Adhesion to and biofilm formation on IB3-1 bronchial cells by Stenotrophomonas maltophilia isolates from cystic fibrosis patients
© Pompilio et al; licensee BioMed Central Ltd. 2010
Received: 30 September 2009
Accepted: 7 April 2010
Published: 7 April 2010
Stenotrophomonas maltophilia has recently gained considerable attention as an important emerging pathogen in cystic fibrosis (CF) patients. However, the role of this microorganism in the pathophysiology of CF lung disease remains largely unexplored. In the present study for the first time we assessed the ability of S. maltophilia CF isolates to adhere to and form biofilm in experimental infection experiments using the CF-derived bronchial epithelial IB3-1cell line. The role of flagella on the adhesiveness of S. maltophilia to IB3-1 cell monolayers was also assessed by using fliI mutant derivative strains.
All S. maltophilia CF isolates tested in the present study were able, although at different levels, to adhere to and form biofilm on IB3-1 cell monolayers. Scanning electron and confocal microscopy revealed S. maltophilia structures typical of biofilm formation on bronchial IB3-1 cells. The loss of flagella significantly (P < 0.001) decreased bacterial adhesiveness, if compared to that of their parental flagellated strains. S. maltophilia CF isolates were also able to invade IB3-1 cells, albeit at a very low level (internalization rate ranged from 0.01 to 4.94%). Pre-exposure of IB3-1 cells to P. aeruginosa PAO1 significantly increased S. maltophilia adhesiveness. Further, the presence of S. maltophilia negatively influenced P. aeruginosa PAO1 adhesiveness.
The main contribution of the present study is the finding that S. maltophilia is able to form biofilm on and invade CF-derived IB3-1 bronchial epithelial cells, thus posing a rationale for the persistence and the systemic spread of this opportunistic pathogen in CF patients. Experiments using in vivo models which more closely mimic CF pulmonary tissues will certainly be needed to validate the relevance of our results.
Cystic fibrosis (CF) is a common inherited genetic disorder, caused by a mutation in the gene encoding the cystic fibrosis transmembrane conductance regulator (CFTR) protein  which is expressed in many different cells. In the lung, the derived chloride transport defect leads to altered airway physiology including impairment of mucociliary clearance, production of plugs of thick mucus and impaired innate immunity [2, 3]. These defects predispose the CF patient to microbial colonization and thus, to infections that tend to become chronic. The likelihood of contracting chronic infections increases with age and Pseudomonas aeruginosa becomes the dominant infecting microorganism, with a colonization percentage varying from 42 to 100% .
Recently, Stenotrophomonas maltophilia has gained considerable attention as an important emerging nosocomial pathogen able to cause infections in debilitated and immunocompromised patients, as well as in CF patients [5, 6]. Colonization of the pulmonary tissues occurs in approximately one third of CF patients, nevertheless, there is controversy as whether S. maltophilia colonization leads to a poorer clinical outcome or morbidity [7–9]. Persistent colonization by P. aeruginosa and the attendant damage of the epithelial mucosa by released pseudomonal exoproducts may increase the probability that S. maltophilia will colonize the respiratory tract of CF patients and significantly contribute to the progressive deterioration of their pulmonary functions [10, 11]. However, the mechanism of pathogenicity enabling S. maltophilia to establish infection and chronic colonization of the respiratory tract of CF patients remains largely unexplored.
Biofilm formation is increasingly recognized as an important bacterial virulence trait contributing to disease progression in CF and other diseases of the respiratory tract associated with chronic infections. Biofilm growth is believed to protect bacteria from natural immune defenses, as well as from the actions of several antibiotic compounds [12, 13]. P. aeruginosa strains isolated from the sputum of CF patients display morphologic and physiologic characteristics suggestive of in vivo biofilm formation, including over a 1000-fold increase in antibiotic resistance and a significant ability in evading host defense factors [14–17].
