 h at 37 °C + 5% CO2 to permit glucan formation. For all experiments, 1 µM dextran-conjugated Cascade Blue (Molecular Probes, Invitrogen) was added to the media before overnight incubation. Fluorescence was quantified using ImageJ.

Statistical analysis

For crystal violet, colony-forming units, and sucrose assays, we analyzed the data using Prism version 8.4.3 (GraphPad Software, LLC). An alpha value of 0.05 was used to determine statistical significance. For the metabolomics data that consisted of 5 replicates, one-way ANOVA was used to determine P values for the single-species group and a two-way ANOVA was used for groups with multiple species.

Supplementary information

Supplementary Figures. (916KB, pdf)

Acknowledgements

We thank Shawn Williams at the University of Alabama at Birmingham High Resolution Imaging Facility for his assistance with the Nikon A1 Confocal microscope and imaging analysis. This project was supported by the following funds and grants awarded to J.A.S: the University of Alabama at Birmingham Department of Microbiology startup funds, National Institutes of Health/National Institute of Dental and Craniofacial Research Grant R00 DE025913, and the American Association for Dental Research/Proctor and Gamble Underrepresented Faculty Research Fellowship.

Author contributions

J.H. and J.S. conceived and performed the experiments and analyzed the results and co-wrote the paper. Both authors discussed the results and revised the manuscript.

Competing interests

The authors declare no competing interests.

Footnotes

Publisher's note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

is available for this paper at 10.1038/s41598-020-76744-5.

