Characterization of biofilm matrix, degradation by DNase treatment and evidence of capsule downregulation in Streptococcus pneumoniae clinical isolates
© Hall-Stoodley et al; licensee BioMed Central Ltd. 2008
Received: 24 April 2008
Accepted: 08 October 2008
Published: 08 October 2008
Streptococcus pneumoniae is a common respiratory pathogen and a major causative agent of respiratory infections, including otitis media (OM). Pneumococcal biofilms have been demonstrated on biopsies of the middle ear mucosa in children receiving tympanostomy tubes, supporting the hypothesis that chronic OM may involve biofilm development by pathogenic bacteria as part of the infectious process. To better understand pneumococcal biofilm formation six low-passage encapsulated nasopharyngeal isolates of S. pneumoniae were assessed over a six-eight day period in vitro.
Multiparametric analysis divided the strains into two groups. Those with a high biofilm forming index (BFI) were structurally complex, exhibited greater lectin colocalization and were more resistant to azithromycin. Those with a low BFI developed less extensive biofilms and were more susceptible to azithromycin. dsDNA was present in the S. pneumoniae biofilm matrix in all strains and treatment with DNase I significantly reduced biofilm biomass. Since capsule expression has been hypothesized to be associated with decreased biofilm development, we also examined expression of cpsA, the first gene in the pneumococcal capsule operon. Interestingly, cpsA was downregulated in biofilms in both high and low BFI strains.
All pneumococcal strains developed biofilms that exhibited extracellular dsDNA in the biofilm matrix, however strains with a high BFI correlated with greater carbohydrate-associated structural complexity and antibiotic resistance. Furthermore, all strains of S. pneumoniae showed downregulation of the cpsA gene during biofilm growth compared to planktonic culture, regardless of BFI ranking, suggesting downregulation of capsule expression occurs generally during adherent growth.
Streptococcus pneumoniae is an important bacterial pathogen worldwide that causes localized disease including pneumonia and otitis media (OM), as well as invasive infections such as septicemia and meningitis. The ability of this organism to persist in the respiratory tract and transition between asymptomatic carriage and infection stimulates intense research interest in S. pneumoniae. Pneumococcus is a leading bacterial cause of acute OM in children where it is estimated that by age five, over 80% of children have had at least one OM episode . S. pneumoniae is also frequently detected in chronic otitis media with effusion (OME) , the most common cause of acquired conductive hearing loss in children. While, invasive disease has decreased with the introduction of the pneumococcal heptavalent conjugate vaccine (PCV7), localized infection in the middle ear has not been reduced as dramatically and new serotypes, some resistant to multiple antibiotics, have emerged [3, 4].
The detection of pneumococcal-specific DNA and RNA in culture-negative effusions in multiple studies suggests that active bacterial infections are present more frequently than culture results indicate [2, 5–7], and both the persistence of bacteria and recalcitrance to antibiotic treatment in OME suggest that chronic OM may be associated with bacterial biofilm development on the mucosal surface of the middle ear [7, 8]. This hypothesis was recently supported by evidence of adherent S. pneumoniae, Haemophilus influenzae and Moraxella catarrhalis directly on the middle-ear mucosal epithelium (MEM) in children receiving tympanostomy tube (TT) placement for chronic otitis media . In this study, clusters of adherent pneumococcus were observed on the MEM using 16S rRNA fluorescent in situ hybridization (FISH) and anti-pneumococcal immunostaining. Pathogenic biofilm bacteria were absent on MEM biopsies from patients undergoing surgery for cochlear implantation, suggesting that adherent bacteria are not typically present on MEM.
Biofilm development is initiated when bacterial cells attach to a surface, proliferate and extrude a complex extracellular matrix that binds cells together and to a surface. Several chronic infections, such as cystic fibrosis pneumonia, and chronic tonsillitis and sinusitis, exhibit biofilm development in the respiratory tract of the human host [10–14]. Bacteria within biofilms exhibit two fundamental characteristics: production of an extracellular polymeric substance (EPS) matrix and increased resistance to antimicrobial treatment [11, 12]. Depending on the type of bacteria in the biofilm, the EPS can be made up of polysaccharides, proteins and DNA . Following attachment and biofilm development, bacteria may undergo significant phenotypic shifts including induction of different metabolic pathways, reduced cell division, and development of resistance to antibiotic concentrations capable of killing planktonic bacteria [16–19]. Biofilm formation is important in understanding the extent of bacterial phenotypic plasticity in response to varying environmental conditions and several papers have reported pneumococcal biofilm formation in vitro under various growth conditions [16, 20–26].
The pneumococcal capsule is considered a major virulence factor. Capsule expression is thought to interfere with biofilm formation [20, 23, 24, 26] and biofilm development may select for unencapsulated phenotypic variants [20, 23, 26]. However, S. pneumoniae is also known to phenotypically vary capsule production upon adherence to epithelial cells . The polysaccharide capsule-specific regions of S. pneumoniae are encoded by a cluster of genes located between dexB upstream and aliA downstream  and the capsule is predicted to be transcribed as a single operon, initiating upstream of the most conserved gene in the operon, cpsA .
We chose a static culture system to examine biofilm formation under conditions that simulate those in the middle ear during OME. Biofilm development in six encapsulated clinical strains of S. pneumoniae representing six different serotypes was assessed by three independent techniques and statistically analyzed to formulate a parametric index of biofilm development that resulted in ranking the strains into two groups. The index was then used to test hypotheses concerning pneumococcal biofilms such as the composition of the extracellular matrix, susceptibility of pneumococcal biofilms to antimicrobial treatment and capsule expression using cpsA.
