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Article

Mechanism of Action of Streptococcus downii, a New Bacterial Species with Probiotic Potential

by
Lucía Martínez-Lamas
1,
Eliane García-Mato
2,
Anniris Rincón-Quintero
1,
Berta Rivas-Mundiña
2,
Pedro Diz-Dios
2,* and
Maximiliano Álvarez-Fernández
1
1
Clinical Microbiology, Hospital Álvaro Cunqueiro, Complejo Hospitalario Universitario de Vigo, Microbiology and Infectology Group, Galicia Sur Health Research Institute (IISGS), 36212 Vigo, Spain
2
Medical-Surgical Dentistry Research Group (OMEQUI), Health Research Institute of Santiago de Compostela (IDIS), University of Santiago de Compostela (USC), 15782 Santiago de Compostela, Spain
*
Author to whom correspondence should be addressed.
Antibiotics 2023, 12(9), 1472; https://doi.org/10.3390/antibiotics12091472
Submission received: 23 August 2023 / Revised: 12 September 2023 / Accepted: 20 September 2023 / Published: 21 September 2023
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Abstract

:
Streptococcus downii is a recently reported bacterial species of oral origin, with inhibitory capacity against Streptococcus mutans, Actinomyces naeslundii, Veillonella parvula and Aggregatibacter actinomycetemcomitans, which confers upon it the potential of being an oral probiotic. The aim of the present study was to identify the potential mechanisms by which S. downii exerts its inhibitory effect on S. mutans. To this end, the study assessed the consumption of glucose and proteins available in the culture medium, the modification of the pH, the production of short-chain fatty acids, the changes in the protein panel of the inhibition halo, the production of hydrogen peroxide and the effect of proteinase K. There were no differences in the glucose values or in the protein content of the medium, but there was a reduction in pH (with no effect on the growth of S. mutans). Significant increases were detected in the levels of lactic and formic acid (with no effect on the growth of S. mutans), as well as changes in the peptide panel (with no effect on the growth of S. mutans). The inhibitory effect was maintained in the presence of peroxidase but disappeared after adding proteinase K. Based on these results, it is suggested that the main mechanism of inhibition of S. downii against S. mutans is the production of bacteriocins.

1. Introduction

Analysis of oral microbiota using next-generation sequencing techniques has enabled the identification of differing clusters of microbial communities that are dependent on oral health, thereby suggesting that good oral health corresponds to a combination of innocuous commensal species that make up a stable ecosystem and hinder the growth of pathogenic bacteria [1,2,3]. Any alteration to this homeostasis, which maintains a healthy microbial composition, results in a microbial dysbiosis that can lead to oral diseases such as dental caries and periodontal disease [2]. The strategies for modulating the dental biofilm include promoting the growth of beneficial bacteria by administering pre- and probiotics [4].
Probiotics are living microorganisms that, when administered in the appropriate quantities, are able to produce a health benefit in the host [5]. The use of probiotics is based on bacterial competition processes [6,7,8] that can occur either directly, due to the secretion of bacteriocins, toxins, enzymes or waste products, or indirectly via changes in the environmental pH [6,9]. These microorganisms stimulate cell-mediated immunity, occupy the niches of pathogenic microorganisms and interrupt host–pathogen communication, thereby progressively replacing pathogenic strains [10]. Although the exact mechanism of probiotic activity in the oral cavity is not fully understood, it is considered to be the result of a combination of the local and system immune responses together with other, non-immunological mechanisms [11,12,13].
Streptococcus downii is a new bacterial species initially detected as part of the oral microbiome in a teenager with Down syndrome with no history of dental caries. S. downii has shown inhibitory capacity against Streptococcus mutans, Actinomyces naeslundii, Veillonella parvula and Aggregatibacter actinomycetemcomitans. In a biofilm model, S. downii showed an antibiofilm effect against S. mutans and a significant reduction in S. mutans and Aggregatibacter actinomycetemcomitans counts and significantly reduced the growth of P. gingivalis and V. parvula in well-structured biofilms [14,15].
Given that S. mutans is the main bacterial species involved in the onset and progress of dental caries [16], the aim of this study was to identify the possible mechanism of action by which S. downii exerts its inhibitory effect on S. mutans.

2. Results

2.1. Availability of Carbon Source and Protein Content

A comparison of solubilized agar samples obtained from a plate of S. mutans ATCC (American Type Culture Collection) 25175T prior to culturing S. downii and those obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T showed that the mean protein contents were 6.363 ± 0.110 and 6.640 ± 0.100 mg/mL (p = 0.1), respectively, with a mean glucose content of 6.377 ± 0.070 and 7.620 ± 0.080 g/L (p = 0.1), respectively.

2.2. Modification of Environmental Potential of Hydrogen (pH)

The pH levels detected in distinct growth environments varied between the medium for the S. mutans ATCC 25175T plate with no S. downii and the medium for the inhibition halo generated by S. downii after culture in the presence of S. mutans ATCC 25175T, with mean pH values of 6.667 ± 0.321 and 5.500 ± 0.200 (p = 0.1), respectively.
To determine whether this acidification was responsible for the growth inhibition of S. mutans ATCC 25175T, the growth ability of this bacterial strain was studied at a pH of 5.5, finding that the decrease in pH was not responsible for the inhibition.

