Streptococcus oligofermentans Inhibits Streptococcus mutans in Biofilms at Both Neutral pH and Cariogenic Conditions


Homeostasis of oral microbiota can be maintained through microbial interactions. Previous studies showed that Streptococcus oligofermentans, a non-mutans streptococci frequently isolated from caries-free subjects, inhibited the cariogenic Streptococcus mutans by the production of hydrogen peroxide (HP). Since pH is a critical factor in caries formation, we aimed to study the influence of pH on the competition between S. oligofermentans and S. mutans in biofilms. To this end, S. mutans and S. oligofermentans were inoculated alone or mixed at 1:1 ratio in buffered biofilm medium in a 96-well active attachment model. The single- and dual-species biofilms were grown under either constantly neutral pH or pH-cycling conditions. The latter includes two cycles of 8 h neutral pH and 16 h pH 5.5, used to mimic cariogenic condition. The 48 h biofilms were analysed for the viable cell counts, lactate and HP production. The last two measurements were carried out after incubating the 48 h biofilms in buffers supplemented with 1% glucose (pH 7.0) for 4 h. The results showed that S. oligofermentans inhibited the growth of S. mutans in dual-species biofilms under both tested pH conditions. The lactic acid production of dual-species biofilms was significantly lower than that of single-species S. mutans biofilms. Moreover, dual-species and single-species S. oligofermentans biofilms grown under pH-cycling conditions (with a 16 h low pH period) produced a significantly higher amount of HP than those grown under constantly neutral pH. In conclusion, S. oligofermentans inhibited S. mutans in biofilms not only under neutral pH, but also under pH-cycling conditions, likely through HP production. S. oligofermentans may be a compelling probiotic candidate against caries.


The human oral cavity harbours a dynamic microbial community, which consists of more than 700 bacterial species [1]. In the healthy situation, this community maintains a healthy microbial homeostasis, through a dynamic balance of synergistic and antagonistic microbial interactions. Disturbance of this homeostasis can lead to shifts in microbial composition and eventually cause diseases e.g. dental caries [2]. Dental caries is chemical dissolution of the dental hard tissues by the acid produced when bacteria metabolise dietary carbohydrates. Under prolonged low-pH environment, the outgrowth of acidogenic and aciduric species such as mutans streptococci and lactobacilli shifts the microbial composition and enhances the dissolution of the dental hard tissue, eventually causing caries [3,4]. One of the key concepts in the prevention and treatment of dental caries is to prevent disturbance of or to re-establish a healthy microbial homeostasis [3]. Clinical studies have indicated that in the dental biofilms high numbers of non-mutans streptococci, such as Streptococcus sanguinis and Streptococcus gordornii, were often associated with low numbers of cariogenic bacteria Streptococcus mutans and this association was mostly observed in healthy subjects, while the inverse was typically found in subjects with caries [5,6]. These findings have emphasised the potential of caries prevention via modulating oral microbial ecology.

Among the commensal oral non-mutans streptococci, Streptococcus oligofermentans has several interesting traits. It was frequently isolated from caries-free subjects or healthy non-carious tooth surfaces [7,8]. It produced less acid from glucose than S. mutans [8] and inhibited the growth of S. mutans [9]. With molecular techniques, Tong et al [9] demonstrated that S. oligofermentans inhibited the growth of S. mutans through the production of hydrogen peroxide (HP) both in suspensions and in biofilms. S. oligofermentans employs three types of enzymes, pyruvate oxidase (POX), lactate oxidase (LOX) and L-amino acid oxidase, to produce HP [9,10,11]. The synergistic action of POX and LOX maximized the HP production of S. oligofermentans [10]. The ability of S. oligofermentans producing HP from lactic acid is particularly interesting, since lactic acid is the major organic acid produced by dental biofilms. This trait of S. oligofermentans may provide dual benefits: minimising pH drop by converting lactic acid into HP and inhibiting the cariogenic bacteria S. mutans through HP production. Therefore, S. oligofermentans may be a good probiotic candidate for maintaining healthy oral microflora.