S. pneumoniaeclinical strains vary in initial attachment, kinetics of biofilm formation and biofilm structural complexity and the Biofilm Forming Index (BFI)
All 6 clinical isolates also attached over a 24 hour period (Fig. 2B) demonstrated by crystal violet staining. However, strains BS69, BS72 and BS75 produced nearly twice as much biofilm as strains BS68, BS71 and BS73. BS71 formed significantly less biomass than all of the other isolates in this assay (P values < 0.05). There was no significant difference between BS72, BS69 and BS75.
Strain differences were also quantified using COMSTAT (Fig. 2C). Biofilm biovolume (biomass) and maximum thickness were lower for the clinical strains BS68, BS71 and BS73. Consistent with the experimental results of the CFU/cm2 and CV assays, BS69 and BS72 exhibited the greatest extent of total biomass and maximum thickness (> 20 μm). Surface roughness, a measure of biofilm heterogeneity, was low for these isolates, with greater heterogeneity correlating with microcolonies separated by large voids (data not shown). ANOVA analysis of COMSTAT data demonstrated significant differences among the strains with respect to biofilm formation. Comparison of averages from grouped COMSTAT data (multiple plates, multiple experiments) demonstrated that BS69 and BS72 exhibited significantly more biomass than the other strains in this biofilm assay.
When data were combined from all 3 biofilm assays using the combined biofilm forming index (BFI) metric, the strains divided into two groups (Fig 2D). Strains BS69, BS72 and BS75 demonstrated far greater biofilm development (in order of ranking), while strains BS68, BS71 and BS73 demonstrated less biofilm development.
Scanning electron microscopy (SEM) comparison of two S. pneumoniaeisolates
S. pneumoniaebiofilms demonstrate a carbohydrate matrix
The multilayered S. pneumoniae biofilm towers of BS69, BS72 and BS75 observed with CLSM and SEM suggested that biofilm towers were held together by an extracellular matrix. Since fixation for SEM dehydrates the biofilm and collapses the matrix, we further tested pneumococcal biofilms for extracellular carbohydrate using a cocktail of 5 fluorescently-conjugated lectins and the nucleic acid probe, Syto59 under hydrated conditions. Figure 3B shows biofilms of each pneumococcal isolate grown for 8 days. High ranked BFI isolates (BS69, BS72 and BS75) exhibited a much greater degree of lectin binding, whereas low ranked BFI isolates BS71 and BS73 exhibited less lectin binding. BS68 showed more biofilm ultrastructure using the combination of lectins and Syto 59 than the other low ranked BFI strains, exhibiting some clusters stained with nucleic acid stain with large discrete patches bound with lectin, however the clusters were uniformly smaller than those of high ranked BFI strains (Fig. 3B). Biofilms of the unencapsulated strain, R6, also bound lectin. Colocalization of lectin and nucleic acid binding differed between strains when biofilms were evaluated with Imaris Colocalization software, using regression analysis (r2 values). Averages of Pearson's coefficient showed greater colocalization of nucleic acid and carbohydrate specific probes with biofilms of BS69, BS72 and BS75 (Rr > 0.75) than BS68, BS71 and BS73 (Rr < 0.70), consistent with lectin binding correlating with higher order biofilm ultrastructure. High ranked BFI strains significantly differed from low ranked strains (P < 0.05).
S. pneumoniaebiofilms exhibit increased resistance to antibiotic treatment
Concentration of antibiotic producing no turbidity after azithromycin treatment for S. pneumoniae clinical isolates grown in planktonic culture and as biofilms treated with a twofold serial dilution of azithromycin from 2 mg ml-1 to 2 μg ml-1 for 24 hours.
Planktonic IC* (μg ml-1)
Biofilm IC† (μg ml-1)
Fold Increase (-)
S. pneumoniaeclinical isolates have extracellular DNA in the matrix which is degraded with DNAse treatment
Degradation of S. pneumoniae Biofilms with DNase treatment.
0 (μg ml-1)
1 (μg ml-1)
100 (μg ml-1)
1000 (μg ml-1)
Biomass (μm 3 /μm 2 )
0.18 (0.020) **
Average thickness (μm)
BS 69 (14)
Maximum thickness (μm)
BS 69 (14)
CpsAexpression is downregulated in pneumococcal biofilms
The ability of upper respiratory pathogens including S. pneumoniae to persist in the nasopharynx and cause chronic disease upon the appropriate conditions may be associated with the ability to form biofilms on mucosal epithelium [7–9]. The presence of structurally complex bacterial biofilms is important because biofilms have been shown to exhibit increased resistance to host immune effectors and increased tolerance to antibiotic treatment [11, 12, 15], and therefore suggest that biofilms may contribute to the persistence of pathogens.
Previous reports have shown that S. pneumoniae can form biofilms in vitro using several different models of biofilm culture [16, 20–26] including a study where CSLM data suggested that some of the strains used in the present study differed according to structural complexity . Moreover in a pair of companion studies we have demonstrated that these strains have vastly different genomic complements  and produce significantly different disease phenotypes in an animal model of infection . We therefore wished to further characterize biofilm formation of 6 of these pneumococcal strains by investigating the kinetics of biofilm formation, biofilm matrix composition, antibiotic resistance and capsule expression.
