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Determination of optimum incubation time for formation of Pseudomonas aeruginosa and Streptococcus pyogenes biofilms in microtiter plate
Bulletin of the National Research Centre volume 43, Article number: 100 (2019)
Pseudomonas aeruginosa and Streptococcus pyogenes are the most common pathogens to humans and are able to form a biofilm following ineffective precautionary approach. Biofilm is defined as a surface-attached community of bacterium embedded in an extracellular matrix which leads to tremendous problems in the environment, among humans and animals. This study aims to investigate the ability of P. aeruginosa and S. pyogenes to form biofilms in 96-well plate before further study in antibiofilm will be done. Initially, the 96-well plate was added with 100 μl of overnight P. aeruginosa culture with optical density (OD) 0.1 and S. pyogenes culture with OD 0.05. The cultures were incubated for 7 days at 37 °C to justify the formation of biofilm. Subsequently, stained blue biofilm was detached from the plate by using 95% ethanol. Biofilms were finally measured using a micro plate reader at 570 nm and were classified based on the adherence strength formula. P. aeruginosa and S. pyogenes biofilms strongly adhered to the plates on days three, four, five and six. Interestingly on day three, biofilms showed the highest formation. However, moderate biofilm formation onto the plates by both P. aeruginosa and S. pyogenes were observed on day two, but non-adherence was observed on days one and seven. Day three is the optimum cultivation period for P. aeruginosa and S. pyogenes to switch into a strong biofilm in microtiter plate and could be beneficial for antibiofilm experiments.
A biofilm is an intricate accumulation of microbial colonies. It leads to form a matrix which consists of a highly structured protective layer of polysaccharides (Ford 2014; López et al. 2010). The adherent cell in biofilm is embedded within a slimy extracellular matrix that contained of extracellular polymeric substances (EPS). Microbial cells are the primary components of biofilms that produce EPS which then contributes 50 to 90% of the total organic carbon in biofilms (Zhao et al. 2014; Flemming et al. 2000). EPS is actually composed of polysaccharide and varies in physical and chemical properties, and is neutral or polyanionic in Gram-positive or Gram-negative bacteria. Its size is between 0.2 to 1.0 nm (Kokare et al. 2009; Nyenje et al. 2012, 2013), and its thickness ranges between 10 and 30 nm (Khan et al. 2017). Microbial cells in biofilm are immobilized by EPS (Flemming et al. 2016; Koo and Yamada 2016) which then retains the cells closely and leads the forming of synergistic micro consortia (Flemming and Wingender 2010). The formation and maintenance of structured multi-cellular microbial communities in biofilm crucially depends on the quantity of EPS (Janissen et al. 2015). Usually, a biofilm matrix is composed of carbohydrate, protein, pili, flagella, adhesion fibres and cellulose (Kostakioti et al. 2013; Xiao and Zheng 2016). All these components with the addition of hydrophobic interaction, and action and entanglement of the biopolymers in the culture plate provide sufficient mechanical stability to maintain spatial arrangement of the biofilm (Mazza 2016; O’Loughlin et al. 2013). Therefore, our study aims to determine the optimum incubation time for P. aeruginosa and S. pyogenes to form biofilms in the microtiter plate.
Materials and methods
A Gram-positive of S. pyogenes (ATCC 19615) and a Gram-negative of P. aeruginosa (ATCC 10145) were used for biofilm formation. P. aeruginosa and S. pyogenes inoculums prepared by picking up two to three morphologically identical colonies from stock culture which were then suspended in 10 mL of sterile Mueller Hinton broth in sterilized universal bottles. The inoculums were incubated at 37 °C for 24 h (Shehu et al. 2016).
Initially, 2 ml of inoculums was removed aseptically from the universal bottle and poured into a micro cuvette (Eppendorf, Germany). The optical density (OD) 0.1 for P. aeruginosa and OD 0.05 for S. pyogenes were adjusted by using sterile Mueller Hinton broth (MHB) at 600 nm with a spectrophotometer (Genesys 20, Thermo Scientific). Subsequently, P. aeruginosa and S. pyogenes biofilms were prepared by transferring 100 μl of adjusted inoculums into sterile 96-well plates (Fisher Scientific, UK). As a negative control, broth without bacteria was prepared. The incubation was done at 37 °C for 7 days. The media were then removed by slightly tapping the plate. The plate was washed three times with sterile distilled water to remove free-floating planktonic bacteria and was then drained off by inverting to allow it to air dry. The biofilms were stained with 100 μl 0.1% (w/v) crystal violet for 10 min. To remove the crystal violet, the plate was washed three times with phosphate-buffered saline. To detach the biofilms, 100 μl of 95% ethanol was added into each well. The solubilized biofilm formations were finally measured by the micro plate reader (Tecan Infinite 200 PRO, Austria Gmbh) at the wavelength of 570 nm (Jaffar et al. 2016). The experiments were performed in triplicate. The following formulas were used to classify the biofilm formation. Non-adherent [NA = OD ≤ ODC)], weak adherent [WA = ODC < OD ≤ (2 × ODC)], moderate adherent [MA = (2 × ODC) < OD ≤ (4 × ODC)] and strong adherent [SA = (4 × ODC) < OD)] (Nyenje et al. 2013).