Although several studies have reported that S. oligofermentans could inhibit the growth of S. mutans in a dual-species biofilm [8,10,11], some characteristics of the biofilm model used in these studies may limit the clinical relevance of their findings: firstly, the studied biofilms were “bottom-biofilms”. These biofilms mostly contain sedimented cells, which are not incorporated by active attachment, while active attachment is a prerequisite for oral biofilm formation. Secondly, the pH in the bottom-biofilm model was unknown and not controlled. Environmental factors, such as the presence of oxygen, sugar availability and pH, were shown to greatly affect the HP production of S. oligofermentans, thereby its inhibition on the growth of S. mutans [12,13]. A previous study demonstrated that the inhibitory effect of S. oligofermentans on S. mutans decreased with the decreasing pH value. At pH 5.5, no interaction between two species was observed in the agar competition assay [12]. Since S. mutans was known to be aciduric and to be able to outcompete other bacterial species at cariogenic condition (pH 5.5), the above findings seemed to suggest the limitations of S. oligofermentans in maintaining healthy microflora at cariogenic conditions. As only planktonic cultures were tested in the previous study, it is relevant to re-evaluate the influence of pH in a biofilm model that allows bacterial active attachment.

The aims of this study are to establish a pH-controllable active-attachment biofilm model and to explore the competition between S. mutans and S. oligofermentans in biofilms under two different pH conditions, constantly neutral pH and pH-cycling. The pH-cycling included a period of 8 h at neutral pH and a period of 16 h at pH 5.5, with the intention to mimic cariogenic conditions that dental biofilms often encounter.

Materials and Methods

Bacterial strains and growth conditions

The strains used in this study were Streptococcus mutans UA159 and Streptococcus oligofermentans LMG22279 [7]. Both bacterial strains were grown anaerobically (90% N2, 5% CO2, 5% H2) at 37°C. Biofilms were grown in a modified semi-defined biofilm medium (BM), which contains 10 mM (NH4)2SO4, 35 mM NaCl, 2 mM MgSO4·7H2O and was supplemented with filter-sterilised vitamins (0.04 mM nicotinic acid, 0.1 mM pyridoxine HCl, 0.01 mM pantothenic acid, 1 μM riboflavin, 0.3 μM thiamine HCl, and 0.05 μM D-biotin), amino acids (4 mM L-glutamic acid, 1 mM L-arginine HCl, 1.3 mM L-cysteine HCl, and 0.1 mM L-tryptophan), and 0.3% (wt/vol) yeast extract [14].

To prepare BM of pH 7.0, 76 mM K2HPO4 and 15 mM KH2PO4 were added to the medium. To prepare BM of pH 5.5, 30 mM MES buffer was added to the medium. For pre-cultures, BMG was prepared by adding 0.4% of glucose to BM and for biofilm growth, BMS was prepared by adding 0.2% of sucrose to BM. This sucrose concentration was chosen because it could promote biofilm formation without causing pH changes.

Biofilm growth

Biofilms were grown in an active attachment model [15]. This model consists of a standard 96-well microtiter plate and a lid with an identical number of polystyrene pegs that fit into wells (Nunc, Roskilde, Denmark). This model was chosen to examine exclusively the actively adhered biofilms, instead of bacterial sedimentation in the 96-well microtiter plate, and to retain the 96-well high-throughput advantage for testing multiple variables. Single or dual-species biofilms were grown for 48 h before further analysis. In detail, to grow single-species biofilms, overnight (16 h) S. mutans and S. oligofermentans cultures in BMG were diluted to a final OD600nm of 0.04 in fresh BMS (pH 7.0) and 200 μl of each cell suspension was dispensed into a 96-well plate. To grow dual-species biofilms, the overnight cultures of each strain were diluted to a final OD600nm of 0.08 in BMS (pH 7.0) and mixed at 1:1 ratio before dispensing 200 μl into the 96-well plate. This mixture contains 4.6 x 106 (± 2.7 x 106) CFU/ml of S. mutans and 1.7 x 107 (± 7.4 x106) CFU/ml of S. oligofermentans. The plate was then covered with the lid containing pegs and incubated for 8 h. Thereafter, the pegs were rinsed with sterile distilled water to remove non-adherent bacterial cells. After rinsing, half of the pegs were inserted in BMS of pH 7.0, while the other half was inserted in BMS of pH 5.5, and both were further incubated for 16 h. Subsequently all pegs were rinsed with sterile distilled water and inserted again in BMS of pH 7.0. After another 8 h incubation, the pegs were inserted in either BMS of pH 7.0 or BMS of pH 5.5 for another 16 h. The 48 h biofilms formed on the pegs were collected for viable cell counts and were examined for their capability to produce lactic acid and HP. The schema of biofilm growth is illustrated in Fig 1.

