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Jorge Jesús Veloz, Marysol Alvear, Luis A. Salazar, "Evaluation of Alternative Methods to Assess the Biological Properties of Propolis on Metabolic Activity and Biofilm Formation in Streptococcus mutans", Evidence-Based Complementary and Alternative Medicine, vol. 2019, Article ID 1524195, 8 pages, 2019. https://doi.org/10.1155/2019/1524195
Evaluation of Alternative Methods to Assess the Biological Properties of Propolis on Metabolic Activity and Biofilm Formation in Streptococcus mutans
Several biological activities have been reported for the Chilean propolis, among their antimicrobial and antibiofilm properties, due to its high polyphenol content. In this study, we evaluate alternative methods to assess the effect of Chilean propolis on biofilm formation and metabolic activity of Streptococcus mutans (S. mutans), a major cariogenic agent in oral cavity. Biofilm formation was studied by using crystal violet and by confocal microscopy. The metabolic activity of biofilm was evaluated by MTT and by flow cytometry analysis. The results show that propolis reduces biofilm formation and biofilm metabolic activity in S. mutans. When the variability of the methods to measure biofilm formation was compared, the coefficient of variation (CV) fluctuated between 12.8 and 23.1% when using crystal violet methodology. On the other hand, the CV ranged between 2.2 and 3.3% with confocal microscopy analysis. The CV for biofilm’s metabolic activity measured by MTT methodology ranged between 5.0 and 11.6%, in comparison with 1.9 to 3.2% when flow cytometry analysis was used. Besides, it is possible to conclude that the methods based on colored compounds presented lower precision to study the effect of propolis on biofilm properties. Therefore, we recommend the use of flow cytometry and confocal microscopy in S. mutans biofilm analysis.
Propolis is a product collected by honeybees (Apis mellifera) and formed by the resinous excretions of buds and bark of trees and shrubs . Propolis is widely used for its medicinal properties. Several biological activities have been reported for propolis including anti-inflammatory, antibacterial, antifungal and/or antiviral, immunomodulatory properties, suppression of HIV-1 replication and immunoregulatory effect, cytotoxicity, hepatoprotection, and free-radical scavenging activity [2–5].
Similarly, the Chilean propolis has showed different biological properties, including antiangiogenic [6–8], antiatherosclerotic [7, 9], antifungal , antidiabetic , antimicrobial [12–16], hepatoprotective , antiproliferative , and antioxidant  activities, due to its high content of polyphenols, mainly pinocembrin .
In relation to antimicrobial activity, our group has demonstrated specifically the antibiofilm properties of the Chilean propolis against Streptococcus mutans (S. mutans) [14–16], a major cariogenic agent in oral cavity. Biofilms are clusters of single or multiple species of bacteria encased in a matrix composed of polysaccharides, proteins, and DNA that protect the bacteria from environmental pressures. There are many protocols that have been proposed to analyze relative biofilm formation . However, some assays cannot usually distinguish between planktonic killing by the antibiotic and specific antibiofilm effects since bacteria are exposed to the compound of interest before they have a chance to adhere . Similarly, assaying residual bound bacteria using crystal violet, the most widely used method to evaluate biofilm activity, has issues since crystal violet stains biomass rather than living bacteria, and thus, dead bound bacteria will still be stained [19, 20]. Thus, it is important to assess the best method to monitor and to analyze biofilm growth in the presence of antibiofilm/antimicrobial agents. Here, we compared various methods for quantifying the antibiofilm activity of Chilean propolis on S. mutans, including crystal violet staining, metabolic dyes, flow cytometry, and confocal microscopy.
2. Materials and Methods
2.1. Preparation of Polyphenol-Rich Extract of Propolis (EP)
To evaluate the effect of polyphenols from EP in antimicrobial activity and biofilm formation of S. mutans, propolis was collected during the Spring of 2008 from the La Araucanía region (Chile). A crude propolis sample was kept frozen (−20°C) and later crushed in cold, and 30 grams was dissolved in 100 mL of ethanol (70%) and macerated for 7 days at room temperature. The ethanolic extract of propolis (EEP) was filtered with a Whatman 2.0 paper and centrifuged at 327 g, during 20 minutes at 5°C. Finally, the solvent was evaporated at a temperature of 40°C, for 2 hours in a rotavaporator (Buchi, R-210, Germany) and dissolved for 24 h with sterile DMSO (0.01%) to obtain polyphenol-rich extract of propolis (EP).