Quantitative analysis of biofilm formation was statistically tested by using SPSS (version 20.0: IBM). Mean difference was determined by using an independent t test. Statistical significance was set at p < 0.05. Data are represented as mean values ± standard deviation.
Results and discussion
The qualitative assay showed the formation of P. aeruginosa and S. pyogenes biofilms in the microtiter plate (Fig. 1). Biofilm was stained blue in colour.
After 7 days of incubation in MHB OD 0.1 and MHB OD 0.05, a variety of biofilm phenotypes were demonstrated. Figure 2 shows biofilm formation by P. aeruginosa. Strong biofilm formation were determined on days three, four, five and six, (1.0 ± 0.10), (0.78 ± 0.04), (0.64 ± 0.02) and (0.37 ± 0.03), respectively. Biofilm moderately adhered on day two (0.12 ± 0.01). However, on days one and seven the biofilms were non-adherent, (0.06 ± 0.00) and (0.09 ± 0.01), respectively.
The biofilm formation by S. pyogenes has shown similar characteristics with P. aeruginosa biofilm (Fig. 3). The strongest adherent S. pyogenes biofilms were on days three, four, five and six, (0.96 ± 0.05), (0.70 ± 0.02), (0.58 ± 0.02) and (0.33 ± 0.01), respectively. Biofilm moderately adhered on day two (0.13 ± 0.01). Meanwhile, on days one and seven, the biofilms were non-adherent, (0.05 ± 0.00) and (0.08 ± 0.01), respectively.
P. aeruginosa biofilms on day three were significantly higher compared to days four, five and six, p < 0.014, p < 0.016 and p < 0.017, respectively. Similarly S. pyogenes biofilms on day three were significantly higher compared to days four, five and six, p < 0.018, p < 0.014 and p < 0.017, respectively. Thus, we suggest on day three, a large number of bacteria in the plate were switched to biofilm. An optimum number of bacteria adherence occurred in microtiter plate resulting strong biofilm formation on that day (Jama et al. 2017; Rossi et al. 2016). In addition to day three, we observed that the biofilm formation by P. aeruginosa and S. pyogenes were strong on days four, five and six. P. aeruginosa and S. pyogenes were not able to produce biofilm on days two and seven. Many factors such as integration of diverse signals from the environment might play a role in biofilm formation, concurrent with other events such as phenotypic and genetic switching during biofilm production and also EPS production (Ismael 2013; Bakar et al. 2018). Commonly, biofilm formation is enhanced by cell motility particularly when it is mediated by flagella. Under certain environmental conditions, flagella is necessary for biofilm formation by P. aeruginosa and S. pyogenes (Priya and Brundha 2013). However, the rapid decrease of biofilm-forming capacity that we observed on day seven could be attributed to the loss of exopolymers from the biofilm and in particular of exopolysaccharides, which may suggest that an active process of detachment was occurring, probably mediated by enzymatic degradation (Allison et al. 1998). Previous studies showed that P. aeruginosa produced a great biofilm on day three, while Escherichia coli was produced biofilm on day six (Culotti and Packman 2014). Another study found that day three was the preferable day in producing strong biofilm by Proteus mirabilis (Emineke et al. 2017). A study in 2001 showed that an ideal cultivation period for producing biofilms by Candida albicans was at 72 h and Saccharomyces cerevisiae was at 60 h (Chandra et al. 2001). The current study shows that many types of pathogenic Leptospira biofilms were classified either as non-adherent or weak adherent after the first and second days of incubation and the strongest biofilm production was found from the third to seventh days (Pui et al. 2017). Another study showed that day five was the optimum day for Leptospires to produce greater biofilm formation (Apun et al. 2018). Previous studies also reported that Listeria monocyte and Listeria sp. produced strong biofilms by which they gradually increased after 2 to 7 days of incubation (Adetunji and Isola 2011; Mueller et al. 2007). A study by Jaffar et al. (2016) demonstrated that Actinomycetemcomitans and Porphyromonas gingivalis produced biofilm from days two to seven, with differing attachment ability. The present study demonstrates that strong biofilms formed on day three. The ability to adhere to a solid surface and the consecutive formation of an organized bacterial biofilm community are crucial for the formation of P. aeruginosa and S. pyogenes biofilms. This is because the formation of biofilm depends on the ability of bacteria to attach on the surface for 96-well plates (Merritt et al. 2006). It is well known that the switching from a planktonic to a biofilm mode of growth is an intricate process, which occurs in response to environmental changes. As the first step of biofilm formation is bacterial adhesion to surface, we can hypothesise that the strains showed a high ability to create hydrophobic interactions with the microtiter plate surface (Woo et al. 2012). Moreover, physical and chemical plate properties are the main factors that regulate the initial adhesion process (Lemos et al. 2014).