In each experiment, a total of 6 groups (single-/dual-species groups, grown under neutral pH or pH-cycling condition) were tested. Each group generally contained 8 biofilms replicates. Four replicates were used for viable cell counts and four were used for the measurement of lactic acid and HP production. The experiment was repeated 3 times.

Viable cell counts

Each individual peg with biofilms was carefully cut off with a sterile scalpel without disturbing the biofilms and placed in 1ml CPW (5 g yeast extract, 1 g peptone, 8.5 g NaCl, 0.5 g L-cysteine hydrochloride per liter, adjusted to pH 7.3). Biofilms were dispersed by sonication on ice 60 times for 1 s at an amplitude of 40 W (Vibra cell, Sonics & Materials Inc., USA). Undiluted samples or serially diluted samples (100 μl) were plated onto Brain Heart Infusion (BHI) agar plates. The plates were incubated for 3 d. The colonies were counted and recorded as Colony Forming Unit (CFU). Since the morphologies of S. mutans and S. oligofermentans were distinct on BHI agar plates, the CFUs of S. mutans and S. oligofermentans in the dual-species biofilm samples were recorded separately based on the colony morphology. The images of the colonies are provided in S1 and S2 Figs. The detection limit of this viable cell count method is 100 CFU per sample.

HP and lactic acid quantification

The capability of HP and lactic acid production of 48 h biofilms was examined by inserting the pegs with biofilms into a 96-well plate, filled with 200 μl per well buffered assay medium (pH 7.0) at 37°C for 4 h. The assay medium contained most of the components of BM except yeast extract, since no further biofilm growth was desired during the incubation. Glucose (1%) was added to the assay medium in order to trigger lactic acid production. After incubation, 50 μl assay medium was immediately used for HP measurement. The rest of the medium was stored at -20°C for lactic acid quantification.

HP was quantified by an enzymatic assay with modifications [16]. In detail, 50 μl of culture medium was added to 45 μl of solution containing 2.5 mM 4-aminoantipyrine (4-amino-2, 3-dimethyl-1-phenyl-3-pyrazolin-5-one; Sigma-Aldrich, St. Louis, MO, USA) and 0.17 M phenol in a 96-well plate. This reaction mixture was incubated for 5 min at room temperature; thereafter horseradish peroxidase (Sigma-Aldrich, St. Louis, MO, USA) was added at a concentration of 640 mU ml-1 in 0.2 M potassium phosphate buffer (pH 7.2). After 4 min, the absorbance was recorded at 510 nm in a spectrophotometer (Perkin Elmer, Norwalk, CT, USA). HP concentration of each sample was calculated from a standard curve generated with known concentrations of HP (Sigma-Aldrich, St. Louis, MO, USA).

Lactic acid was measured with an enzymatic-spectrophotometric method [17]. The principle of the method is based on the enzymatic conversion of L-lactate to pyruvate with concomitant conversion of NAD to NADH, the increase in absorbance at 340 nm being proportional to NADH formation.

HP production of S. oligofermentans suspension cells at pH 7.0 or pH 5.5

To understand how environmental pH influenced the ability of HP production of S. oligofermentans, we chose to carry out the experiment on suspension cells since these cells were more homogenous and better controlled than the biofilm cells. Overnight S. oligofermentans culture grown in BMG (pH 7.0) was centrifuged and resuspended in either BM pH7.0 or BM pH5.5, without any addition of sucrose. The cell density was adjusted to an OD600nm of 0.9. The resuspensions were incubated anaerobically for either 4 or 16 h. The ability of these suspension cells to produce HP was examined in the same way as the biofilms were tested. In detail, the resuspensions were centrifuged, incubated in the buffered assay medium for 4 h. The supernatants were used for HP quantification (the procedure is described above). The S. oligofermentans cells before and after 4 or 16 h of incubation were also subjected to viable cell counts. This experiment was repeated 3 times. Duplicate samples per group were included in each experiment.