2.2. Determination of Total Phenolic Content in EP
The content of total polyphenols in EP was quantified by Folin–Ciocalteu reaction by a modification of Popova and collaborator’s methodology . For this assay, 100 μL of EP was mixed with 100 μL of distilled water and 2 mL of Folin–Ciocalteu reagent (Merck, Germany). The resulting solution was incubated for 8 minutes, and finally, 3 mL of sodium carbonate (20%) (w/v) was added. The absorbance of this solution was measured at 760 nm after 2 hours of incubation at room temperature. The concentration of polyphenols was calculated from a calibration curve and was expressed in mg·mL−1 equivalent to the pinocembrin-galangin standard mixture (1 : 1).
2.3. Bacteria Culture Conditions and Inoculum
Bacteria were obtained from clinical isolates from children with tooth decay. S. mutans was identified using the methodology proposed by Salazar et al. . The cultures were made in Petri plates with Columbia agar (Becton Dickinson and Co., NY, and USA) supplied with sucrose (1%) in an anaerobic container (GasPak EZ. Becton Dickinson and Co., NY, USA) and it was incubated at 37°C and 5% of CO2, for 24 hours. The inoculum was adjusted using optical density comparison from 1.0 to 550 nm which corresponds to 2 × 108 CFU·mL−1 (stock suspension).
2.4. Determination of Antibacterial Activity
Minimum inhibitory concentration (MIC) was determined by the serial dilution method following the NCCLS guidelines . The suspension of 5 × 105 CFU·mL−1 was inoculated in 96-well microplates, containing 100 μL of sterile trypticase soy broth (Becton Dickinson and Co., NY, USA) with sucrose 1% and with different concentrations of polyphenol-rich extract of propolis (EP) (from 0.1 to 1.96 μg·mL−1). Chlorhexidine digluconate (0.2%) was used as positive control, and cultures in DMSO (0.01%) without propolis were used as a negative control. The assay was performed in triplicate and incubated for 48 hours.
2.5. Biofilm Formation and S. mutans Adherence
Biofilm growth was quantified and indirectly assessed by crystal violet staining assay. The S. mutans attachment cells were grown in microplates with sterile trypticase soy broth (TSB) and sucrose (1%). S. mutans cultures were supplied with concentrations of EP, between 0.1 and 1.96 μg·mL−1, under anaerobic conditions 37°C and 5% of CO2, for 48 hours. First, the broth was removed, the plates were washed three times to eliminate nonadherent bacteria with PBS, and the plates were dried at 60°C for 45 minutes. After that, each well was stained with 100 μL of crystal violet 1% (w/v) solution, incubated for 15 minutes, and washed again with sterile PBS. Biofilm formation was determined by adding 125 μL of ethanol 95% per well and then transferred to a new plate to measure the optical density (OD) at 590 nm in a microplate reader in comparison with the control biofilm (without EP) .
2.6. Biofilm Growth for Morphology Analysis
For biofilm generation, samples were prepared in FluoroDish plates (World Precision Instrument Inc., China) that contained 3 mL of sterile tripticase soy broth supplied with sucrose, 1%. The plates were prepared with 10 μL of bacterial inoculum (5 × 105 UFC·mL−1) for incubation at 5% of atmosphere CO2, at 37°C for 48 hours. Biofilm was generated in a liquid medium, and different concentrations of EP were added (0.1 to 1.96 μg·mL−1).
2.7. Fluorescent Labeling
Biofilms were stained with calcein Biofilm Tracer™ (Invitrogen, the USA). First, the plates were incubated with 50 μL of calcein probe and were incubated for 1 hour. After incubation, a medium was removed and, then, the plates were washed three times using PBS to eliminate unabsorbed tracer .
2.8. Microscopic Analysis of Biofilm Thickness
A 60 × 0.21 NA objective lens was used to visualize bacterial plaque by means of the confocal scanning laser microscope Olympus Fluoview 100. For imaging antimicrobial effect, the 480 nm laser was used for excitation and the ﬂuorescent signal was detected in a green channel. All images were captured by directed acquisition by Z-step, ranging to take a series of time-lapse image scans (512 × 512 pixels) at intervals of 15 seconds and 0.5 μm for each confocal plane. Data were analyzed by ImageJ Mac Biophotonic software.