S. maltophilia has been recently reported to be able to adhere to cultured epithelial respiratory cells, as well as to produce biofilm on a variety of abiotic surfaces [10, 18, 19]. In particular, S. maltophilia strains isolated from CF patients were shown to be able, although with striking differences, to adhere to and form biofilm on polystyrene . Since information on the ability of S. maltophilia to grow as biofilm in CF airway tissues is scarce, in the study described in this paper we evaluated, by quantitative assays and microscopic analysis (scanning electron and confocal laser microscopy), the ability of CF S. maltophilia strains to adhere, invade and form biofilm on CF-derived IB3-1 bronchial epithelial cell monolayers. Moreover, the role of flagella in adhesiveness on IB3-1 epithelial cells was also evaluated by the construction of two independent S. maltophiia fliI deletion mutants that were used to infect cultured monolayers. Some of the results of the present study have been previously presented in the form of an abstract at the 18th European Congress of Clinical Microbiology and Infectious Diseases .
S. maltophilia is able to adhere to and form biofilm on IB3-1 cell monolayers
Microbiological features of S. maltophilia OBGTC strains (n = 12) used in this study.
Chronic lung infection isolateb
Past P. aeruginosa infection
With regard to biofilm formation, as judged by the number of cfu recovered after 24 hours of incubation, S. maltophilia strain OBGTC37 produced the highest amount of biofilm (5.4 ± 0.8 × 107 cfu chamber-1) (Figure 1B), a value significantly higher if compared to the other strains tested (P < 0.001). No significant correlation was found between adhesiveness and the amount of biofilm formed (Pearson r, 0.158; P > 0.05).
Flagella are involved in S. maltophilia adhesion to IB3-1 cell monolayers
Contrary to wt strains, exposure of IB3-1 cells to OBGTC9 and -10 fliI mutant strains for 24 hours disrupted cell monolayer. Thus, results about biofilm formation by mutant strains are not available.
S. maltophilia is able to adhere to and form biofilm on polystyrene
S. maltophilia internalizes within IB3-1 cells at low levels
To ascertain whether our strains of S. maltophilia are able to enter IB3-1 cells, bacterial internalization was evaluated by a classical antibiotic exclusion assay. Due to high-level of gentamicin resistance, only 5 strains were tested for invasiveness. Gentamicin was highly effective on inhibiting the growth of the S. maltophilia strains (inhibition of growth ≥ 99.9%, data not shown) and was proved to be not toxic for IB3-1 cells even when they were exposed up to 1200 μg ml-1, as assessed by the XTT assay (data not shown).
The results of the invasion experiments indicated that all strains tested were able to invade IB3-1 cells, albeit at a very low level. Viable intracellular bacteria represented only a minor fraction of the total bacterial input used to infect cell monolayers.
Internalization rates (cfus released upon cell lysis, compared to cfus used to infect cell monolayers) were 0.54, 0.01, 4.94, 2.48, 0.03% for OBGTC9, OBGTC10, OBGTC37, OBGTC38, and OBGTC50, respectively. Internalization levels (expressed as number of internalized bacteria) were not significantly related to adhesion levels (expressed as number of adhered bacteria) (Pearson r: 0.044, P > 0.05).
Swimming and twitching motilities are not involved in S. maltophilia adhesion to and biofilm formation on IB3-1 cells
The motility of our twelve S. maltophilia clinical isolates was assessed by swimming and twitching assays, as described in Materials and Methods. S. maltophilia strains exhibited a very broad range of motility (data not shown). Ten out of 12 (83.3%) strains showed swimming motility, ranging from 4 mm (strain OBGTC49) to 17 mm (strain OBGTC5). Strains OBGTC52 and OBGTC50 did not exhibit swimming motility. All strains were able to move by twitching, ranging from 3 mm (strain OBGTC49) to 15 mm (strain OBGTC37). Neither swimming nor twitching motility significantly correlated with adhesiveness to or biofilm formation on IB3-1 cells (data not shown). As expected, both OBGTC9 and OBGTC10 fliI deletion mutants failed to show swimming motility (Figure 4B).
Pre-exposure to P. aeruginosa influences S. maltophilia adhesion to IB3-1 cell monolayers
Although recent clinical evidence highlights an increase in the frequency of isolation of S. maltophilia from respiratory tract of CF patients, the role of this microorganism in the pathophysiology of CF lung disease, as well as patient-to-patient spread, have not yet been clearly elucidated [5, 7–9]. Moreover, the correlation between S. maltophilia persistent lung colonization and reduced pulmonary function first reported by Karpati et al , has not yet been confirmed by further studies [23–26]. On the other hand, the increased isolation of S. maltophilia from the sputa of CF patients has become a cause of concern in the CF community, as the organism is highly resistant to many of the antibiotics prescribed in CF management .