Statistical analysis

The data were analysed with the Statistical Package for Social Science (SPSS, Version 17.0, Chicago, IL, USA). One-way ANOVA was used to evaluate the differences in CFU, HP and lactic acid concentration between single- and dual-species biofilms. Specifically, independent-samples t test was used to examine the influence of pH (neutral pH vs. pH-cycling) on the variables. The CFU counts were log transformed before the statistical tests. p<0.05 was considered significant.


Viable cell counts of single- and dual-species biofilms

Both S. mutans and S. oligofermentans were able to form biofilms alone and together in the presence of 0.2% sucrose. At every refreshment point the pH of the spent medium was monitored. After 16 h incubation, the pH of phosphate buffered biofilm medium (pH7.0) had remained constant, but the pH of MES buffered medium (pH 5.5) dropped 0.5 unit.

Fig 2 displays the CFU counts of single- and dual-species biofilms. Compared to constantly neutral pH condition, pH 7.0–5.5 cycling condition generally lead to one log reduction in the total cell counts of 48 h biofilms. The presence of S. oligofermentans in dual-species biofilms significantly suppressed the growth of S. mutans. The cell counts of S. mutans dropped from 106 CFU/peg in single-species biofilms to 103 CFU/peg in dual-species biofilms at constantly neutral pH, and dropped from 105 CFU/peg to under the detection limit (102 CFU/peg) at pH-cycling conditions. However, the presence of S. mutans in dual-species biofilms did not seem to affect S. oligofermentans cell counts at tested pH conditions. The number of S. oligofermentans viable cells in dual-species biofilms was similar to that in single-species biofilms at either tested pH.


Fig 2. Viability of single-species and dual-species 48 h biofilms.

Biofilms were grown under constantly neutral pH or pH-cycling (8 h pH 7.0 and 16 h pH 5.5) conditions. The viability of the biofilms was evaluated by CFU counts. A. Viable cell counts of S. mutans biofilms. Single Sm: S. mutans single-species biofilms; Dual Sm: S. mutans counts in dual-species biofilms. B. Viable cell counts of S. oligofermentans biofilms. Single So: S. oligofermentans single-species biofilms; Dual So: S. oligofermentans counts in dual-species biofilms. The dash line indicates the detection limit. Four replicates were used for viable cell counts in each experiment. The experiment was repeated 3 times. * indicates the significant difference between Single Sm and Dual Sm, p < 0.05.

Lactic acid concentration of single- and dual-species biofilms

The growth pH conditions affected only the lactic acid concentration of single-species S. mutans biofilms (Fig 3). The pH-cycling condition, compared to neutral pH condition, significantly reduced lactic acid production of single-species S. mutans biofilms (p<0.05). The lactic acid concentration in dual-species biofilms was significantly lower than that in single-species S. mutans biofilms. The reduction was around 12-fold under constantly neutral pH and 2.7-fold under pH-cycling condition. Similar level of acid concentration was observed in dual-species and single-species S. oligofermentans biofilms.


Fig 3. Lactic acid concentration of single-species and dual-species 48 h biofilms.

Biofilms were grown under constantly neutral pH or pH-cycling conditions. Before quantification of lactic acid concentration, the biofilms were incubated in the assay medium (pH 7.0), supplemented with 1% glucose for 4 h. Single Sm: S. mutans single-species biofilms; Single So: S. oligofermentans single-species biofilms; Dual: dual-species biofilms. Four replicates were used for lactic acid quantification in each experiment. The experiment was repeated 3 times. * indicates the significant difference between Single Sm and the other two groups (Single So and Dual), p < 0.05.

HP production of single- and dual-species biofilms

No HP production was measured for single-species S. mutans biofilms. We also examined the suspension cells of S. mutans UA159 grown in either BHI or BMS (pH 7.0) and found no HP production. This experiment was performed twice with duplicate samples (data not shown). Therefore HP in the biofilms was produced by S. oligofermentans alone (Fig 4). There were no differences in HP production between dual-species and single-species S. oligofermentans biofilms. The HP production in the biofilms grown at the pH-cycling condition was 2-fold higher than those in the biofilms grown at constantly neutral pH.


Fig 4. Hydrogen peroxide (HP) production of single-species and dual-species 48 h biofilms.

Biofilms were grown under constantly neutral pH or pH-cycling conditions. The HP production was quantified after the biofilms were incubated in the assay medium (pH 7.0), supplemented with 1% glucose for 4 h. Single So: S. oligofermentans single-species biofilms; Dual: dual-species biofilms. Four replicates were used for HP production in each experiment. The experiment was repeated 3 times. * indicates the significant difference between constantly neutral pH and pH-cycling conditions, p < 0.05.