2.9. Analyses of Biofilm Metabolic Activity in 96-Well Microplates
EP cytotoxicity was performed by the modified reduction assay of 3-[4,5-dimethylthiazol-2yl]-2,5-diphenyltetrazolium (MTT) bromide (Sigma-Aldrich, France). Because of this, the reagent was dissolved in PBS, taking it to a concentration of 5 mg·mL−1, and added in microplate wells containing 90 μL of trypticase soy broth, plus sucrose (1%). Besides, 10 μL of a bacterial suspension equivalent to 5 × 104 CFU·mL−1 was added and supplied with concentrations of EP (0.1 to 1.6 μg·mL−1) and 200 μL of MTT to obtain formazan. The plates were incubated at 37°C and 5% CO2 for 48 hours. The absorbance of obtained solutions was quantified at 490 nm. Cytotoxicity was expressed in percentages of inhibition in the cellular viability in cultures with less than 50% growth (IC50%) and compared to the color developed by untreated cells. The controls included DMSO at 0.01% as vehicle control, and untreated cells (negative control) and chlorhexidine digluconate at 0.2% as positive control. All the tests were carried out in triplicate.
The inhibition percentage of biofilm viability was calculated using the following formula:
2.10. Biofilm Viability by Flow Cytometry
A biofilm was formed in glass tubes at anaerobial conditions at 37°C and for 48 hours using sterile trypticase soy broth (TSB), sucrose (1%), and EP (0.1 to 1.96 μg·mL−1) to a final volume of 10.000 μL. After incubation, an aliquot of 100 μL of biofilm suspension was transferred to an eppendorf and was stained with Live/Dead® BacLight Bacterial Viability Kit. First, 10 μL of Syto9 (20 μM) was added for 15 minutes, and later, 10 μL of PI (800 μM) was added for 5 minutes; the tubes were washed twice with sterile PBS and centrifuged for 1 minute at . Finally, cells were resuspended in sterile PBS, and they were analyzed by flow cytometry (FACS CantoII™, BD Biosytem). The sample with two stain components was excited at 488 nm, and the emission was registered using the FITC channel for Syto 9 (530/30) and PerCP channel (670/LP) for propidium iodide. Suspension containing 5 × 106 cell·mL−1 were aspirated with a flow rate 12 μL·min−1. The results of biofilm cell viability were expressed in percentage in relation with untreated control cells .
2.11. Statistical Analysis
Statistical analyses were performed using the computational Statistical Program R, version 3.5.1. The D’Shapiro–Wilson test was applied to determine the results’ normal distribution. Afterwards, the values were analyzed using the nonparametric Wilcoxon test for related samples. The values are expressed as median ± SD. The variability of the evaluated methods was determined by calculating the coefficient of variation (CV). Significant differences were considered at .
3.1. Total Polyphenol Content in Chilean Propolis
The content of polyphenols in EP in equivalence of the pinocembrin-galangin mixture was quantified by Folin–Ciocalteu reaction, and it was 137.7 ± 0.7 mg·g−1. Previous studies of our group described the chemical composition of the EP. The main flavonoids identified in the Chilean propolis by means of the HPLC-DAD as quercetin, apigenin, pinocembrin, and caffeic acid phenethyl ester (CAPE) [13, 16].
3.2. Biofilm Inhibition Assessed by Crystal Violet Staining
The percentage of biofilm inhibition in cultures was calculated considering untreated cells as 100% of biofilm growth (control). When EP was added at 1.96 μg·mL−1 and 0.8 μg·mL−1, the values of biofilm reduction were 53.4 ± 2.0% and 47.7 ± 2.0%, respectively (). Similarly, when we used EP at a concentration of 0.4 μg·mL−1, the bacterial pellicle decreased in 43.5 ± 3.3% (). Also, when we used EP at 0.2 and 0.1 μg·mL−1, these concentrations prevented the biofilm growth in 24.9 ± 4.0% and 19.2 ± 3.3%, respectively (). Finally, chlorhexidine and DMSO reduced the biofilm formation in 18.8 ± 2.9% and 8.8 ± 2.1%, respectively (Figure 1).
3.3. Biofilm Formation Analysis by Confocal Microscopy
The extracellular matrix (biofilm) obtained from S. mutans cultures treated with EP at a concentration of 0.8 μg·mL−1 shows a size of 7.3 ± 0.2 μm in comparison to the control biofilm (20.8 ± 0.3 μm); when 0.4 μg·mL−1 of polyphenols was applied, the obtained biofilm was 9.3 ± 0.2 μm; other concentrations such as 0.2 μg·mL−1 and 0.1 μg·mL−1 generated greater biofilms, with 10.7 ± 0.2 μm and 15.0 ± 0.2 μm. Although the effect of chlorhexidine was higher than these low concentrations, the synthetic compound allowed sizes of 13.9 ± 0.6 μm. This may probably be because excipients contained in their formulation may be affecting this result. Figure 2 shows the effect of different polyphenol concentrations in biofilm thickness.