2.3. Organic Acid Production

Table 1 shows the differential production of organic acids in the solubilized agar samples obtained from the S. mutans ATCC 25175T plate before culture with S. downii and those obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T.
Higher levels of lactic (27-fold) and formic acid (10-fold) were detected in the samples obtained from the inhibition halo of S. downii than in those obtained prior to culture with S. downii, although these results did not reach statistical significance. In light of these findings, the direct inhibitory effect of both acids on S. mutans ATCC 25175T was investigated by diluting the acids to various concentrations (formic acid: 0.01, 0.03, 0.06, 0.12 and 0.24 mg/mL; lactic acid: 0.05, 0.10, 0.20, 0.40, 0.80 and 1.6 mg/mL). A combination of 0.24 mg/mL of formic acid and 1.6 mg/mL of lactic acid was also tested. After adding 5 µL of each acid to S. mutans ATCC 25175T and incubating for 17 h, no inhibition was observed at any concentration or after adding the combination of both organic acids. Consequently, the production of short-chain organic acids by S. downii was ruled out as being responsible for the inhibition of S. mutans ATCC 25175T.

2.4. Analysis of Protein Fractionation

Solubilized agar samples collected before culture with S. downii and from the inhibition halo generated after culture thereof with S. mutans ATCC 25175T were analyzed, fractionating the protein content by applying cut-offs with a molecular size of 3 and 10 kDa. The fractionated protein content < 3 kDa was 3.190 ± 0.165 and 2.107 ± 0.200 (p = 0.1), respectively, for both sample types, while the content < 10 kDa was 5.017 ± 0.101 and 3.733 ± 0.208 (p = 0.1), respectively.
Although the growth of S. downii caused changes in the peptide profile, the inhibitory effect was not reproduced when inoculating these fractions directly onto S. mutans ATCC 25175T. Consequently, the presence of peptide compounds in the <3 kDa and <10 kDa fractions produced by S. downii with a potential ability to inhibit S. mutans ATCC 25175T was ruled out.

2.5. Hydrogen Peroxide Production and Proteinase K Test

Figure 1 shows the result of the presence of peroxidase and proteinase K on the inhibitory effect produced by S. downii on S. mutans ATCC 25175T. This inhibitory effect is maintained in the presence of peroxidase but disappears after adding proteinase K, suggesting that inhibition might be caused by a molecule of a peptide-type nature.

2.6. Inhibition of S. mutans by the S. downii Supernatant

Figure 2 shows how the addition of the concentrated S. downii supernatant produces an inhibitory effect against the growth of S. mutans compared with the growth curve obtained when adding the concentrated brain heart infusion (BHI) medium.
In summary, there were no differences in the glucose values or in the protein content of the medium, but there was a reduction in pH (with no effect on the growth of S. mutans). Significant increases were detected in the levels of lactic and formic acid (with no effect on the growth of S. mutans), as well as changes in the peptide panel (with no effect on the growth of S. mutans). The inhibitory effect was maintained in the presence of peroxidase but disappeared after adding proteinase K, suggesting the presence of the inhibitory molecules in the S. downii supernatant. Figure 3 summarizes all the experiments performed to study the mechanism of S. downii inhibition of S. mutans as well as the results.