All clinical isolates developed biofilms containing viable, adherent cells over time under static conditions in vitro. However, biofilm development was highly variable among the different isolates. A multiparameter ranking, formulated to compare biofilm formation among the clinical strains using 3 standard assays commonly used to measure biofilm formation, identified two groups: those with a high biofilm forming index (BFI); BS69, BS72 and BS75, which attached quickly and produced more biofilm than the other strains, and those with a low BFI; BS68, BS71 and BS73 which produced biofilms consisting of adherent cells in small cell clusters with few towers. Our study suggests that a multi-assay approach for the quantification of biofilm formation better addresses strain to strain variation in the context of overall biofilm heterogeneity. Bacteria are frequently categorized as being positive or negative for biofilm formation typically using only a single assay such as crystal violet staining. However, our study suggests that such a binary distinction may lead to an oversimplified conclusion. Clearly, each of the six strains formed biofilms, but to different degrees. In the absence of clinical data correlating the degree of in vitro biofilm formation with infection severity and history, a biofilm etiology, even for a poor in vitro biofilm forming strain, should not necessarily be discounted. Not only was the BFI a useful construct to provide a clearer picture of the relative biofilm forming capacity of each strain, but it was also useful in testing putative biofilm characteristics, since a higher BFI correlated with greater binding with carbohydrate-specific lectins and antibiotic resistance in vitro.
Since SEM suggested that BFI was associated with biofilm structural complexity, biofilms from each pneumococcal strain were assessed for the presence of carbohydrate in the EPS matrix using lectin binding. High BFI strains (BS69, BS72 and BS75) exhibited the most lectin co-localization with the EPS matrix, while strains with a low BFI (BS71 and BS73) demonstrated reduced lectin co-localization, suggesting that polysaccharide is associated with larger multilayered aggregates of attached cells. BS68 exhibited some biofilm towers associated with nucleic acid and larger discrete patches of lectin binding (suggesting carbohydrate) than other low BFI strains. Lectin binding did not necessarily correlate with the pneumococcal capsule, since an unencapsulated strain (R6) which formed good biofilms, also bound lectin, suggesting that carbohydrate is associated with noncapsular EPS.
We further assessed another hallmark of biofilm development; antibiotic resistance. Six day pneumococcal biofilms with a low BFI exhibited a 2-fold increase in resistance to azithromycin compared to planktonic growth. However, strains with a high BFI required significantly higher concentrations to inhibit outgrowth from biofilms. In situ examination of 6 day biofilms treated with 20 μg ml-1 of azithromycin (a concentration that was bactericidal for S. pneumoniae in epithelial cell culture)  showed large clusters of viable bacteria in high ranked BFI strains. Few viable attached cells were observed after azithromycin treatment in low ranked isolates. Although our study did not reflect a standardized minimum inhibitory concentration on biofilm bacteria due to the difficulty of assessing cell density within biofilms, these results support the hypothesis that biofilm-forming pneumococcal strains can persist in spite of antibiotic treatment and may contribute to chronic infection.
The presence of extracellular DNA (eDNA) in biofilms is now well documented in several types of bacterial biofilms including non-typeable H. influenzae, another major pathogen associated with chronic OM [33–36]. We therefore investigated if eDNA was present in the pneumococcal biofilm matrix. All strains showed evidence of eDNA shown by in situ staining of the matrix with the dsDNA stain, PicoGreen, and by a dose-dependent reduction of the pneumococcal biofilm biomass by recombinant human DNase I treatment using Pulmozyme® (dornase alfa), used clinically to treat cystic fibrosis pneumonia. DNase-treated biofilms were significantly reduced in all pneumococcal strains when treated with the clinical dose of Pulmozyme® (1 mg ml-1), exceeding 90% reduction in all but one strain. These results agree with those of Moscoso et al. who showed that DNase treatment reduced biofilms of the unencapsulated S. pneumoniae strain R6, and are consistent with the ability of S. pneumoniae to autolyse and release DNA [24, 35].
Other in vitro studies with pneumococci have shown that capsule expression was associated with decreased biofilm formation [20, 23, 24, 26] and some have reported that biofilm development may select for unencapsulated phenotypic variants [20, 24, 26]. However, S. pneumoniae is also known to phenotypically vary capsule production upon adherence to epithelial cells . Therefore we hypothesized that the capsule operon might be downregulated in pneumococcal biofilms. Real time-qPCR results indicate that cpsA is downregulated in the biofilm up to 10-fold depending on the strain, compared to planktonic cultures regardless of the strain's BFI, suggesting that capsule production is variably modulated during sessile growth. In situ immunofluorescence staining with anti-capsule type-specific antibody further demonstrated that S. pneumoniae growing in biofilms was encapsulated and capsule immunostaining was brightest in biofilm towers compared to adherent cells. These results support the role of cpsA in capsule production [37, 38]. Numerous reports demonstrate capsule phenotypic variation and show that variants with greater amounts of capsule colonize epithelial cells less efficiently [39–44]. Phenotypic variation of the capsule has been demonstrated microscopically during the initial stages of infection where adherent or invasive S. pneumoniae exhibited reduced amounts of capsule compared to cells not associated with epithelial cells . Our results showing downregulation of cpsA in pneumococcal biofilms are consistent with observations that S. pneumoniae modulates capsule production upon adherence.
Biofilm growth differed among six clinical isolates of S. pneumoniae. A multi-parametric assessment grouped isolates into two categories: those with a high biofilm forming index, which exhibited complex ultrastructure consisting of large multilayered biofilm towers; and those with a low BFI, which exhibited small compact microcolonies. BFI correlated with increased lectin binding and resistance to azithromycin. BFI did not correlate with the presence of DNA in biofilm EPS or modulation of capsule expression. DNase treatment resulted in a significant reduction of pneumococcal biofilms in all strains, however lectin binding to biofilm towers suggests the pneumococcal biofilm matrix is made up of both carbohydrate and DNA. Finally, cpsA was downregulated in all biofilm grown strains suggesting that capsule expression is phenotypically regulated upon biofilm development.