HP production by S. oligofermentans suspension cells

To further explore if the increased HP production of S. oligofermentans under the pH-cycling condition was stress-related, we measured HP production of S. oligofermentans suspension cells after they were incubated in a buffer of pH 7.0 or pH 5.5 for 4 or 16 h. Table 1 shows that the CFU counts significantly dropped after incubating the cell suspension in a buffer of pH 5.5 for 16 h. No changes in CFU counts were observed under other incubation conditions. The S. oligofermentans suspension cells incubated in a buffer of pH 5.5 for 16 h demonstrated the highest potential of producing HP. As a result, the amount of HP produced per viable cell under this condition was about 15-fold higher than those incubated under other conditions.


In the oral cavity, the retention sites of the teeth, such as fissures and approximal sites, are prone to caries. The pH of dental biofilms at these sites drops rapidly upon intake of carbohydrates and can remain below pH 5.5 for a substantial period of time [18]. The prolonged low pH condition favours the aciduric bacterial species, such as cariogenic mutans streptococci and lactobacilli, which are able to survive and grow under this adverse condition [3,4]. Acid tolerance is considered the virulence trait for cariogenic bacteria to outcompete other microbes in dental biofilms. In this study, the competition between the cariogenic S. mutans and the commensal S. oligofermentans in dual-species biofilms was examined under either a constantly neutral pH or a pH-cycling condition (with a 16 h low pH period) in an active attachment biofilm model. Our data demonstrated that S. oligofermentans strongly inhibited the growth of S. mutans in dual-species biofilms and reduced lactic acid concentration at not only neutral pH condition, but also the pH-cycling condition. The inhibition of S. oligofermentans on the growth of S. mutans in dual-species biofilms has been reported in previous studies [8,10,11]. What is new in our finding is that the biofilms were formed through an active attachment process, while the previous studies formed the biofilms at the bottom of the wells. Since S. mutans is known to adhere better to a surface than other streptococci under sucrose condition, one could question if S. oligofermentans was still able to suppress S. mutans in the actively attached biofilms. The data from this study provided a positive answer to the question. Moreover, a recent study found that a low pH environment (pH<6.0) affected the ability of S. oligofermentans to inhibit the growth of S. mutans [12]. This result is contradictory to what we reported here. The discrepancy in these two studies might be explained by the experimental design. In the study of Liu et al. [12], the competition between two species was only tested on agar plates with various pH levels. Therefore, the growth of both bacterial species (S. mutans and S. oligofermentans) was affected by the constantly low pH, which made the competition between these two species impossible to observe. In our study, the oscillation of pH between 7.0 and 5.5 allowed the growth of both bacterial species. This design mimics the clinical condition better and makes it possible to study the competition between both species. Overall, our finding implied that S. oligofermentans might be a compelling probiotic candidate to compete against cariogenic bacterial species at sites prone to caries.

S. mutans is known to be acid tolerant. Previously, a panel of oral streptococci was tested for their acid tolerance [1921]. All S. mutans strains were more aciduric than tested non-mutans streptococci, like S. sanguinis. Although substantial evidence has indicated that S. sanguinis and S. gordonii were capable of inhibiting the growth of S. mutans, these results were mostly achieved at a neutral pH environment. When a multi-species community was incubated under prolonged low pH condition, S. mutans would be favoured while S. sanguinis and S. gordonii would be suppressed [14,22]. S. gordonii was once tested as a probiotic for its inhibition on the growth of S. mutans in a rat caries model [23]. But S. mutans was found to overgrow S. gordonii, irrespective of the availability of sucrose and inoculation sequences. Therefore, S. sanguinis and S. gordonii may not be a good probiotic candidate to inhibit S. mutans at caries susceptible sites. The data presented here suggested that unlike S. sanguinis and S. gordonii, S. oligofermentans could inhibit S. mutans even after co-incubation at low pH for 16 h. This trait was indicated by the relatively high CFU counts of single-species S. oligofermentans biofilms under pH-cycling condition. It seems that S. oligofermentans is as acid resistant as S. mutans, since a similar level of CFU reduction was observed for both bacterial species when comparing pH-cycling condition with neutral pH condition.