3. Discussion

The known mechanisms by which probiotics inhibit and/or interfere with other bacterial populations include pH modification, the production of antimicrobial compounds, competition for binding sites and/or nutrients and the stimulation of immunomodulatory cells [17].
Given that the binding of microorganisms to the tooth surface represents the first step in the pathogenesis of dental caries, competition during this adhesion process as a result of bacterial adhesion is one of the key mechanisms of action for oral probiotics [18]. Indeed, in vitro studies have shown the ability of various species of the genus Streptococcus to inhibit the colonization of epithelial cells by A. actinomycetemcomitans [19]. Similarly, S. mitis inhibits the adhesion of Porphyromonas gingivalis to gingival epithelial cells [20], and S. dentisani inhibits the growth of periodontal pathogens by way of adherence, competition and displacement mechanisms [21].
Bacterial competition for the available substrates is another possible inhibition mechanism. Bifidobacterium spp. has been observed to interrupt the growth of P. gingivalis by reducing the essential nutritional factors available in the environment [15].
The production of alkaline substances might prevent growth of the pathogens responsible for dental caries and alter the chemical equilibrium in favor of tooth remineralization. Somewhat paradoxically, the production of organic acids, such as lactic and acetic acid, causes a decrease in pH as the non-dissociated form of the acid enters the bacterial cell, where it dissociates in the cytoplasm, thereby acidifying the medium. This intracellular build-up of the ionized form of the acid could itself cause the death of the potential pathogen [22,23].
Another mechanism exhibited by oral commensal streptococci and that affects the ecosystem of the oral biofilm due to its inhibitory effect on certain microorganisms is the production of hydrogen peroxide (H2O2) from lactic acid, thereby minimizing the decrease in pH. H2O2 inhibits the growth of S. mutans and numerous other oral pathogens at concentrations that do not markedly affect the producing strains [24]. Lactic acid bacteria produce various antimicrobial agents, including organic acids, H2O2, low molecular weight antimicrobial peptides, bacteriocins and adhesion inhibitors [25,26]. Polonskaia [27] was the first author to claim that Lactobacillus acidophilus might inhibit the growth of other bacteria. Specifically, Lactobacilli from the strain GG produce organic acids, H2O2, carbon dioxide, diacetyl, low molecular weight antimicrobial peptides, bacteriocins and adhesion inhibitors against Streptococcus spp. and can therefore be considered a potent probiotic [28]. S. sanguinis, which is a H2O2 producer, has been found to suppress the growth of A. actinomycetemcomitans in vitro and to antagonize the colonization thereof in gnotobiotic rats [29]. Similarly, Tong et al. and Bao et al. showed that S. oligofermentans inhibits the growth of S. mutans by producing H2O2, both in suspension and in biofilm studies [30,31]. Streptococcus A12 also inhibits growth and intercellular signaling in S. mutans and can exert a buffer effect by modifying the pH via the arginolytic pathway [32].
However, the percentage contribution of lactic acid and other organic acids to the antibacterial activity of lactic acid bacteria has been estimated at less than 50% [33]. Terai et al. showed that Lactobacillus spp. isolates conserved some antibacterial activity after being neutralized by these acids, suggesting that the isolates produce bacteriocins or other antibacterial substances [34]. Indeed, bacteriocins have been isolated from certain Lactobacillus spp., such as salivaricin from L. salivarius [35], reuterin and reutericyclin from L. reuteri [36] or plantaricin from a strain of L. plantarum [37]. Reuterin is a broad-spectrum antimicrobial agent that can inhibit the growth of Gram-positive and Gram-negative bacteria, including oral pathogens such as S. mutans, A. actinomycetemcomitans, Prevotella intermedia and Fusobacterium nucleatum [38]. A strain of S. mutans (JH1001) that produces a bacteriocin, namely mutacin 1140, which inhibits the growth of a wide range of bacteria, including Streptococcus spp., Actinomyces spp. and Lactobacillus spp. in vitro, has been isolated [39,40,41]. Previously, the genome for the JH strain of S. salivarius has been shown to contain the biosynthetic loci for the bacteriocins salivaricin A3 and E, streptin, and streptococcin SA-FF22; this strain also produces the bacteriocin zoocin A, which, in combination with the preparation of dextranase, exhibited potent anti-S. mutans activity [42]. The strain S. salivarius K12, in turn, produces salivaricin, which is mainly responsible for its potential as an oral probiotic [43]. Similarly, the probiotic S. salivarius M18 produced bacteriocins that antagonize the acidogenic activity of S. mutans. When this strain colonizes the human oral mucosa, it produces dextranase and urease, which can counteract plaque formation and the acidity of saliva, respectively [44]. S. dentisani, in turn, metabolizes arginine and produces bacteriocins to exert its oral probiotic effect [45,46].
In light of the above, we can consider at least three mechanisms by which S. downii exerts its probiotic action: competition for the binding site to oral tissues and/or nutrients, the production of antimicrobial agents and/or bacteriocins and modification of the host’s immune response. Given that the experiments in this study were performed in vitro, we were unable to demonstrate a role for immunomodulation in the inhibitory effect observed.
No major differences in nutrient content were detected for the solubilized agar samples obtained from the S. mutans ATCC 25175T plate prior to culture with S. downii and those obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T. It therefore appears unlikely that S. mutans inhibition is the result of competition for the substrate or a depletion of nutrients. Although differences in terms of pH were observed after culture with S. downii, the effect thereof on the growth of S. mutans was ruled out in subsequent studies. A marked increase in the levels of lactic acid and formic acid was detected in the samples obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T compared with the solubilized agar samples obtained from the S. mutans ATCC 25175T plate prior to culture with S. downii. However, neither of these two acids exhibited a direct inhibitory effect on S. mutans. H2O2 production was also ruled out as a mechanism for bacterial antagonism, given that the inhibitory effect remained unchanged after adding peroxidase.
Given that inhibition in the in vitro tests occurred after pre-growth of the strain, S. downii either produces a metabolite that diffuses through the agar or modifies the medium, thereby favoring S. mutans inhibition. Consequently, the most likely option to explain the inhibitory effect observed is the production of antimicrobial substances of a peptide-type nature, which can diffuse freely through the agar, thereby inhibiting the growth of susceptible strains [14]. The likelihood that the inhibitory molecules are peptidic in nature is strengthened by the fact that the inhibitory effect was significantly reduced upon treatment with proteinase K [47].
Based on the results and given that a significant number of Streptococcus spp. isolates were shown to be bacteriocin-producing [48], class IIb bacteriocins have been identified in the genomes of Streptococcus pyogenes [49], Streptococcus MIA (M 18) [50] and S. dentisani [51], among others. In this sense, it has been pointed out that the genomic analysis of S. downii has revealed the presence of putative genes of the family of bacteriocin IIb lactobinA/cerein 7B [52]. A comparative genomics study of S. downii to detect the presence of these genes related to the production of bacteriocins would confirm the study’s findings. Moreover, it is essential to isolate the bacteriocin through the concentrated supernatant, similar to the study by Conrads et al. with S. dentisani [51].

4. Materials and Methods

4.1. Inhibition of S. mutans by S. downii

A 0.3 McFarland suspension of S. mutans ATCC 25175T was prepared on BHI plates to obtain a carpet-type growth. A 10-µL aliquot of S. downii was deposited on each plate in the form of a button after completing growth in pure culture for 24 h. S. mitis ATCC 49456T and S. salivarius ATCC 7073T were used as negative controls, and S. dentisani CECT 7747T was used as a positive control. The plates were incubated at 35–37 °C in an aerobic atmosphere for 24 h. The inhibitory capacity versus S. mutans ATCC 25175T was confirmed at 48 h by the presence of inhibition haloes. The test was performed in triplicate.

4.2. Inhibition of S. mutans by the S. downii Supernatant

To obtain the concentrated supernatant, we inoculated several colonies of S. downii in 50 mL of brain heart infusion broth (BHI, Bd) incubating at 37 °C for 48 h in an aerobic atmosphere. After incubation, the mixture was centrifuged at 4000 rpm for 10 min, discarding the pellets. The supernatant was passed through filters (pore size of 0.2 μm) (Millipore) and concentrated in a Rotavapor (rotary evaporator) 10 times. The resulting 5 mL was once again passed through filters (pore size of 0.2 μm) (Millipore) and stored at −20 °C until its use.
The supernatant’s inhibitory activity was determined by measuring the absorption at 610 nm in an automated microplate reader, incubating the sample at 37 °C for 14 h and recording the absorption every 30 min. To this end, we diluted S. mutans with BHI medium until an optical density of 0.1 was achieved. We then mixed 160 μL of the S. mutans suspension with 40 μL of the concentrated S. downii supernatant. As a negative control, we mixed 160 μL of the S. mutans suspension with 40 μL of concentrated BHI 10 times. The experiment was repeated 3 times.