Isolation of strains and growth conditions
Clinical isolates of S. pneumoniae used in this study were obtained from nasal washes from symptomatic pediatric patients participating in a vaccine trial at Children's Hospital of Pittsburgh and isolated, cultured, serotyped and frozen as described previously . All clinical isolates were encapsulated and were cultured identically. The six strains were: BS68 (serotype 9V); BS69 (serotype 14); BS71 (serotype 3); BS72 (serotype 23F); BS73 (serotype 6A); and BS75 (serotype 19F). Frozen stocks of S. pneumoniae were plated and individual colonies were picked and grown in THB to an optical density corresponding to 108 cells ml-1. Growth curves were obtained for each strain and OD and CFUs ml-1 were correlated using regression analysis. Calibration curves for 1 × 108 CFUs ml-1 and OD were used to estimate the inoculated number of S. pneumoniae cells and validated by plating as follows: BS68 (OD600 0.03); BS69 (OD600 0.04); BS71 (OD600 0.07); BS72 (OD600 0.03); BS73 (OD600 0.04) and BS75 (OD600 0.06). All experiments were carried out at 37°C, 5% CO2.
Crystal violet assay for initial biofilm attachment
1 × 107 S. pneumoniae in THB were inoculated into 48-well plates (Corning, Lowell, MA), incubated for 24 hours and rinsed to remove non-adherent cells. One ml of 0.5% crystal violet (CV) solution (Sigma Aldrich) was added  and read at 600 nm using a Beckman DU 650 spectrophotometer (Beckman Coulter Inc., Fullerton, CA.). Background absorbance from medium blanks was subtracted from the values of triplicate samples from 5 independent experiments.
1 × 108 ml-1 S. pneumoniae was inoculated into MatTek culture plates (MatTek Corporation, Ashland, MA) or 6-well tissue culture plates (Falcon) and allowed to adhere overnight. S. pneumoniae biofilms were grown for 1, 3 and 6 days and culture medium was replaced daily with fresh, warm 1/5 strength THB. For colony forming unit (CFU) enumeration, S. pneumoniae biofilms were rinsed thrice with THB and adherent bacteria were detached using a cell scraper (Corning). One plate was harvested per time point and duplicate wells were combined (3 per 6 well plate), vortexed, diluted and plated in 2 independent experiments.
Confocal Laser Scanning Microscopy
Pneumococcal biofilms were also visualized directly using CLSM and the BacLight Bacterial Viability Kit. Biofilms were grown for 1, 3, and 6 days and stained according to the manufacturer's directions, rinsed, immersed in Hank's balanced salt solution (HBSS) with Ca+2 and Mg+2 and immediately examined with a Leica DM RXE microscope attached to a TCS SP2 AOBS confocal system (Leica Microsystems, Exton, PA) using a 63× water immersion lens and the sequential scanning mode. Images were analyzed using the Leica LCS software, COMSTAT  and Imaris Software (Bitplane; St. Paul, MN).
Scanning electron microscopy (SEM)
Biofilms were processed for SEM by dehydration in a graded ethanol series. Samples were sputter coated with 200 angstroms of gold using a Hummer VII Sputtering System (Anatech Ltd., Alexandria, VA), visualized at an accelerator voltage of 5 kV using a Tescan Mira field emission scanning electron microscope (Tescan USA, Cranberry Township, PA) and digitized TIFF images were collected.
EPS Carbohydrate binding with fluorescent lectin probes
To assess the extent and distribution of carbohydrate in the pneumococcal biofilm matrix, cultures were grown for 8 days as above, rinsed and stained with a cocktail of 5 lectins consisting of Alexa 488-conjugated lectins (Invitrogen) at the following concentrations: 50 μg ml-1 of Canavalia ensiformis (Con A) specific for α-mannopyranosyl and α-glucopyranosyl residues, 125 μg ml-1 of (Wheat germ agglutinin) WGA specific for N-acetyl glucosamine and N-acetylneuraminic acid, 100 μg ml-1 of Griffonia simplicifolia (GS II), specific for terminal α- and β- linked N-acetyl-D-glucosaminyl residues; 125 μg ml-1 of (Soybean agglutinin) SBA, specific for terminal β-galactose; and 75 μg ml-1 of (Peanut agglutinin) PNA, specific for terminal α- and β-N-acetyl-galactosamine and galactopyranosyl residues in HBSS. Three μl of Syto 59 nucleic acid stain was added per ml of the cocktail. Cultures were stained for 35 minutes rinsed to remove unbound lectin and nucleic acid probe and sequentially scanned using the 488 and 633 nm laser lines to minimize channel cross-talk for co-localization analysis.
COMSTAT image analysis
Quantitative analyses of the CLSM images by the COMSTAT computer software was performed on day 6 biofilms stained with BacLight , or with PicoGreen, a dsDNA stain  as described. The biofilm parameters, biomass (biovolume), maximum and average thickness, and roughness coefficient (an indicator of biofilm heterogeneity) were assessed using a minimum of 5 different images per plate from 2 independent experiments for each isolate.
Statistical comparisons were made using one-way analysis of variance (ANOVA) (Excel 2000, Microsoft). Differences were reported statistically significant for P < 0.05.