Another intriguing finding of this study was the enhanced HP production of S. oligofermentans biofilms after growth under pH-cycling conditions. This was unexpected since the number of viable S. oligofermentans cells grown under pH-cycling conditions was much lower than of those grown under neutral pH conditions. There are a few possible explanations. The first one is that the presence of S. mutans in dual-species biofilms might trigger the HP production under pH-cycling conditions. But it could not explain why the HP production in single-species S. oligofermentans biofilms was as high as dual-species biofilms. The second explanation is that the high HP production was caused by the high lactate concentration, since S. oligofermentans is able to convert lactate into HP [9]. This assumption could explain the low lactate concentration observed in S. oligofermentans biofilms. But it could not explain why lactate concentration in S. oligofermentans biofilms was similar under both pH conditions, while HP production was different. The third explanation is related to the plating method used in this study. Since this method cannot detect those viable but not culturable bacterial cells, the unculturable S. oligofermentans cells in the biofilms might be the reason for the high HP production. We have carried out the metabolism (resazurin) assay to examine the metabolic activity of the tested biofilms, besides plating. This assay is able to detect viable bacterial cells without the requirement of further culturing. The results obtained from the assay were consistent with the results obtained from the plating method (data not shown). The fourth explanation is that the prolonged low pH incubation triggered the stress response of S. oligofermentans cells and resulted in enhanced HP production after the bacterial cells were incubated at neutral pH again. To explore this assumption, we carried out an additional experiment on S. oligofermentans suspension cells. Our data indicated 16 h, but not 4 h, mild acid pre-challenge could indeed increase the HP production per S. oligofermentans cell, even though the overall HP increase was not as pronounced as in biofilms.

In this study, we successfully established a high-throughput pH-cycling biofilm model. In order to establish a controllable pH-cycling condition, different buffers (phosphate or MES buffer) were added to the growth media. As a result, the pH of the biofilms could be maintained as designed. Since dental biofilms in the oral cavity constantly experience pH fluctuations, the established model can mimic this fluctuation condition and help to understand its influence on the bacterial interaction in dental biofilms. On the other hand, we also realized that the presented biofilm model, though well controlled, is too simple to fully mimic the complex oral conditions. Several important factors, such as dental hard tissues as substrata, salivary buffering, salivary flow or a multi-species community, should be taken into account in the model in the future studies. Eventually, the feasibility of S. oligofermentans as a probiotic under cariogenic condition should be evaluated in a more realistic model, such as an animal model.

In summary, the data presented here indicated that the non-mutans streptococci S. oligofermentans not only have the reported properties, including low acidogenic and being an HP producer, but also is aciduric and able to produce a substantial amount of HP after substantial acid challenge in the biofilms. These traits make S. oligofermentans the most competent candidate to compete against cariogenic bacteria S. mutans in vivo.

Author Contributions

Conceived and designed the experiments: XDB JJDS XJG CVL DMD. Performed the experiments: XDB LBH DMD. Analyzed the data: XDB JJDS CVL DMD. Contributed reagents/materials/analysis tools: XDB HCT CVL DMD. Wrote the paper: XDB HCT JJDS CVL DMD.