4.3. Availability of Carbon Source and Protein Content

To confirm that the inhibition of S. mutans ATCC 25175T did not occur as a result of the consumption of glucose or proteins present in the medium by S. downii, agar samples (some lacking S. downii and others from the inhibition halo region that appears in the plate tests after culturing S. downii for 17 h) were collected, solubilized and analyzed. Glucose was analyzed using the biochemical kit K-GLUHK (Megazyme, Bray, Ireland). Proteins were analyzed using a Pierce BCA Protein Assay Kit (Thermo Scientific, Rockford, IL, USA).
The agar solubilization protocol was performed as described previously with minor modifications [53]. Using a set of parallel blades, we obtained 3 strips (measuring 5mm × 5 mm) of BHI agar from the S. mutans plaque before culture with S. downii and from the inhibition halo generated by the co-culture of both species. Each fragment of agar medium was added to 1.5 mL of double-distilled sterile water and melted in a bath at 85–90 °C for 3 min (the agar’s melting temperature). We then measured the resulting volume to be able to adjust the calculations according to the dilution factor obtained in each case. We used as copies equidistant fragments of the S. mutans plaque before culture with S. downii and those obtained from the inhibition halo generated by the co-culture of both species.

4.4. Modification of Environmental pH

To study whether pH modification of the medium caused by the growth of S. downii affected the growth of S. mutans ATCC 25175T, agar samples were taken, solubilized in a similar manner to those used in the nutrient-consumption experiments at various growth points and in the inhibition zone generated, and analyzed to detect any differences in terms of pH.

4.5. Organic Acid Production

Certain short-chain organic acids, such as succinic, lactic, formic, acetic, propionic, isobutyric, butyric, isovaleric, valeric and caproic, might inhibit the growth of S. mutans ATCC 25175T. To analyze the differential production of these organic acids, two samples of solubilized agar (one with no S. downii and the other from the inhibition halo generated by this microorganism after culture with S. mutans ATCC 25175T) were taken. The organic acids present therein were analyzed by high-performance liquid chromatography coupled to a refractive index detector [54]. The direct action of these acids on S. mutans ATCC 25175T at supposedly inhibitory concentrations was also studied. To that end, the acids were diluted in phosphate-buffered saline (PBS) and a 5-µL aliquot inoculated to S. mutans ATCC 25175T simultaneously.

4.6. Analysis of Protein Fractionation

To evaluate the possible changes in the protein (peptide) profile after the culture of S. downii, the protein content of two solubilized agar samples was analyzed. One sample lacked S. downii, and the other was obtained from the inhibition halo generated after the culture of S. downii together with S. mutans ATCC 25175T. Samples were ultrafiltered on an exclusion column (Amicon, Millipore, Bedford, MA, USA) of 3 and 10 kDa (molecular weight cut-offs), and the protein content was quantified using the Pierce BCA Protein Assay Kit (Thermo Scientific, Rockford, IL, USA). Both protein fractions were also tested directly, adding 5 µL of each while simultaneously inoculating S. mutans ATCC 25175T.

4.7. Hydrogen Peroxide Production and Proteinase K Test

To evaluate the production of H2O2 by S. downii, after incubation in a solid medium for 24 h, 10 μL of peroxidase (64 μg/mL) was added to one side of the colony, and 10 μL of PBS was added to the other. Subsequently, 5 μL of S. mutans ATCC 25175T was inoculated to the right and left sides, as reported previously by other authors [6,55]. S. sanguinis DMSZ (German Collection of Microorganims and Cell Cultures) 20567T was used as a positive control [56], and S. mutans ATCC 25175T was used as a negative control. If S. downii is a H₂O₂-producer, slight effervescence is observed immediately, and no inhibition haloes are observed after 24 h.
To determine whether bacteriocins might be responsible for the inhibition by S. downii, after incubation in a solid medium for 24 h, 10 μL of proteinase K (70 μg/mL; Sigma, St. Louis, MO, USA) was added to one side of the colony, and 10 μL of PBS was added to the other. Subsequently, 5 μL of S. mutans ATCC 25175T was inoculated to the right and left sides, as reported previously by other authors [6,18]. Mutacin-producing S. mutans ATCC 25175T [6] was used as a positive control, and S. sanguinis DMSZ 20567T was used as a negative control. The plates were visualized after incubation at 37 °C for 24 h, and the absence of haloes indicated that inhibition was caused by molecules of a peptide-type nature.

4.8. Statistical Analysis

For the statistical analysis of the experimental data, we employed the statistical package SPSS (SPSS 28.0 for Windows, SPSS Ltd., Surrey, United Kingdom). Due to the non-normal distribution, the differences between the mean values were assessed using the nonparametric Mann–Whitney U test. Significance was established for p ≤ 0.05. All experiments have been repeated 3 times, and we agree that the statistical power of 3 samples is very weak, and therefore these results should be interpreted with extreme caution.

5. Conclusions

The results of this study show that the mechanism of action by which S. downii exerts its inhibitory effect on S. mutans is not regulated by the consumption of glucose and proteins available in the culture medium, the change in pH, the production of short-chain fatty acids, the changes in the inhibition halo’s protein panel or the production of hydrogen peroxide. Consequently, and given that the inhibitory effect disappeared after adding proteinase K, these results allow us to speculate that the most likely mechanism by which S. downii exerts its inhibitory action on certain oral pathogenic bacteria is the production of antimicrobial substances of a peptide nature.