Because of its increasing clinical relevance, its high level of antibiotic-resistance, and the paucity of information on its specific role in the pathogenesis of CF lung infections, new information regarding the interactions between S. maltophilia and CF airway tissues are of paramount importance. To our knowledge, this is the first study which evaluated the ability of CF-derived S. maltophilia clinical isolates to adhere to and form biofilm in experimental infection experiments using the CF-derived bronchial epithelial IB3-1cell line.
Employing an in vitro static culture model, by using electron and confocal microscopy and determining the number (cfu) of attached bacteria at different time points post-infection, we showed that all the twelve studied CF-derived S. maltophilia isolates were able, although at different levels, to adhere and form biofilm when co-cultured with IB3-1 cell monolayers. Such results suggest that these characteristics might be highly conserved among S. maltophilia strains isolated from CF patients. Electron and confocal microscopy revealed S. maltophilia structures typical of biofilm formation on almost all bronchial IB3-1 cells. In particular, the overall cellular areas occupied by bacteria and their numbers are suggestive of the formation of microcolony, a finding reminiscent of the "flat" biofilm phenotype produced by P. aeruginosa, significantly different from the "mushroom-like" phenotype . Electron microscopy photographs revealed that S. maltophilia adhered to IB3-1 cells loses its cell profile, probably due to the presence of extracellular matrix. In fact, CLSM examination showed microcolony embedded in extracellular matrix whose production was significantly increased following exposure to S. maltophilia.
The ability of S. maltophilia to form biofilm on IB3-1 cells may contribute to explain why S. maltophilia tends to produce persistent infections in chronic obstructive pulmonary disease despite intensive antibiotic treatment . In this context, it is worth mentioning that some antibiotic-resistant S. maltophilia strains may persist in CF patients pulmonary tissue for up to 3 years, and that many patients are colonized at the same time with multiple strains of S. maltophilia .
Invasion of epithelial respiratory cells has been reported for CF-derived S. maltophilia clinical isolates [10, 20]. We have recently reported that, with the exception of an environmental S. maltophilia isolate (strain LMG959) all the CF-derived strains assayed were able to invade A549 cells . In the present study we evaluated the ability of twelve S. maltophilia CF isolates to invade IB3-1 cells, by classical invasion assays. The results obtained clearly indicated, for the first time, that S. maltophilia CF isolates were able to invade IB3-1 cells, albeit at a very low level (data not shown). Since strains presented a significant degree of heterogeneity in internalization efficiencies, it might be possible to hypothesize that S. maltophilia entry within IB3-1 cells may be strain-dependent. Together with the ability to form biofilm, the capability of S. maltophilia to enter IB3-1 might also explain the tendency of this microorganism to become persistent within CF pulmonary tissues, since within intracellular compartments it could find protection against host defenses and the reach of antibiotics. Moreover, internalization may likely influence the modulation of the inflammatory response of the infected host.
It has been reported that flagella could act as adhesins which play a role in bacterial binding to host mucosal surfaces as well as to abiotic surfaces [22, 31]. To study the role of flagella in the adhesiveness of S. maltophilia, we generated two independent mutants presenting a deletion encompassing the fliI gene of S. maltophilia strains OBGTC9 and OBGTC10. fliI encodes a substrate-specific ATPase (FliI), an enzyme necessary to provide energy for the export of flagellar structural components in a wide range of bacterial species . Swimming ability of the two mutant strains was almost completely abolished (Figure 4B). When co-cultured with IB3-1 cell monolayers, the two mutants showed a reduced capacity to adhere to IB3-1 cells, if compared to that of parental wild type strains (Figure 4A). Further, we showed that neither swimming nor twitching motilities were significantly associated to adhesion to or biofilm formation on IB3-1 cells. Thus, taken together, our results suggest that although flagella must play some role in S. maltophilia adhesiveness, regardless of their functionality, other structures must also be involved in this phenomenon, since the fliI mutation only attenuates, but not abolishes, the ability of S. maltophilia strains to adhere to IB3-1 cells.
We were not able to assess the role of flagella in S. maltophilia biofilm formation since exposure of IB3-1 monolayers to fliI- mutant strains caused their disruption already after 6h-exposure. Further investigations are warranted to explain this apparent increased virulence following the loss of motility.