Calculation of a "biofilm forming index" (BFI)
To combine the information from the 3 biofilm assays (crystal violet, 6 day CFU/cm2 count and COMSTAT data) to give an overall assessment of the degree of biofilm formation of each pneumococcal strain, we used a simple normalized ranking system based on a "biofilm forming index" (BFI) for each assay. The Shapiro-Wilk normality test (The R Project for Statistical Computing: R statistical software version 2.6.2 (2008 02 08) freely available at http://www.r-project.org) was used to determine whether the data sets needed to be transformed to achieve a normal distribution (P > 0.05). Of the data sets for the 6 pneumococcal strains, 4 of 6 were normal for the CV assay and viable cell count, and 1 of 6 was normal for COMSTAT. Log10 transformation of the data resulted in all data sets conforming to a normal distribution (P > 0.05). The BFI for each of the individual assays for each of the six strains was determined using:
BFIOD or BFICFU or BFICOMSTAT = (Log(10) Strain value - Log(10) lowest value)/(Log(10) highest value - Log(10) lowest value)
Thus each strain was assigned a value ranging from "I", for the least biofilm, to "1" for the most biofilm.
The data from the 3 assays was combined to find the overall combined (BFI) from:
BFI = (BFIOD + BFICFU + BFICOMSTAT)/3
Antibiotic treatment of S. pneumoniaeplanktonic cells and biofilms
Planktonic cultures were grown to mid-log phase and incubated with twofold dilutions of azithromycin ranging from a concentration of 2 mg ml-1 to 2 μg ml-1 in 1/5 THB for 24 hours in 24-well polystyrene plates (BD, Franklin Lakes, NJ). Biofilms were grown in 24-well plates for 6 days whereby non-adherent cells were removed to a new 24 well plate and incubated with twofold dilutions of azithromycin to test if nonattached cells at this period of culture were resistant to azithromycin. Spectrophotometric readings were taken at 595 nm using a GENios plate reader and also scored visually. The concentration of azithromycin that showed a lack of turbidity corresponding to the spectrophotometric reading of the negative control (THB only) was interpreted as indicating the minimum concentration of antibiotic that inhibited bacterial growth. Biofilms were exposed to identical concentrations of azithromycin and incubated as for planktonic cells; rinsed with THB and incubated for a further 24 hours. Visual and spectrophotometric readings of duplicate wells were taken in 3 different experiments and the lowest concentration that indicated no turbidity (inhibition of planktonic growth from the biofilm or 'showering') was interpreted as the minimum concentration of antibiotic that inhibited bacterial outgrowth from the biofilm. Additionally, S. pneumoniae biofilms were grown in MatTek plates for 6 days, rinsed and treated with 20 μg ml-1 of azithromycin for 24 h , stained with BacLight kit and imaged in situ.
Pulmozyme®(DNase 1) experiments
Six day biofilms for each strain were incubated for 15 minutes at RT in the dark with Pulmozyme® (dornase alfa), a synthetic DNase I (supplied as 1 mg ml-1 solution), (Genentech Inc, San Franscisco, CA) in duplicate at each of three concentrations (1 μg ml-1, 100 μg ml-1 and 1 mg ml-1). Untreated controls were incubated with 200 μl of buffer alone (8.7 mg ml-1 NaCl-0.15 mg ml-1CaCl2). Plates were rinsed and stained for 15 minutes with 100 μl each of PicoGreen (1 μl ml-1) and Syto 59 (3 μl ml-1) (Invitrogen)  in HBSS, rinsed and imaged.
Isolation of RNA
To assess capsular gene expression in clinical isolates, real-time quantitative PCR (RT-qPCR) was used to measure the transcripts of the pneumococcal capsular gene, cpsA . For the isolation of RNA, BS69, BS71, BS72 and BS73 and the unencapsulated strain R6, were grown to late log phase (planktonic) or harvested from 6-well plates after 6 days (biofilm). Total cellular RNA was then isolated as previously described . RNA preparations were tested for contaminating DNA by no-reverse-transcriptase PCR reactions.
Real-time quantitative PCR
Oligonucleotide primers and TaqMan probes used in RT-qPCR analysis of gene expression
Taqman Probe (Fam-Tamra)
In this study
PCR reactions were done in 15 μl reaction volumes containing the reaction mixtures as follows: 1.5 μl cDNA; 7.5 μl universal PCR master mix; 1.2 μl forward primer (800 pM); 1.2 μl reverse primer (800 pM); 1.2 μl Taqman probe (160 pM) and 2.4 μl nuclease-free de-ionized H2O. PCR amplification parameters were as follows: 50°C for 2 minutes, followed by 95°C for 10 minutes, and then 45 cycles of 95°C for 15 s and 60°C for 1 minute. All qPCR reactions were done in triplicate and the mean CT was used for analysis of results. The constitutively expressed gene for DNA gyrase (gyr) was used as an endogenous control as described previously . The ΔCT values were determined by subtracting the gyr CT value from the gene-specific CT values. The ΔΔCT value was calculated by subtracting the ΔCT value obtained with the ΔCT calibrator value. To verify the absence of contaminating DNA, each RT-qPCR experiment included controls that lacked template cDNA or reverse transcriptase. The amount of target gene transcript was expressed as the difference (n-fold) from the amount of the control gene (2-ΔCT), where ΔCT represents the difference in threshold cycle between the target and control genes. Analysis of expression of each gene was done based on at least 2 independent experiments. Twofold or higher changes in gene expression were considered significant.