Author Contributions

Conceptualization, M.Á.-F. and P.D.-D.; methodology, M.Á.-F., B.R.-M. and L.M.-L.; formal analysis, L.M.-L. and A.R.-Q.; investigation, E.G.-M. and L.M.-L.; writing—original draft preparation, L.M.-L. and B.R.-M.; writing—review and editing, M.Á.-F., E.G.-M. and P.D.-D.; supervision, A.R.-Q. and P.D.-D.; project administration, A.R.-Q. and E.G.-M.; funding acquisition, B.R.-M. and L.M.-L. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by project IN855A-2016/36 financed by the Xunta de Galicia under the Resolution of the Galician Innovation Agency of 12 August 2016 (Ignicia Program); project I4TRANSF financed by the Galician Agency for Knowledge Management in Health (PRIS3 Program); project 00-00002474-16 financed by the Foundation for Innovation and Foresight in Health in Spain (FIPSE); and project DTS22/00056 funded by Instituto de Salud Carlos III (ISCIII) and co-funded by the European Union.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The data are available upon request to the corresponding author.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Belda-Ferre, P.; Alcaraz, L.D.; Cabrera-Rubio, R.; Romero, H.; Simon-Soro, A.; Pignatelli, M.; Mira, A. The oral metagenome in health and disease. ISME J. 2012, 6, 46–56. [Google Scholar] [CrossRef]
  2. Lamont, R.J.; Koo, H.; Hajishengallis, G. The oral microbiota: Dynamic communities and host interactions. Nat. Rev. Microbiol. 2018, 16, 745–759. [Google Scholar] [CrossRef] [PubMed]
  3. Solbiati, J.; Frias-Lopez, J. Metatranscriptome of the oral microbiome in health and Disease. J. Dent. Res. 2018, 97, 492–500. [Google Scholar] [CrossRef] [PubMed]
  4. Liu, Y.; Ren, Z.; Hwang, G.; Koo, H. Therapeutic strategies targeting cariogenic biofilm microenvironment. Adv. Dent. Res. 2018, 29, 86–92. [Google Scholar] [CrossRef]
  5. Food and Agricultural Organization of the United Nations; World Health Organization. Joint FAO/WHO Working Group Report on Drafting Guidelines for the Evaluation of Probiotics in Food; Food and Agricultural Organization of the United Nations: Rome, Italy, 2002. [Google Scholar]
  6. 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. [Google Scholar] [CrossRef] [PubMed]
  7. Kreth, J.; Zhang, Y.; Herzberg, M.C. Streptococcal antagonism in oral biofilms: Streptococcus sanguinis and Streptococcus gordonii interference with Streptococcus mutans. J. Bacteriol. 2008, 190, 4632–4640. [Google Scholar] [CrossRef] [PubMed]
  8. Kolenbrander, P.E.; Palmer, R.J., Jr.; Rickard, A.H.; Jakubovics, N.S.; Chalmers, N.I.; Diaz, P.I. Bacterial interactions and successions during plaque development. Periodontology 2000 2006, 42, 47–79. [Google Scholar] [CrossRef]
  9. Myneni, S.R.; Brocavich, K.H.; Wang, H. Biological strategies for the prevention of periodontal disease: Probiotics and vaccines. Periodontology 2000 2020, 84, 161–175. [Google Scholar] [CrossRef]
  10. Burton, J.P.; Chilcott, C.N.; Moore, C.J.; Speiser, G.; Tagg, J.R. A preliminary study of the effect of probiotic Streptococcus salivarius K12 on oral malodour parameters. J. Appl. Microbiol. 2006, 100, 754–764. [Google Scholar] [CrossRef]
  11. Seminario-Amez, M.; López-López, J.; Estrugo-Devesa, A.; Ayuso-Montero, R.; Jané-Salas, E. Probiotics and oral health: A systematic review. Med. Oral Patol. Oral Cir. Bucal. 2017, 22, e282–e288. [Google Scholar] [CrossRef]
  12. Lodi, C.S.; Oliveira, L.V.; Brighenti, F.L.; Delbem, A.C.B.; Martinhon, C.C.R. Effects of probiotic fermented milk on biofilms, oral microbiota, and enamel. Braz. Oral Res. 2015, 29, S1806–S83242015000100229. [Google Scholar] [CrossRef] [PubMed]
  13. Logares, R.; Haverkamp, T.H.; Kumar, S.; Lanzén, A.; Nederbragt, A.J.; Quince, C.; Kauserud, H. Environmental microbiology through the lens of high-throughput DNA sequencing: Synopsis of current platforms and bioinformatics approaches. J. Microbiol. Methods 2012, 91, 106–113. [Google Scholar] [CrossRef] [PubMed]
  14. Martínez-Lamas, L.; Limeres-Posse, J.; Diz-Dios, P.; Álvarez-Fernández, M. Streptococcus downii sp. nov., isolated from the oral cavity of a teenager with Down syndrome. Int. J. Syst. Evol. Microbiol. 2020, 70, 4098–4104. [Google Scholar] [CrossRef] [PubMed]
  15. Cuenca, M.; Sánchez, M.C.; Diz, P.; Martínez-Lamas, L.; Álvarez, M.; Limeres, J.; Sanz, M.; Herrera, D. In vitro anti-biofilm and antibacterial properties of Streptococcus downii sp. nov. Microorganisms 2021, 9, 450. [Google Scholar] [CrossRef]
  16. Bhaumik, D.; Manikandan, D.; Foxman, B. Cariogenic and oral health taxa in the oral cavity among children and adults: A scoping review. Arch. Oral Biol. 2021, 129, 105204. [Google Scholar] [CrossRef]