A number of methods have been developed for cultivation and quantification of biofilms , but no standardized protocol for assessment of biofilm formation has been established so far. Nevertheless, the microtiter plate method remains among the most frequently used assays for investigation of biofilm formation, and a number of modifications have been developed for the cultivation and quantification of bacterial biofilms . Since S. maltophilia biofilm formation on abiotic surfaces is generally considered less relevant than biofilm formation on cultured epithelial cells or in vivo, in this study we assayed biofilm formation onto an abiotic surface and compared the results to the ability of our S. maltophilia strains to form biofilm on IB3-1 cells, as assessed by quantitative colony counts. In agreement with previously reported experiments [20, 34], all the twelve S. maltophilia clinical isolates tested were able to form biofilm on both polystyrene and IB3-1 cultured epithelial cells. However, no correlation was found between quantitative biofilm formation on the abiotic surface and qualitative biofilm formation on cultured cell monolayers, thus suggesting that the microtiter plate assay may not be predictive of the ability of S. maltophilia to form biofilm in vivo. Several explanations may account for this discrepancy. The crystal violet assay is surely a less specific method, and it is likely that the dye might also stain negatively charged extracellular molecules, including cell surface molecules and polysaccharides present in the extracellular matrix in mature biofilms, thus influencing the outcome of the test. Further studies are certainly needed to clarify this point.
Recent studies from different laboratories have highlighted the importance of interspecies bacterial interactions in influencing bacterial virulence and response to antibiotic therapy, both in pulmonary infections of CF and non-CF patients [35, 36]. In CF patients, there are several lines of evidence indicating the presence of a mosaic of diverse bacteria so that infections of CF pulmonary tissues are usually considered always polymicrobial . Recently, Ryan et al.  have reported that the presence of S. maltophilia significantly influences, as through the synthesis of a diffusible signal factor, the architecture of P. aeruginosa biofilm formation and augments its susceptibility to polymyxins, recently re-introduced into clinical practice as anti-pseudomonal agents.
In general, S. maltophilia is very often co-isolated with P. aeruginosa from CF patients [6, 25, 39, 40] and it has been hypothesized that infection by P. aeruginosa may enhance the chance of S. maltophilia to colonize CF pulmonary tissues [12, 13]. If this is true, it is reasonable to hypothesize that P. aeruginosa might enhance the ability of S. maltophilia to adhere to and/or invade CF pulmonary tissues. In order to analyze this possibility we first infected IB3-1 cell monolayers with reference P. aeruginosa PAO1 strain, and then with S. maltophilia strain OBGTC9 (the most adhesive of our group of strains; Figure 1A). The results obtained showed that while P. aeruginosa PAO1 binds more efficiently to cell monolayers than does S. maltophilia OBGTC9, a previous exposition of IB3-1 cell monolayers to P. aeruginosa PAO1 significantly improves S. maltophilia adhesiveness; therefore, it suggests a synergistic relationship between these pathogens similarly to what reported by Saiman et al.  who found a synergistic relationship between P. aeruginosa and P. cepacia. Demonstrating this, most (9 out of 12, 75%) of S. maltophilia-positive CF patients considered in the present study was found to have been infected in the past with P. aeruginosa (Table 1).
Although the pathogenic role of S. maltophilia in CF lung disease is unclear and subject to controversy, the results of the present study suggest that this microorganism should not be considered just a bystander in CF patients. In this respect, we have shown that : i) S. maltophilia is able to adhere to and invade CF-derived IB3-1 cultured bronchial epithelial cells; ii) the ability of S. maltophilia strains to form biofilm and to invade epithelial cells might account for the persistence and the systemic spread of this opportunistic pathogen in CF patients; iii) a previous infection by P. aeruginosa may have an impact on S. maltophilia colonization of CF pulmonary tissues.
Further experiments using in vivo models which more closely mimic CF pulmonary tissues are certainly needed to validate the relevance of our results. Furthermore, our model may be useful to study the different stages of the intricate relationships between S. maltophilia and the CF airway epithelium, if compared to the abiotic model method. This may help in the development of new strategies for preventive and/or therapeutic intervention against the factors that trigger CF airways colonization by S. maltophilia.