This study demonstrated that P. aeruginosa and S. pyogenes successfully formed biofilms on the 96-well plate by using MHB after 3 days of cultivation. The cultivation period had significantly affected biofilm formation for both bacteria. Importantly, the study has proven that a duration less than 3 days or more than 3 days was not the optimum condition to form biofilm for both P. aeruginosa and S. pyogenes in microtiter plate.
American type culture collection
Extracellular polymeric substances
International Business Machines Corporation
Mueller Hinton broth
- p :
Statistical package for the social sciences
- w/v :
Weight per volume
Adetunji VO, Isola TO (2011) Crystal violet binding assay for assessment of biofilm formation by Listeria monocytogenes and Listeria spp on wood, steel and glass surfaces. Glob Vet 6(1):6–10
Allison DG, Ruiz B, SanJose C, Jaspe A, Gilbert P (1998) Extracellular products as mediators of the formation and detachment of Pseudomonas fluorescens biofilms. FEMS Microbiol Lett 167(2):179–184
Apun K, Jalan J, Pui CF, Bilung LM, Hashim HF, Aina A (2018) Biofilm forming ability of intermediate and saprophytic Leptospira on abiotic and biotic surfaces. Malays J Microbiol 14(4):313–319
Bakar MA, McKimm J, Haque SZ, Majumder MA, Haque M (2018) Chronic tonsillitis and biofilms: a brief overview of treatment modalities. J Inflamm Res 11:329
Chandra J, Kuhn DM, Mukherjee PK, Hoyer LL, McCormick T, Ghannoum MA (2001) Biofilm formation by the fungal pathogen Candida albicans: development, architecture, and drug resistance. J Bacteriol 183(18):5385–5394
Culotti A, Packman AI (2014) Pseudomonas aeruginosa promotes Escherichia coli biofilm formation in nutrient-limited medium. PLoS One 9(9):e107186
Emineke S, Cooper AJ, Fouch S, Birch BR, Lwaleed BA (2017) Diluted honey inhibits biofilm formation: potential application in urinary catheter management. J Clin Pathol 70(2):140–144
Flemming HC, Wingender J (2010) The biofilm matrix. Nat Rev Microbiol 8(9):623
Flemming HC, Wingender J, Griebe T, Mayer C (2000) Physico-chemical properties of biofilms. Biofilms: recent advances in their study and control, pp 19–34
Flemming HC, Wingender J, Szewzyk U, Steinberg P, Rice SA, Kjelleberg S (2016) Biofilms: an emergent form of bacterial life. Nat Rev Microbiol 14(9):563
Ford M (ed) (2014) Medical microbiology. fundamental biomedical science. Oxford University Press (1):2–17
Ismael NF (2013 Sep) (Vinegar) as anti-bacterial biofilm formed by Streptococcus pyogenes isolated from recurrent tonsillitis patients, in vitro. Jordan J Biol Sci 147(898):1–7
Jaffar N, Miyazaki T, Maeda T (2016 Nov) Biofilm formation of periodontal pathogens on hydroxyapatite surfaces: implications for periodontium damage. J Biomed Mater Res A 104(11):2873–2880
Jama C, Abdallah M, Boukherroub R, Faille C, Chihib NE (2017) Effect of incubation duration, growth temperature, and abiotic surface type on cell surface properties, adhesion and pathogenicity of biofilm-detached Staphylococcus aureus cells. AMB Express 7(1):191
Janissen R, Murillo DM, Niza B, Sahoo PK, Nobrega MM, Cesar CL, Temperini ML, Carvalho HF, De Souza AA, Cotta MA (2015) Spatiotemporal distribution of different extracellular polymeric substances and filamentation mediate Xylella fastidiosa adhesion and biofilm formation. Sci Rep 5:9856
Khan MS, Altaf MM, Ahmad I (2017) Chemical nature of biofilm matrix and its significance. biofilms in plant and soil health, p 151
Kokare CR, Chakraborty S, Khopade AN, Mahadik KR (2009) Biofilm: importance and applications. Indian J Biotechnol 8:159–168
Koo H, Yamada KM (2016) Dynamic cell–matrix interactions modulate microbial biofilm and tissue 3D microenvironments. Curr Opin Cell Biol 42:102–112
Kostakioti M, Hadjifrangiskou M, Hultgren SJ (2013) Bacterial biofilms: development, dispersal, and therapeutic strategies in the dawn of the postantibiotic era. Cold Spring Harb Perspect Med 3(4):a010306
Lemos M, Borges A, Teodósio J, Araújo P, Mergulhão F, Melo L, Simões M (2014) The effects of ferulic and salicylic acids on Bacillus cereus and Pseudomonas fluorescens single-and dual-species biofilms. Int Biodeterior Biodegradation 86:42–51
López D, Vlamakis H, Kolter R (2010) Biofilms. Cold Spring Harb Perspect Biol 2(7):a000398
Mazza MG (2016 Apr 18) The physics of biofilms—an introduction. J Phys D Appl Phys 49(20):203001
Merritt JH, Kadouri DE, O'Toole GA (2006) Growing and analyzing static biofilms. Curr Protoc Microbiol 1: Unit–1B (1):1–29.