  17. Alok, A.; Singh, I.D.; Singh, S.; Kishore, M.; Jha, P.C.; Iqubal, M.A. Probiotics: A new era of biotherapy. Adv. Biomed. Res. 2017, 6, 31. [Google Scholar] [CrossRef]
  18. Saha, S.; Tomaro-Duchesneau, C.; Rodes, L.; Malhotra, M.; Tabrizian, M.; Prakash, S. Investigation of probiotic bacteria as dental caries and periodontal disease biotherapeutics. Benef. Microbes 2014, 5, 447–460. [Google Scholar] [CrossRef]
  19. Teughels, W.; Kinder Haake, S.; Sliepen, I.; Pauwels, M.; van Eldere, J.; Cassiman, J.J.; Quirynen, M. Bacteria interfere with A. actinomycetemcomitans colonization. J. Dent. Res. 2007, 86, 611–617. [Google Scholar] [CrossRef]
  20. Van Hoogmoed, C.G.; Geertsema-Doornbusch, G.I.; Teughels, W.; Quirynen, M.; Busscher, H.J.; van der Mei, H.C. Reduction of periodontal pathogens adhesion by antagonistic strains. Oral Microbiol. Immunol. 2008, 23, 43–48. [Google Scholar] [CrossRef]
  21. Ferrer, M.D.; López-López, A.; Nicolescu, T.; Perez-Vilaplana, S.; Boix-Amorós, A.; Dzidic, M.; Garcia, S.; Artacho, A.; Llena, C.; Mira, A. Topic application of the probiotic Streptococcus dentisani improves clinical and microbiological parameters associated with oral health. Front. Cell. Infect. Microbiol. 2020, 10, 465. [Google Scholar] [CrossRef]
  22. Chen, L.J.; Tsai, H.T.; Chen, W.J.; Hsieh, C.Y.; Wang, P.C.; Chen, C.S.; Wang, L.; Yang, C.C. In vitro antagonistic growth effects of Lactobacillus fermentum and Lactobacillus salivarius and their fermentative broth on periodontal pathogens. Braz. J. Microbiol. 2012, 43, 1376–1384. [Google Scholar] [CrossRef] [PubMed]
  23. Poorni, S.; Srinivasan, M.R.; Nivedhitha, M.S. Probiotic Streptococcus strains in caries prevention: A systematic review. J. Conserv. Dent. 2019, 22, 123–128. [Google Scholar] [CrossRef]
  24. Huang, X.; Browngardt, C.M.; Jiang, M.; Ahn, S.J.; Burne, R.A.; Nascimento, M.M. Diversity in antagonistic interactions between commensaloral Streptococci and Streptococcus mutans. Caries Res. 2018, 52, 88–101. [Google Scholar] [CrossRef] [PubMed]
  25. Lee, K.; Walker, A.R.; Chakraborty, B.; Kaspar, J.R.; Nascimento, M.M.; Burne, R.A. Exploring novel probiotic mechanisms of Streptococcus A12 with functional genomics. bioRxiv 2019. [Google Scholar] [CrossRef]
  26. Allaker, R.P.; Ian Douglas, C. Non-conventional therapeutics for oral infections. Virulence 2015, 6, 196–207. [Google Scholar] [CrossRef] [PubMed]
  27. Polonskaia, M.S. Antibiotic substances in acidophil bacteria. Mikrobiologiia 1952, 21, 303–310. [Google Scholar]
  28. Silva, M.; Jacobus, N.V.; Deneke, C.; Gorbach, S.L. Antimicrobial substance from a human Lactobacillus strain. Antimicrob. Agents Chemother. 1987, 31, 1231–1233. [Google Scholar] [CrossRef]
  29. Hillman, J.D.; Shivers, M. Interaction between wild-type, mutant and revertant forms of the bacterium Streptococcus sanguis and the bacterium Actinobacillus actinomycetemcomitans in vitro and in the gnotobiotic rat. Arch. Oral Biol. 1988, 33, 395–401. [Google Scholar] [CrossRef]
  30. Tong, H.; Dong, Y.; Wang, X.; Hu, Q.; Yang, F.; Yi, M.; Deng, H.; Dong, X. Redox-regulated adaptation of Streptococcus oligofermentans to hydrogen peroxide stress. mSystems 2020, 5, e00006-20. [Google Scholar] [CrossRef]
  31. Bao, X.; de Soet, J.J.; Tong, H.; Gao, X.; He, L.; van Loveren, C.; Deng, D.M. Streptococcus oligofermentans inhibits Streptococcus mutans in biofilms at both neutral pH and cariogenic conditions. PLoS ONE 2015, 10, e0130962. [Google Scholar] [CrossRef]
  32. Huang, X.; Palmer, S.R.; Ahn, S.J.; Richards, V.P.; Williams, M.L.; Nascimento, M.M.; Burne, R.A. A highly arginolytic Streptococcus species that potently antagonizes Streptococcus mutans. Appl. Environ. Microbiol. 2016, 82, 2187–2201. [Google Scholar] [CrossRef] [PubMed]
  33. Olivares, M.; Díaz-Ropero, M.P.; Martín, R.; Rodríguez, J.M.; Xaus, J. Antimicrobial potential of four Lactobacillus strains isolated from breast milk. J. Appl. Microbiol. 2006, 101, 72–79. [Google Scholar] [CrossRef] [PubMed]
  34. Terai, T.; Okumura, T.; Imai, S.; Nakao, M.; Yamaji, K.; Ito, M.; Nagata, T.; Kaneko, K.; Miyazaki, K.; Okada, A.; et al. Screening of probiotic candidates in human oral bacteria for the prevention of dental disease. PLoS ONE 2015, 10, e0128657. [Google Scholar] [CrossRef] [PubMed]
  35. Arihara, K.; Ogihara, S.; Mukai, T.; Itoh, M.; Kondo, Y. Salivacin 140, a novel bacteriocin from Lactobacillus salivarius subsp. salicinius T140 active against pathogenic bacteria. Lett. Appl. Microbiol. 1996, 22, 420–424. [Google Scholar] [CrossRef] [PubMed]