Bacterial strains and culture conditions
Twelve S. maltophilia strains, herein designated as OBGTC, were used in this study (Table 1). All strains were isolated from the respiratory secretions of CF patients admitted to CF Unit of Pediatric Hospital "Bambino Gesù" of Rome. The isolates were identified as S. maltophilia by conventional biochemical tests (API 20-NE System; BioMérieux, Marcy-L'Etoile, France). P. aeruginosa PAO1 was used as a reference strain in IB3-1 co-infection experiments with S. maltophilia. Strains were kept at -80°C and grown overnight at 37°C on Mueller-Hinton or Trypticase Soy broth or agar (Oxoid; Garbagnate Milanese, Italy).
IB3-1 cells (ATCC#CRL-2777) are transformed bronchial epithelial cells isolated from a pediatric CF patient who harbored the ΔF508/W1282X mutations within the CFTR gene. Cells were grown at 37°C in LHC-8 medium supplemented with 5% fetal bovine serum (FBS) (Gibco, Italy) in a 5% CO2atmosphere.
Bacteria used to infect cell monolayers were grown in Trypticase Soy broth overnight at 37°C, under agitation (90 rpm), washed twice in sterile phosphate buffered solution (PBS; Sigma-Aldrich, Milan, Italy) and resuspended in LHC-8 medium (BioSource; Camarillo, Ca) to an OD550 = 0.450, corresponding to about 5 × 108 cfu ml-1. The concentration (cfu ml-1) of each bacterial suspension used to infect cultured cells was always determined.
Construction of S. maltophilia flagellar mutants (fliI-)
S. maltophilia fliI chromosomal knockout mutants of strains OBGTC9 and OBGTC10 were constructed by using the gene replacement vector pEX18Tc, as described by Hoang et al. . Briefly, a 2509-bp fragment, encompassing the entire ORF of the fliI gene, was PCR-amplified from total DNA preparations of S. maltophilia K279a reference strain using primers fliI Fw [5'-GGGGGGATCCAAGTCCTTTCCGCCTTCGCT-3' (the bold sequence corresponds to a Bam HI restriction site)] and fliI Rv [GGGGGAAGCTTGACAACTTCAGCCGACCGCT-3' (the bold sequence indicates a Hind III restriction site)]. The PCR-amplified fragment was digested with BamH I/Hind III and then cloned into the multicloning site of plasmid pEX18Tc, digested with the same restriction enzymes, thus generating plasmid pEX18ap. Next, a 971-bp cloramphenicol resistance cassette was PCR amplified from plasmid pACYC184 using the primer pair cat Fw [5'GGGGGGCTGCAGGCACCTCAAAAACACCATCATACA-3' (the bold sequence corresponds to a Pst I restriction site)] and cat RV [5'-GGGGGGTCGACCAGGCGTTTAAGGGCACCAATA-3' (the bold sequence indicates a Sal I restriction site)]. To generate a 1321-bp deletion within the internal coding region of fliI, the amplified 971-bp fragment was Pst I/Sal I digested and then cloned into plasmid pEX18Tap which had previously been digested with the same enzymes, thus generating plasmid pPEX53ap. pPEX53ap was introduced into E. coli S17-1 and independently mobilized into S. maltophilia strains OBGTC9 and OBGTC10 via conjugation. Transconjugants were selected on LB agar supplemented with 20 μg ml-1 of tetracycline, 10 μg ml-1 of cloramphenicol and 10 μg ml-1 of kanamicin. Emerging resistant colonies were streaked on LB agar supplemented with 10% (wt vol-1) sucrose and then incubated overnight at 37°C. On the following day, sucrose-resistant colonies were screened for cloramphenicol resistance by growing individual colonies in LB plates supplemented with cloramphenicol. The inactivation of the fliI gene in chloramphenicol resistant colonies was confirmed by PCR amplification, Southern blot hybridization (data not shown) and swimming motility assays.