3.4. Analyses of Biofilm’s Metabolic Activity by MTT
The MTT method showed significant reduction values in a percentage of cellular viability for concentrations lower than MIC. For the EP concentration at 0.8 μg·mL−1, the reduction was 58.2 ± 3.5%; for EP at 0.4 μg·mL−1 was 69.2 ± 8.6%; for EP at 0.2 μg·mL−1 was 82.1 ± 8.8%, and for EP at 0.1 μg·mL−1 was 85.0 ± 7.2%. The reduction for chlorhexidine was 83.0 ± 7.0%, with significant statistical differences. Cellular viability at different EP concentrations is shown in Figure 3.
3.5. Biofilm Metabolic Activity of S. mutans by Flow Cytometry
Figure 4 shows individual dot plots of the S. mutans biofilm analyzed by flow cytometry; the assays to measure metabolic activity in the S. mutans biofilm generated for 48 hours facilitated the differentiation of live and dead cell populations performed with excitation/emission fluorescence Syto 9 and propidium iodide stains. Some EP concentrations such as 0.8 μg·mL−1 (0.04 ± 0.005% of live cells) and 0.4 μg·mL−1 (0.08 ± 0.004% of live cells) had a higher effect than chlorexidine in the reduction of live cells detected; the value for chlorexidine was 0.95 ± 0.003%. For the EP at 0.2 μg·mL−1 and EP at 0.1 μg·mL−1, a low number of detected viable cells but less than chlorhexidine was observed (1.41 ± 0.004 and 4.1 ± 0.008 of live cells; Figure 5). We found higher statistical differences in comparison with untreated cells in all treatments ().
The antimicrobial agents in propolis produce changes in biofilm structure and in cellular aggregation due to fluctuations in the levels of protein and enzymatic expression . In this study, we evaluated several methods to assess the antibiofilm activity of the Chilean propolis. When we compared the variability of the methods to measure biofilm formation, the coefficient of variation (CV) fluctuated between 12.8 and 23.1% after using crystal violet methodology. However, the CV ranged between 2.2 and 3.3% when we used confocal microscopy. The high degree of dispersion for crystal violet staining is probably due to the interference by color development. The other factor that explained the differences is that the crystal violet stains biomass rather than living bacteria, and thus, dead bound bacteria will still be stained. In spite of its popularity, crystal violet has certain weaknesses, including nonspecific binding to anionic proteins and other negatively charged molecules, like capsules, lipopolysaccharides, and DNA/nucleic acids, leading to an inability to distinguish between live and dead bacterial populations [19, 20]. These problems contribute to a large variability among samples that may complicate the interpretation of biofilm screening results.
Colorimetric methods such as MTT have been used to quantify metabolic activity in cultures. The basic principle is the conversion by cellular metabolic activity of the substrate into a colored formazan from tetrazolium, later measurable with a spectrophotometer. Our results show that the CV for biofilm’s metabolic activity measured by MTT ranged between 5.0 and 11.6%, in comparison with 1.9 to 3.2% when using flow cytometry analysis. The differences between these methodologies can be explained considering that the flow cytometry used propidium iodide costained with Syto9 (LIVE/DEAD staining) as an indicator for cellular membrane integrity. This combination on stable biofilm with calcein probe alone improves the discrimination between live and dead cells . These results confirm that the techniques involving probes or excitation by laser allowed acquire more accurate information.
Nevertheless, it is necessary to establish a gold standard method to validate the accuracy of the evaluated methods. In addition, it is necessary to eliminate interferences that could appear on having used these methodologies, implementing some validation, for example, using culture-based methods as a reference, to assess metabolic activity (MTT methodology) in parallel to DNA staining or minimizing extracellular matrix coharvesting, if harvested cell viability is to be assessed by staining .
These results suggest that the staining methods presented a large variability to evaluate the effect of propolis on biofilm formation and metabolic activity. Flow cytometry and confocal microscopy allowed more accurate results when compared with traditional methodologies. Thus, we recommend the use of flow cytometry and confocal microscopy to evaluate the antimicrobial properties of propolis in Streptococcus mutans.
The data used to support the findings of this study are available from the corresponding author upon request.
Conflicts of Interest
The authors declare that there are no conflicts of interest regarding the publication of this paper.
All authors have read the manuscript and agreed with the content. JJV and LAS conceived and designed the study. JJV performed the experiments. JJV, MA, and LAS analyzed the data. MA and LAS contributed reagents/materials and analysis tools. JJV wrote the paper. LAS reviewed and edited the manuscript.
The authors would like to express their gratitude to CONICYT Scholarship and the financial support of DIUFRO Project (#DI10-0031).
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