  36. Ganzle, M.G.; Höltzel, A.; Walter, J.; Jung, G.; Hammes, W.P. Characterization of reutericyclin produced by Lactobacillus reuteri LTH2584. Appl. Environ. Microbiol. 2000, 66, 4325–4333. [Google Scholar] [CrossRef]
  37. Van Reenen, C.A.; Dicks, L.M.; Chikindas, M.L. Isolation, purification and partial characterization of plantaricin 423, a bacteriocin produced by Lactobacillus plantarum. J. Appl. Microbiol. 1998, 84, 1131–1137. [Google Scholar] [CrossRef]
  38. Baca-Castanón, M.L.; De la Garza-Ramos, M.A.; Alcázar-Pizana, A.G.; Grondin, Y.; Coronado-Mendoza, A.; Sánchez-Najera, R.I.; Cárdenas-Estrada, E.; Medina-De la Garza, C.E.; Escamilla-García, E. Antimicrobial effect of Lactobacillus reuteri on cariogenic bacteria Streptococcus gordonii, Streptococcus mutans, and periodontal diseases Actinomyces naeslundii and Tannerella forsythia. Probiotics Antimicrob. Proteins 2015, 7, 1–8. [Google Scholar] [CrossRef] [PubMed]
  39. Hillman, J.D.; McDonell, E.; Cramm, T.; Hillman, C.H.; Zahradnik, R.T. A spontaneous lactate dehydrogenase deficient mutant of Streptococcus rattus for use as a probiotic in the prevention of dental caries. J. Appl. Microbiol. 2009, 107, 1551–1558. [Google Scholar] [CrossRef] [PubMed]
  40. Hoare, A.; Marsh, P.D.; Diaz, P.I. Ecological therapeutic opportunities for oral diseases. Microbiol. Spectr. 2017, 5. [Google Scholar] [CrossRef]
  41. Hillman, J.D.; Johnson, K.P.; Yaphe, B.I. Isolation of a Streptococcus mutans strain producing a novel bacteriocin. Infect. Immun. 1984, 44, 141–144. [Google Scholar] [CrossRef]
  42. Walker, G.V.; Heng, N.C.; Carne, A.; Tagg, J.R.; Wescombe, P.A. Salivaricin E and abundant dextranase activity may contribute to the anti-cariogenic potential of the probiotic candidate Streptococcus salivarius JH. Microbiology 2016, 162, 476–486. [Google Scholar] [CrossRef] [PubMed]
  43. Masdea, L.; Kulik, E.M.; Hauser-Gerspach, I.; Ramseier, A.M.; Filippi, A.; Waltimo, T. Antimicrobial activity of Streptococcus salivarius K12 on bacteria involved in oral malodour. Arch. Oral Biol. 2012, 57, 1041–1047. [Google Scholar] [CrossRef] [PubMed]
  44. Di Pierro, F.; Zanvit, A.; Nobili, P.; Risso, P.; Fornaini, C. Cariogram outcome after 90 days of oral treatment with Streptococcus salivarius M18 in children at high risk for dental caries: Results of a randomized, controlled study. Clin. Cosmet. Investig. Dent. 2015, 7, 107–113. [Google Scholar] [CrossRef] [PubMed]
  45. Camelo-Castillo, A.; Benítez-Páez, A.; Belda-Ferre, P.; Cabrera-Rubio, R.; Mira, A. Streptococcus dentisani sp. nov., a novel member of the mitis group. Int. J. Syst. Evol. Microbiol. 2014, 64, 60–65. [Google Scholar] [CrossRef] [PubMed]
  46. López-López, A.; Camelo-Castillo, A.; Ferrer, M.D.; Simon-Soro, Á.; Mira, A. Health-Associated niche inhabitants as oral probiotics: The case of Streptococcus dentisani. Front. Microbiol. 2017, 8, 379. [Google Scholar] [CrossRef]
  47. Gönczi, N.N.; Strang, O.; Bagi, Z.; Rákhely, G.; Kovács, K.L. Interactions between probiotic and oral pathogenic strains. Biol. Futur. 2021, 72, 461–471. [Google Scholar] [CrossRef]
  48. Nes, I.F.; Diep, D.B.; Holo, H. Bacteriocin diversity in Streptococcus and Enterococcus. J. Bacteriol. 2007, 189, 1189–1198. [Google Scholar] [CrossRef]
  49. Armstrong, B.D.; Herfst, C.A.; Tonial, N.C.; Wakabayashi, A.T.; Zeppa, J.J.; McCormick, J.K. Identification of a two-component Class IIb bacteriocin in Streptococcus pyogenes by recombinase-based in vivo expression technology. Sci. Rep. 2016, 6, 36233. [Google Scholar] [CrossRef]
  50. Heng, N.C.; Haji-Ishak, N.S.; Kalyan, A.; Wong, A.Y.; Lovrić, M.; Bridson, J.M.; Artamonova, J.; Stanton, J.A.L.; Wescombe, P.A.; Burton, J.P.; et al. Genome sequence of the bacteriocin-producing oral probiotic Streptococcus salivarius strain M18. J. Bacteriol. 2011, 193, 6402–6403. [Google Scholar] [CrossRef]
  51. Conrads, G.; Westenberger, J.; Lürkens, M.; Abdelbary, M.M. Isolation and Bacteriocin-Related Typing of Streptococcus dentisani. Front. Cell. Infect. Microbiol. 2019, 9, 110. [Google Scholar] [CrossRef]
  52. Martinez Lamas, L. Identification of Streptococcus downii sp. nov., a New Bacterial Species with Probiotic Potential. Doctoral Thesis, University of Vigo, Vigo, Spain, 2022. [Google Scholar]
  53. Robson, G.D.; Bell, S.D.; Kuhn, P.J.; Trinci, A.P. Glucose and penicillin concentrations in agar medium below fungal colonies. J. Gen. Microbiol. 1987, 133, 361–367. [Google Scholar] [CrossRef] [PubMed]
  54. Silva, Á.; Gonzalez, N.; Terrén, A.; García, A.; Martinez-Blanch, J.F.; Illescas, V.; Morales, J.; Maroto, M.; Genovés, S.; Ramón, D.; et al. An infant milk formula supplemented with heat-treated probiotic Bifidobacterium animalis subsp. lactis CECT 8145, reduces fat deposition in C. elegans and augments acetate and lactate in a fermented infant slurry. Foods 2020, 9, E652. [Google Scholar]