Mueller RS, McDougald D, Cusumano D, Sodhi N, Kjelleberg S, Azam F, Bartlett DH (2007) Vibrio cholerae strains possess multiple strategies for abiotic and biotic surface colonization. J Bacteriol 189(14):5348–5360
Nyenje M, Green E, Ndip R (2013) Evaluation of the effect of different growth media and temperature on the suitability of biofilm formation by Enterobacter cloacae strains isolated from food samples in South Africa. Molecules 18(8):9582–9593
Nyenje ME, Green E, Ndip RN (2012) Biofilm formation and adherence characteristics of Listeria ivanovii strains isolated from ready-to-eat foods in Alice, South Africa. Sci World J V 2012:7.
O’Loughlin CT, Miller LC, Siryaporn A, Drescher K, Semmelhack MF, Bassler BL (2013) A quorum-sensing inhibitor blocks Pseudomonas aeruginosa virulence and biofilm formation. Proc Natl Acad Sci 110(44):17981–17986
Priya S, Brundha S (2013) Biofilm formation by Streptococcus serotypes on dental plaques. Int J Adv Med 1(1):7–10 Article ID Med-54
Pui CF, Apun K, Jalan J, Bilung LM, Su’ut L, Fatma HH (2017) Microtitre plate assay for the quantification of biofilm formation by pathogenic Leptospira. Res J Microbiol 12(2):146–153
Rossi C, Chaves-López C, Serio A, Goffredo E, Goga BT, Paparella A (2016) Influence of incubation conditions on biofilm formation by Pseudomonas fluorescens isolated from dairy products and dairy manufacturing plants. Italian J Food Saf 5:3
Shehu A, Ismail S, Rohin MA, Harun A, Aziz AA, Haque M (2016) Antifungal properties of Malaysian Tualang honey and stingless bee propolis against Candida albicans and Cryptococcus neoformans. J Appl Pharm Sci 6(2):044–050
Woo JH, Kim ST, Kang IG, Lee JH, Cha HE, Kim DY (2012) Comparison of tonsillar biofilms between patients with recurrent tonsillitis and a control group. Acta Otolaryngol 132(10):1115–1120
Xiao R, Zheng Y (2016) Overview of microalgal extracellular polymeric substances (EPS) and their applications. Biotechnol Adv 34(7):1225–1244
Zhao C, Xing M, Yang J, Lu Y, Lv B (2014) Microbial community structure and metabolic property of biofilms in vermifiltration for liquid-state sludge stabilization using PLFA profiles. Bioresour Technol 151:340–346
This work was supported by grants UniSZA/2017/DPU/37 R0018-R341 and UniSZA /2018/DPU/13. We thank the Microbiological Laboratory Members of the Faculty of Health Science and the Medical Faculty, Universiti Sultan Zainal Abidin for their assistance.
Financial support for this whole project obtained from Dana Penyelidikan Universiti Sultan Zainal Abidin.
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Al-kafaween, M.A., Mohd Hilmi, A.B., Jaffar, N. et al. Determination of optimum incubation time for formation of Pseudomonas aeruginosa and Streptococcus pyogenes biofilms in microtiter plate. Bull Natl Res Cent 43, 100 (2019). https://doi.org/10.1186/s42269-019-0131-9
- Pseudomonas aeruginosa
- Streptococcus pyogenes