Planktonic cultures of BS68, BS71, BS72 and BS73 were incubated with capsule-specific antiserum according to supplier instructions (Statens Seruminstitut, Copenhagen, Denmark). For qualitative determination of pneumococcal capsule, biofilms were rinsed, scraped and incubated with type-specific capsule antibodies as for planktonic cells. Additionally, 8 day biofilm cultures were rinsed and examined in situ using CLSM after incubation with polyclonal rabbit anti-capsular antibody and a secondary AffiniPure F(ab)2 fragment Texas Red-conjugated donkey antirabbit IgG (H+L chain) antibody (Jackson ImmunoResearch, West Grove, PA).
This work was supported by Allegheny General Hospital/Allegheny Singer Research Institute and grants from the NIDCD DC05659, DC04173, and DC02148. The authors thank Karen Barbadora and David Greenberg for the clinical pneumococcal strains and Mary O'Toole for administrative assistance.
- Bakaletz LO: From Otitis media. Polymicrobial Diseases. Edited by: Brogden KA, Guthmiller JM. 2002, Washington, D.C.: ASM Press, 259-298.View ArticleGoogle Scholar
- Post JC, Preston RA, Aul JJ, Larkins-Pettigrew M, Rydquist-White J, Anderson KW, Wadowsky RM, Reagan DR, Walker ES, Kingsley LA, Magit AE, Ehrlich GD: Molecular analysis of bacterial pathogens in otitis media with effusion. JAMA. 1995, 273 (3): 1598-1604. 10.1001/jama.273.20.1598.View ArticlePubMedGoogle Scholar
- Pichichero ME, Casey JR: Emergence of a multiresistant serotype 19A pneumococcal strain not included in the 7-valent conjugate vaccine as an otopathogen in children. JAMA. 2007, 298 (15): 1772-1778. 10.1001/jama.298.15.1772.View ArticlePubMedGoogle Scholar
- Whitney CG, Farley MM, Hadler J, Harrison LH, Bennett NM, Lynfield R, Reingold A, Cieslak PR, Pilishvili T, Jackson D, Facklam RR, Jorgensen JH, Schuchat A, Active Bacterial Core Surveillance of the Emerging Infections Program Network: Decline in invasive pneumococcal disease after the introduction of protein-polysaccharide conjugate vaccine. N Engl J Med. 2003, 348 (18): 1737-1746. 10.1056/NEJMoa022823.View ArticlePubMedGoogle Scholar
- Aul JJ, Anderson KW, Wadowsky RM, Doyle WJ, Kingsley LA, Post JC, Ehrlich GD: A comparative evaluation of culture and PCR for the detection and determination of persistence of bacterial strains and DNAs in the Chinchilla laniger model of otitis media. Ann Otol Rhinol Laryngol. 1998, 107 (6): 508-513.View ArticlePubMedGoogle Scholar
- Dingman JR, Rayner MG, Mishra S, Zhang Y, Ehrlich MD, Post JC, Ehrlich GD: Correlation between presence of viable bacteria and presence of endotoxin in middle-ear effusions. J Clin Microbiol. 1998, 36 (11): 3417-3419.PubMed CentralPubMedGoogle Scholar
- Rayner MG, Zhang Y, Gorry MC, Chen Y, Post JC, Ehrlich GD: Evidence of bacterial metabolic activity in culture-negative otitis media with effusion. JAMA. 1998, 79 (4): 296-299. 10.1001/jama.279.4.296.View ArticleGoogle Scholar
- Ehrlich GD, Veeh R, Wang X, Costerton JW, Hayes JD, Hu FZ, Daigle BJ, Ehrlich MD, Post JC: Mucosal biofilm formation in middle-ear mucosa in the chinchilla model of otitis media. JAMA. 2002, 287 (13): 1710-1715. 10.1001/jama.287.13.1710.View ArticlePubMedGoogle Scholar
- Hall-Stoodley L, Hu F, Gieseke A, Nistico L, Nguyen D, Hayes J, Forbes M, Greenberg D, Dice B, Burrows A, Stoodley P, Post JC, Ehrlich GD, Kerschner J: Direct detection of bacterial biofilms on the middle-ear mucosa of children with chronic otitis media. JAMA. 2006, 296 (2): 202-211. 10.1001/jama.296.2.202.PubMed CentralView ArticlePubMedGoogle Scholar
- Chole RA, Faddis BT: Anatomical evidence of microbial biofilms in tonsillar tissues: a possible mechanism to explain chronicity. Arch Otolaryngol Head Neck Surg. 2003, 129 (6): 634-636. 10.1001/archotol.129.6.634.View ArticlePubMedGoogle Scholar
- Costerton JW, Stewart PS, Greenberg EP: Bacterial biofilms: a common cause of persistent infections. Science. 1999, 284 (5418): 1318-1322. 10.1126/science.284.5418.1318.View ArticlePubMedGoogle Scholar
- Donlan RM, Costerton JW: Biofilms: survival mechanisms of clinically relevant microorganisms. Clin Microbiol Rev. 2002, 15 (2): 167-193. 10.1128/CMR.15.2.167-193.2002.PubMed CentralView ArticlePubMedGoogle Scholar
- Ehrlich GD, Hu FZ, Post JC: From Role for biofilms in infectious disease. Microbial Biofilms. Edited by: Ghannoum M, O'Toole GA. 2004, ASM Press, Washington, D.C.:ASM Press, 332-358.View ArticleGoogle Scholar
- Psaltis AJ, Ha KR, Beule AG, Tan LW, Wormald PJ: Confocal scanning laser microscopy evidence of biofilms in patients with chronic rhinosinusitis. Laryngoscope. 2007, 117 (7): 1302-1306. 10.1097/MLG.0b013e31806009b0.View ArticlePubMedGoogle Scholar