  55. Zhu, L.; Kreth, J. The role of hydrogen peroxide in environmental adaptation of oral microbial communities. Oxidative Med. Cell. Longev. 2012, 2012, e717843. [Google Scholar] [CrossRef] [PubMed]
  56. Holmberg, K.; Hallander, H.O. Production of bactericidal concentrations of hydrogen peroxide by Streptococcus sanguis. Arch. Oral Biol. 1973, 18, 423–434. [Google Scholar] [CrossRef] [PubMed]
Antibiotics 12 01472 g001
Figure 1. Inhibition test for S. downii versus S. mutans in the presence of peroxidase (A) and proteinase K (B). Hydrogen peroxide production is not responsible for the inhibition, given that after adding peroxidase, the inhibitory capacity of S. downii versus S. mutans is maintained (A); however, the presence of proteinase K eliminates the inhibitory effect, which confirms the molecule’s protein nature with inhibitory capacity produced by S. downii (B).
Figure 1. Inhibition test for S. downii versus S. mutans in the presence of peroxidase (A) and proteinase K (B). Hydrogen peroxide production is not responsible for the inhibition, given that after adding peroxidase, the inhibitory capacity of S. downii versus S. mutans is maintained (A); however, the presence of proteinase K eliminates the inhibitory effect, which confirms the molecule’s protein nature with inhibitory capacity produced by S. downii (B).
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Figure 2. Growth curves of S. mutans in the presence of concentrated S. downii supernatant (SP S. downii) and concentrated BHI medium (BHI × 10). The addition of the concentrated S. downii supernatant inhibits the growth of S. mutans (blue line), while S. mutans preserves its growth capacity after the addition of the concentrated BHI medium (red line). Mean and standard deviation of three replicates.
Figure 2. Growth curves of S. mutans in the presence of concentrated S. downii supernatant (SP S. downii) and concentrated BHI medium (BHI × 10). The addition of the concentrated S. downii supernatant inhibits the growth of S. mutans (blue line), while S. mutans preserves its growth capacity after the addition of the concentrated BHI medium (red line). Mean and standard deviation of three replicates.
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Antibiotics 12 01472 g003
Figure 3. Summary of the experiments performed to study the mechanism of S. downii inhibition of S. mutans.
Figure 3. Summary of the experiments performed to study the mechanism of S. downii inhibition of S. mutans.
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Table 1. Mean and standard deviation concentration of three replicates of organic acids present in solubilized agar samples obtained from the S. mutans ATCC 25175T plate before culture with S. downii (S. mutans) and those obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T.
Table 1. Mean and standard deviation concentration of three replicates of organic acids present in solubilized agar samples obtained from the S. mutans ATCC 25175T plate before culture with S. downii (S. mutans) and those obtained from the inhibition halo generated by S. downii after culture with S. mutans ATCC 25175T.
Organic Acids (mg/mL)
S. mutansS. mutans + S. downiip-Value
Succinic0.051 ± 0.0040.010 ± 0.0010.1
Lactic0.055 ± 0.0071.616 ± 0.0570.1
Formic0.018 ± 0.0020.182 ± 0.0030.1
Acetic0.183 ± 0.0080.273 ± 0.0250.1
Propionic0.095 ± 0.0070.064 ± 0.0060.1
Isobutyric---
Butyric0.0140.004-
Isovaleric---
Valeric-0.041 ± 0.004-
Caproic0.073 ± 0.0040.043 ± 0.0040.1
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Martínez-Lamas, L.; García-Mato, E.; Rincón-Quintero, A.; Rivas-Mundiña, B.; Diz-Dios, P.; Álvarez-Fernández, M. Mechanism of Action of Streptococcus downii, a New Bacterial Species with Probiotic Potential. Antibiotics 2023, 12, 1472. https://doi.org/10.3390/antibiotics12091472

AMA Style

Martínez-Lamas L, García-Mato E, Rincón-Quintero A, Rivas-Mundiña B, Diz-Dios P, Álvarez-Fernández M. Mechanism of Action of Streptococcus downii, a New Bacterial Species with Probiotic Potential. Antibiotics. 2023; 12(9):1472. https://doi.org/10.3390/antibiotics12091472

Chicago/Turabian Style

Martínez-Lamas, Lucía, Eliane García-Mato, Anniris Rincón-Quintero, Berta Rivas-Mundiña, Pedro Diz-Dios, and Maximiliano Álvarez-Fernández. 2023. "Mechanism of Action of Streptococcus downii, a New Bacterial Species with Probiotic Potential" Antibiotics 12, no. 9: 1472. https://doi.org/10.3390/antibiotics12091472

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