References

  • 1.Dye BA, Li X, Thorton-Evans G. Oral Health Disparities as Determined by Selected Healthy People 2020 Oral Health Objectives for the United States, 2009–2010. NCHS Data Brief. Hyattsville: National Center for Health Statistics; 2012. pp. 1–8. [PubMed] [Google Scholar]
  • 2.Casamassimo PS, Thikkurissy S, Edelstein BL, Maiorini E. Beyond the dmft: The human and economic cost of early childhood caries. J. Am. Dent. Assoc. 2009;140:650–657. doi: 10.14219/jada.archive.2009.0250. [DOI] [PubMed] [Google Scholar]
  • 3.Aoki H, Shiroza T, Hayakawa M, Sato S, Kuramitsu HK. Cloning of a Streptococcus mutans glucosyltransferase gene coding for insoluble glucan synthesis. Infect. Immun. 1986;53:587–594. doi: 10.1128/IAI.53.3.587-594.1986. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 4.Hanada N, Kuramitsu HK. Isolation and characterization of the Streptococcus mutans gtfC gene, coding for synthesis of both soluble and insoluble glucans. Infect. Immun. 1988;56:1999–2005. doi: 10.1128/IAI.56.8.1999-2005.1988. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5.Hanada N, Kuramitsu HK. Isolation and characterization of the Streptococcus mutans gtfD gene, coding for primer-dependent soluble glucan synthesis. Infect. Immun. 1989;57:2079–2085. doi: 10.1128/IAI.57.7.2079-2085.1989. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 6.Bowen WH, Koo H. Biology of Streptococcus mutans-derived glucosyltransferases: Role in extracellular matrix formation of cariogenic biofilms. Caries Res. 2011;45:69–86. doi: 10.1159/000324598. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7.Lemos JA, et al. The biology of Streptococcus mutans. Microbiol. Spectr. 2019 doi: 10.1128/microbiolspec.GPP3-0051-2018. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 8.Van Houte J, Sansone C, Joshipura K, Kent R. Mutans streptococci and non-mutans streptococci acidogenic at low pH, and in vitro acidogenic potential of dental plaque in two different areas of the human dentition. J. Dent. Res. 1991;70:1503–1507. doi: 10.1177/00220345910700120601. [DOI] [PubMed] [Google Scholar]
  • 9.Palmer CA, et al. Diet and caries-associated bacteria in severe early childhood caries. J. Dent. Res. 2010;89:1224–1229. doi: 10.1177/0022034510376543. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 10.Kanasi E, et al. Microbial risk markers for childhood caries in pediatricians’ offices. J. Dent. Res. 2010;89:378–383. doi: 10.1177/0022034509360010. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 11.Falsetta ML, et al. Symbiotic relationship between Streptococcus mutans and Candida albicans synergizes virulence of plaque biofilms in vivo. Infect. Immun. 2014;82:1968–1981. doi: 10.1128/IAI.00087-14. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 12.Richards VP, et al. Microbiomes of site-specific dental plaques from children with different caries status. Infect. Immun. 2017;85:e00106–00117. doi: 10.1128/IAI.00106-17. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 13.de Carvalho FG, Silva DS, Hebling J, Spolidorio LC, Spolidorio DM. Presence of mutans streptococci and Candida spp. in dental plaque/dentine of carious teeth and early childhood caries. Arch. Oral. Biol. 2006;51:1024–1028. doi: 10.1016/j.archoralbio.2006.06.001. [DOI] [PubMed] [Google Scholar]
  • 14.Raja M, Hannan A, Ali K. Association of oral candidal carriage with dental caries in children. Caries Res. 2010;44:272–276. doi: 10.1159/000314675. [DOI] [PubMed] [Google Scholar]
  • 15.Bachtiar EW, Bachtiar BM. Relationship between Candida albicans and Streptococcus mutans in early childhood caries, evaluated by quantitative PCR. F1000Research. 2018;7:1645. doi: 10.12688/f1000research.16275.2. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 16.Yang C, et al. Antigen I/II mediates interactions between Streptococcus mutans and Candida albicans. Mol. Oral. Microbiol. 2018;33:283–291. doi: 10.1111/omi.12223. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 17.Ellepola K, et al. Multi-omics analyses reveal synergistic carbohydrate metabolism in Streptococcus mutans–Candida albicans mixed-species biofilms. Infect. Immun. 2019 doi: 10.1128/IAI.00339-19. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 18.Williamson PR, Huber MA, Bennett JE. Role of maltase in the utilization of sucrose by Candida albicans. Biochem. J. 1993;291(Pt 3):765–771. doi: 10.1042/bj2910765. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 19.Hwang G, et al. Candida albicans mannans mediate Streptococcus mutans exoenzyme GtfB binding to modulate cross-kingdom biofilm development in vivo. PLoS Pathog. 2017;13:e1006407. doi: 10.1371/journal.ppat.1006407. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.Kim D, et al. Candida albicans stimulates Streptococcus mutans microcolony development via cross-kingdom biofilm-derived metabolites. Sci. Rep. 2017;7:41332. doi: 10.1038/srep41332. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 21.He J, et al. RNA-Seq reveals enhanced sugar metabolism in Streptococcus mutans co-cultured with Candida albicans within mixed-species biofilms. Front. Microbiol. 2017;8:1036. doi: 10.3389/fmicb.2017.01036. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 22.Human Microbiome Project Consortium Structure, function and diversity of the healthy human microbiome. Nature. 2012;486:207–214. doi: 10.1038/nature11234. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 23.Bernardi S, et al. Combining culture and culture-independent methods reveals new microbial composition of halitosis patients’ tongue biofilm. Microbiologyopen. 2020;9:e958. doi: 10.1002/mbo3.958. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Richards VP, et al. Phylogenomics and the dynamic genome evolution of the genus Streptococcus. Genome Biol. Evol. 2014;6:741–753. doi: 10.1093/gbe/evu048. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 25.Abranches J, et al. Biology of oral streptococci. Microbiol. Spectr. 2018 doi: 10.1128/microbiolspec.GPP3-0042-2018. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 26.Duan D, Scoffield JA, Zhou X, Wu H. Fine-tuned production of hydrogen peroxide promotes biofilm formation of Streptococcus parasanguinis by a pathogenic cohabitant Aggregatibacter actinomycetemcomitans. Environ. Microbiol. 2016;18:4023–4036. doi: 10.1111/1462-2920.13425. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 27.Geng J, et al. Complete genome and transcriptomes of Streptococcus parasanguinis FW213: Phylogenic relations and potential virulence mechanisms. PLoS ONE. 2012;7:e34769. doi: 10.1371/journal.pone.0034769. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 28.Kreth J, Zhang Y, Herzberg MC. Streptococcal antagonism in oral biofilms: Streptococcus sanguinis and Streptococcus gordonii interference with Streptococcus mutans. J. Bacteriol. 2008;190:4632–4640. doi: 10.1128/JB.00276-08. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Redanz S, et al. Pyruvate secretion by oral streptococci modulates hydrogen peroxide dependent antagonism. ISME J. 2020;14:1074–1088. doi: 10.1038/s41396-020-0592-8. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 30.Diaz PI, et al. Synergistic interaction between Candida albicans and commensal oral streptococci in a novel in vitro mucosal model. Infect. Immun. 2012;80:620–632. doi: 10.1128/IAI.05896-11. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 31.Lobo CIV, et al. Dual-species biofilms of Streptococcus mutans and Candida albicans exhibit more biomass and are mutually beneficial compared with single-species biofilms. J. Oral. Microbiol. 2019;11:1581520. doi: 10.1080/20002297.2019.1581520. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 32.Herrero ER, et al. Antimicrobial effects of commensal oral species are regulated by environmental factors. J. Dent. 2016;47:23–33. doi: 10.1016/j.jdent.2016.02.007. [DOI] [PubMed] [Google Scholar]
  • 33.Zheng LY, Itzek A, Chen ZY, Kreth J. Oxygen dependent pyruvate oxidase expression and production in Streptococcus sanguinis. Int. J. Oral. Sci. 2011;3:82–89. doi: 10.4248/IJOS11030. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 34.Scoffield JA, Wu H. Oral streptococci and nitrite-mediated interference of Pseudomonas aeruginosa. Infect. Immun. 2015;83:101–107. doi: 10.1128/IAI.02396-14. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 35.Kreth J, Merritt J, Shi W, Qi F. Competition and coexistence between Streptococcus mutans and Streptococcus sanguinis in the dental biofilm. J. Bacteriol. 2005;187:7193–7203. doi: 10.1128/JB.187.21.7193-7203.2005. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 36.Garcia-Mendoza A, Liebana J, Castillo AM, de la Higuera A, Piedrola G. Evaluation of the capacity of oral streptococci to produce hydrogen peroxide. J. Med. Microbiol. 1993;39:434–439. doi: 10.1099/00222615-39-6-434. [DOI] [PubMed] [Google Scholar]
  • 37.Xiao J, et al. The exopolysaccharide matrix modulates the interaction between 3D architecture and virulence of a mixed-species oral biofilm. PLoS Pathog. 2012;8:e1002623. doi: 10.1371/journal.ppat.1002623. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 38.Alem MA, Oteef MD, Flowers TH, Douglas LJ. Production of tyrosol by Candida albicans biofilms and its role in quorum sensing and biofilm development. Eukaryot. Cell. 2006;5:1770–1779. doi: 10.1128/EC.00219-06. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 39.Desai JV, et al. Regulatory role of glycerol in Candida albicans biofilm formation. MBio. 2013;4:e00637–e00612. doi: 10.1128/mBio.00637-12. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 40.Koo H, Xiao J, Klein MI, Jeon JG. Exopolysaccharides produced by Streptococcus mutans glucosyltransferases modulate the establishment of microcolonies within multispecies biofilms. J. Bacteriol. 2010;192:3024–3032. doi: 10.1128/JB.01649-09. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 41.Jenkinson HF, Lala HC, Shepherd MG. Coaggregation of Streptococcus sanguis and other streptococci with Candida albicans. Infect. Immun. 1990;58:1429–1436. doi: 10.1128/IAI.58.5.1429-1436.1990. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 42.Scoffield J, et al. Dietary nitrite drives disease outcomes in oral polymicrobial infections. J. Dent. Res. 2019;98:1020–1026. doi: 10.1177/0022034519855348. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 43.Sztajer H, et al. Cross-feeding and interkingdom communication in dual-species biofilms of Streptococcus mutans and Candida albicans. ISME J. 2014;8:2256–2271. doi: 10.1038/ismej.2014.73. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 44.Scoffield JA, Duan D, Zhu F, Wu H. A commensal streptococcus hijacks a Pseudomonas aeruginosa exopolysaccharide to promote biofilm formation. PLoS Pathog. 2017;13:e1006300. doi: 10.1371/journal.ppat.1006300. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 45.Zhang Q, et al. Structure-based discovery of small molecule inhibitors of cariogenic virulence. Sci. Rep. 2017;7:5974. doi: 10.1038/s41598-017-06168-1. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 46.Ren Z, et al. Molecule targeting glucosyltransferase inhibits Streptococcus mutans biofilm formation and virulence. Antimicrob. Agents Chemother. 2016;60:126–135. doi: 10.1128/AAC.00919-15. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 47.Nijampatnam B, et al. Inhibition of Streptococcus mutans biofilms by the natural stilbene piceatannol through the inhibition of glucosyltransferases. ACS Omega. 2018;3:8378–8385. doi: 10.1021/acsomega.8b00367. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 48.Filkins LM, et al. Prevalence of streptococci and increased polymicrobial diversity associated with cystic fibrosis patient stability. J. Bacteriol. 2012;194:4709–4717. doi: 10.1128/JB.00566-12. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 49.O'Toole GA. Microtiter dish biofilm formation assay. J. Vis. Exp. 2011 doi: 10.3791/2437. [DOI] [PMC free article] [PubMed] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Supplementary Figures. (916KB, pdf)

Articles from Scientific Reports are provided here courtesy of Nature Publishing Group

RESOURCES