- Hall-Stoodley L, Costerton JW, Stoodley P: Bacterial biofilms: from the natural environment to infectious diseases. Nat Rev Microbiol. 2004, 2 (2): 95-108. 10.1038/nrmicro821.View ArticlePubMedGoogle Scholar
- Allegrucci M, Hu FZ, Shen K, Hayes J, Ehrlich GD, Post JC, Sauer K: Phenotypic characterization of Streptococcus pneumoniae biofilm development. J Bacteriol. 2006, 188 (7): 2325-2335. 10.1128/JB.188.7.2325-2335.2006.PubMed CentralView ArticlePubMedGoogle Scholar
- Borriello G, Werner E, Roe F, Kim AM, Ehrlich GH, Stewart PS: Oxygen limitation contributes to antibiotic tolerance of Pseudomonas aeruginosa in biofilms. Antimicrob Agents Chemother. 2004, 48 (7): 2659-2664. 10.1128/AAC.48.7.2659-2664.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Fux CA, Wilson S, Stoodley P: Detachment characteristics and oxacillin resistance of Staphyloccocus aureus biofilm emboli in an in vitro catheter infection model. J Bacteriol. 2004, 186 (14): 4486-4491. 10.1128/JB.186.14.4486-4491.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Sauer K, Camper AK, Ehrlich GD, Costerton JW, Davies DG: Pseudomonas aeruginosa displays multiple phenotypes during development as a biofilm. J Bacteriol. 2002, 184 (4): 1140-1154. 10.1128/jb.184.4.1140-1154.2002.PubMed CentralView ArticlePubMedGoogle Scholar
- Allegrucci M, Sauer K: Characterization of colony morphology variants isolated from Streptococcus pneumoniae biofilms. J Bacteriol. 2007, 189 (5): 2030-2038. 10.1128/JB.01369-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Budhani RK, Struthers JK: The use of Sorbarod biofilms to study the antimicrobial susceptibility of a strain of Streptococcus pneumoniae. J Antimicrob Chemother. 1997, 40 (4): 601-602. 10.1093/jac/40.4.601.View ArticlePubMedGoogle Scholar
- Donlan RM, Piede JA, Heyes CD, Sanii L, Murga R, Edmonds P, El-Sayed I, El-Sayed MA: Model system for growing and quantifying Streptococcus pneumoniae biofilms in situ and in real time. Appl Environ Microbiol. 2004, 70 (8): 4980-4988. 10.1128/AEM.70.8.4980-4988.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- McEllistrem MC, Ransford JV, Khan SA: Characterization of in vitro biofilm-associated pneumococcal phase variants of a clinically relevant serotype 3 clone. J Clin Micro. 2007, 45 (1): 97-101. 10.1128/JCM.01658-06.View ArticleGoogle Scholar
- Moscoso M, Garcia E, Lopez R: Biofilm formation by Streptococcus pneumoniae : role of choline, extracellular DNA, and capsular polysaccharide in microbial accretion. J Bacteriol. 2006, 188 (22): 7785-7795. 10.1128/JB.00673-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Oggioni MR, Trappetti C, Kadioglu A, Cassone M, Iannelli F, Ricci S, Andrew PW, Pozzi G: Switch from planktonic to sessile life: a major event in pneumococcal pathogenesis. Mol Microbiol. 2006, 61 (5): 1196-1210. 10.1111/j.1365-2958.2006.05310.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Waite RD, Struthers JK, Dowson CG: Spontaneous sequence duplication within an open reading frame of the pneumococcal type 3 capsule locus causes high-frequency phase variation. Mol Microbiol. 2001, 42 (5): 1223-1232. 10.1046/j.1365-2958.2001.02674.x.View ArticlePubMedGoogle Scholar
- Hammerschmidt S, Wolff S, Hocke A, Rosseau S, Müller E, Rohde M: Illustration of pneumococcal polysaccharide capsule during adherence and invasion of epithelial cells. Infect Immun. 2005, 73 (8): 4653-4667. 10.1128/IAI.73.8.4653-4667.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Yother J: From Capsule. The Pneumococcus. Edited by: Tuomanen EI. 2004, Washington, DC: ASM Press, 30-48.Google Scholar
- Hathaway LJ, Bättig P, Mühlemann K: In vitro expression of the first capsule gene of Streptococcus pneumoniae, cpsA, is associated with serotype-specific colonization prevalence and invasiveness. Microbiology. 2007, 153 (8): 2465-2471. 10.1099/mic.0.2006/005066-0.View ArticlePubMedGoogle Scholar
- Hiller NL, Janto B, Hogg JS, Boissy R, Yu S, Powell E, Keefe R, Ehrlich NE, Shen K, Hayes J, Barbadora K, Klimke W, Dernovoy D, Tatusova T, Parkhill J, Bentley SD, Post JC, Ehrlich GD, Hu FZ: Comparative genomic analyses of seventeen Streptococcus pneumoniae strains: insights into the pneumococcal supragenome. J Bacteriol. 2007, 189 (22): 8186-8195. 10.1128/JB.00690-07.PubMed CentralView ArticlePubMedGoogle Scholar