  1. 1.
    Aas JA, Paster BJ, Stokes LN, Olsen I, Dewhirst FE (2005) Defining the normal bacterial flora of the oral cavity. J Clin Microbiol 43: 5721–5732. pmid:16272510
  2. 2.
    Marsh P (1994) Microbial ecology of dental plaque and its significance in health and disease. Advances in dental research 8: 263–271. pmid:7865085
  3. 3.
    Marsh PD (2006) Dental plaque as a biofilm and a microbial community–implications for health and disease. BMC Oral health 6: S14. pmid:16934115
  4. 4.
    Nyvad B, Crielaard W, Mira A, Takahashi N, Beighton D (2013) Dental caries from a molecular microbiological perspective. Caries Res 47: 89–102. pmid:23207320
  5. 5.
    Becker MR, Paster BJ, Leys EJ, Moeschberger ML, Kenyon SG, Galvin JL, et al. (2002) Molecular Analysis of Bacterial Species Associated with Childhood Caries. Journal of Clinical Microbiology 40: 1001–1009. pmid:11880430
  6. 6.
    Berkowitz RJ (2003) Causes, treatment and prevention of early childhood caries: a microbiologic perspective. Journal-Canadian Dental Association 69: 304–307. pmid:12734024
  7. 7.
    Tong H, Gao X, Dong X (2003) Streptococcus oligofermentans sp. nov., a novel oral isolate from caries-free humans. International Journal of Systematic and Evolutionary Microbiology 53: 1101–1104. pmid:12892133
  8. 8.
    Zhang J, Tong HC, Dong XZ, Yue L, Gao XJ (2010) A preliminary study of biological characteristics of Streptococcus oligofermentans in oral microecology. Caries Res 44: 345–348. pmid:20616551
  9. 9.
    Tong H, Chen W, Merritt J, Qi F, Shi W, Dong X (2007) Streptococcus oligofermentans inhibits Streptococcus mutans through conversion of lactic acid into inhibitory H2O2: a possible counteroffensive strategy for interspecies competition. Mol Microbiol 63: 872–880. pmid:17302806
  10. 10.
    Liu L, Tong H, Dong X (2012) Function of the pyruvate oxidase-lactate oxidase cascade in interspecies competition between Streptococcus oligofermentans and Streptococcus mutans. Appl Environ Microbiol 78: 2120–2127. pmid:22287002
  11. 11.
    Tong H, Chen W, Shi W, Qi F, Dong X (2008) SO-LAAO, a novel L-amino acid oxidase that enables Streptococcus oligofermentans to outcompete Streptococcus mutans by generating H2O2 from peptone. J Bacteriol 190: 4716–4721. pmid:18469105
  12. 12.
    Liu Y, Chu L, Wu F, Guo L, Li M, Wang Y, et al. (2014) Influence of pH on inhibition of Streptococcus mutans by Streptococcus oligofermentans. Eur J Oral Sci 122: 57–61. pmid:24267570
  13. 13.
    Liu Y, Wu L, Wu F, Chu L, Liu X, Xia K, et al. (2012) Interspecies competition and inhibition within the oral microbial flora: environmental factors influence the inhibition of Streptococcus mutans by Streptococcus oligofermentans. Eur J Oral Sci 120: 179–184. pmid:22607333
  14. 14.
    Bradshaw D, Marsh P, Hodgson R, Visser J (2002) Effects of glucose and fluoride on competition and metabolism within in vitro dental bacterial communities and biofilms. Caries research 36: 81–86. pmid:12037363
  15. 15.
    Li X, Hoogenkamp MA, Ling J, Crielaard W, Deng DM (2013) Diversity of Streptococcus mutans strains in bacterial interspecies interactions. J Basic Microbiol 54: 97–103. pmid:23456658
  16. 16.
    Seki M, Iida K-i, Saito M, Nakayama H, Yoshida S-i (2004) Hydrogen peroxide production in Streptococcus pyogenes: involvement of lactate oxidase and coupling with aerobic utilization of lactate. Journal of bacteriology 186: 2046–2051. pmid:15028688
  17. 17.
    Gutmann I, Wahlefeld A, Bergmeyer H (1974) Methods of enzymatic analysis. New York: Academic Press. pp. 1464.
  18. 18.
    Jensen ME, Schachtele CF (1983) Plaque pH measurements by different methods on the buccal and approximal surfaces of human teeth after a sucrose rinse. J Dent Res 62: 1058–1061. pmid:6578234
  19. 19.
    Harper D, Loesche WJ (1984) Growth and acid tolerance of human dental plaque bacteria. Archives of oral biology 29: 843–848. pmid:6594096
  20. 20.
    Bender GR, Sutton S, Marquis RE (1986) Acid tolerance, proton permeabilities, and membrane ATPases of oral streptococci. Infection and immunity 53: 331–338. pmid:3015800
  21. 21.
    Jd Soet, Nyvad B, Kilian M (2000) Strain-related acid production by oral streptococci. Caries Res 34: 486–490. pmid:11093023
  22. 22.
    Bradshaw D, Marsh P (1998) Analysis of pH–driven disruption of oral microbial communities in vitro. Caries research 32: 456–462. pmid:9745120
  23. 23.
    Tanzer JM, Thompson A, Sharma K, Vickerman MM, Haase EM, Scannapieco FA (2012) Streptococcus mutans out-competes Streptococcus gordonii in vivo. J Dent Res 91: 513–519. pmid:22431892
Rate this post