- Forbes ML, Horsey E, Hiller NL, Buchinsky FJ, Hayes JD, Compliment JM, Hillman T, Ezzo S, Shen K, Keefe R, Barbadora K, Post JC, Hu FZ, Ehrlich GD: Strain-specific virulence phenotypes of Streptococcus pneumoniae assessed using the Chinchilla laniger model of otitis media. PLoS ONE. 2008, 3 (4): e1969-10.1371/journal.pone.0001969.PubMed CentralView ArticlePubMedGoogle Scholar
- Ulrich M, Albers C, Moller JG, Dalhoff A, Korfmann G, Kunkele F, Doring G: Moxifloxacin and azithromycin but not amoxicillin protect human respiratory epithelial cells against Streptococcus pneumoniae in vitro when administered up to 6 hours after challenge. Antimicrob Agents Chemother. 2005, 49 (12): 5119-5122. 10.1128/AAC.49.12.5119-5122.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Matsukawa M, Greenberg EP: Putative exopolysaccharide synthesis genes influence Pseudomonas aeruginosa biofilm development. J Bacteriol. 2004, 186 (14): 4449-4456. 10.1128/JB.186.14.4449-4456.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Jurcisek JA, Bakaletz LO: Biofilms formed by nontypeable Haemophilus influenzae in vivo contain both double-stranded DNA and type IV pilin protein. J Bacteriol. 2007, 189 (10): 3868-3875. 10.1128/JB.01935-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Moscoso M, Claverys JP: Release of DNA into the medium by competent Streptococcus pneumoniae: kinetics, mechanism and stability of the liberated DNA. Mol Microbiol. 2004, 54 (3): 783-794. 10.1111/j.1365-2958.2004.04305.x.View ArticlePubMedGoogle Scholar
- Whitchurch CB, Tolker-Nielsen T, Ragas PC, Mattick JS: Extracellular DNA required for bacterial biofilm formation. Science. 2002, 295 (5559): 1487-10.1126/science.295.5559.1487.View ArticlePubMedGoogle Scholar
- Guidolin A, Morona JK, Morona R, Hansman D, Paton JC: Nucleotide sequence analysis of genes essential for capsular polysaccharide biosynthesis in Streptococcus pneumoniae type 19F. Infect Immun. 1994, 62 (12): 5384-5396.PubMed CentralPubMedGoogle Scholar
- Morona JK, Paton JC, Miller DC, Morona R: Tyrosine phosphorylation of CpsD negatively regulates capsular polysaccharide biosynthesis in Streptococcus pneumoniae. Mol Microbiol. 2000, 35 (6): 1431-1442. 10.1046/j.1365-2958.2000.01808.x.View ArticlePubMedGoogle Scholar
- Briles DE, Novak L, Hotomi M, van Ginkel FW, King J: Nasal colonization with Streptococcus pneumoniae includes subpopulations of surface and invasive pneumococci. Infect Immun. 2005, 73 (10): 6945-6951. 10.1128/IAI.73.10.6945-6951.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Cundell DR, Weiser JN, Shen J, Young A, Tuomanen EI: Relationship between colonial morphology and adherence of Streptococcus pneumoniae. Infect Immun. 1995, 63 (3): 757-761.PubMed CentralPubMedGoogle Scholar
- Kim JO, Weiser JN: Association of intrastrain phase variation in quantity of capsular polysaccharide and teichoic acid with the virulence of Streptococcus pneumoniae. J Infect Dis. 1998, 177 (2): 368-377.View ArticlePubMedGoogle Scholar
- Magee AD, Yother J: Requirement for capsule in colonization by Streptococcus pneumoniae. Infect Immun. 2001, 69 (6): 3755-3761. 10.1128/IAI.69.6.3755-3761.2001.PubMed CentralView ArticlePubMedGoogle Scholar
- Weiser JN, Austrian R, Sreenivasan PK, Masure HR: Phase variation in pneumococcal opacity: relationship between colonial morphology and nasopharyngeal colonization. Infect Immun. 1994, 62 (6): 2582-2589.PubMed CentralPubMedGoogle Scholar
- Weiser JN, Markiewicz Z, Tuomanen EI, Wani JH: Relationship between phase variation and colony morphology, intrastrain variation in cell wall physiology, and nasal colonization by Streptococcus pneumoniae. Infect Immun. 1996, 64 (6): 2240-2245.PubMed CentralPubMedGoogle Scholar
- Shen K, Gladitz J, Antalis P, Dice B, Janto B, Keefe R, Hayes J, Ahmed A, Dopico R, Ehrlich N, Jocz J, Kropp L, Yu S, Nistico L, Greenberg DP, Barbadora K, Preston RA, Post JC, Ehrlich GD, Hu FZ: Characterization, distribution, and expression of novel genes among eight clinical isolates of Streptococcus pneumonia. Infect Immun. 2006, 74 (1): 321-330. 10.1128/IAI.74.1.321-330.2006.PubMed CentralView ArticlePubMedGoogle Scholar
- Heydorn A, Toftgaard Nielsen A, Hentzer M, Sternberg C, Givskov M, Kjær Ersbøll B, Molin S: Quantification of biofilm structures by the novel computer program COMSTAT. Microbiology. 2000, 146 (10): 2395-2407.View ArticlePubMedGoogle Scholar
- Sambanthamoorthy K, Smeltzer MS, Elasri MO: Identification and characterization of msa (SA1233), a gene involved in expression of SarA and several virulence factors in Staphylococcus aureus. Microbiology. 2006, 152 (Pt 9): 2559-2572. 10.1099/mic.0.29071-0.View ArticlePubMedGoogle Scholar
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