Adhesiveness and biofilm formation on IB3-1 cultured monolayers
The ability of the twelve S. maltophilia strains and of the two independent OBGTC9 and OBGTC10 fliI deletion mutants to adhere to and form biofilms on IB3-1 cell monolayers was assayedusing a static co-culture model system. Briefly, IB3-1 cells were cultured in 8-well polystyrene chambers (CultureSlides, BD Falcon, Milan, Italy) seeded with 3 × 105 cells chamber-1, and grown to confluence in LHC-8 complete medium at 37°C and 5% CO2. Before seeding, wells were coated with 0.01 mg ml-1 human fibronectin (BD Falcon), 0.03 mg ml-1 bovine type 1 collagen (BD Falcon), and 0.01 mg ml-1 bovine serum albumin (Sigma-Aldrich). Monolayers were infected with approximately 2.5 × 108 cells of each S. maltophilia strain analyzed, suspended in LHC-8 medium to obtain a multiplicity of infection (MOI) of approximately 1000, relative to the number of cells originally seeded. After 2 (adhesion assay) or 24 hours (biofilm assay) of incubation at 37°C, infected monolayers were washed three times with PBS to remove non-adherent bacteria and treated with 0.25% trypsin/EDTA (Sigma-Aldrich) for 10 minutes. Cells were recovered and then vortexed for 3 minutes, serially diluted, and bacteria plated on MH agar to determine the number (cfu chamber-1) of bacteria which adhered to IB3-1 cells.
Epithelial-monolayer integrity was assessed at 2 and 24 hours post-infection by confocal laser scanning and phase-contrast microscopy.
Bacterial internalization assays
As described above, confluent IB3-1 cell cultures were infected with S. maltophilia strains (MOI 1000). After 2 hours of incubation at 37°C, infected monolayers were extensively washed with sterile PBS, and further incubated for other 2 hours in LHC-8 medium supplemented with gentamicin sulphate (600 μg ml-1; Sigma-Aldrich) in order to kill extracellular bacteria. We had previously determined that, at this concentration, gentamicin inhibits S. maltophilia growth by 99.9% (data not shown). At the end of the experiments, infected monolayers were extensively washed in PBS, then lysed with a solution of 0.1% Triton X-100 (Sigma-Aldrich) in PBS for 10 minutes at room temperature to count internalized bacteria. Aliquots of cell lysates were serially diluted and plated to quantify viable intracellular bacteria (cfu chamber-1).
Evaluation of toxicity of gentamicin towards IB3-1 cells was assessed by an XTT-based colorimetric assay (Cell Proliferation Kit II; Roche, Milan, Italy). Briefly, 500 μl of a mixture of XTT (1 mg ml-1) supplemented with 1.25 mM N-methyl dibenzopyrazine methyl sulfate was added to the wells containing cells incubated for 2 hours in LHC-8 medium supplemented with different concentrations (150 to 1200 μg ml-1) of gentamicin. IB3-1 cells not treated with gentamicin were used as control. Absorbance of supernatants was then measured at 492 nm in an ELISA plate reader (SpectraMax; Applied BioSystem Italia, Monza, Italy), subtracting background absorbance at 650 nm.
Adhesiveness and biofilm formation on a polystyrene abiotic surface
Five-hundred microliters aliquots of bacterial cultures containing approximately 5 × 108 cfu ml-1 were disposed on independent void wells of a sterile 48-wells flat-bottom polystyrene tissue culture plate (Iwaki; Bibby Scientific Italia, Riozzo di Cerro al Lambro, Milan, Italy). Bacteria were incubated at 37°C for 2 (adhesion assay) or 24 hours (biofilm assay) in a closed, humidified plastic container. At the end of the experiment, the medium was discarded, and non-adherent bacteria were removed by three washes with sterile PBS. Quantification of bacterial adhesiveness and biofilm formation on polystyrene was assessed by a spectrophotometric method, as previously described by Christensen et al. , with minor modifications. Briefly, after washing, attached bacteria were fixed for 1 hour at 60°C and then stained with Hucker crystal violet solution for 5 minutes. After washing with water to remove the excess of stain, the plates were dried for 30 minutes at 37°C. The color produced by attached bacteria (indirect index of adhesiveness or biofilm formation) was measured spectrophotometrically at OD492. A low cut-off corresponding to 3 standard deviations (SDs) above the mean of control wells not seeded with bacteria was chosen .
Co-infection assays were performed using S. maltophilia strain OBGTC9 and P. aeruginosa strain PAO1. Briefly, confluent IB3-1 cell monolayers were first infected for 2 hours at 37°C with P. aeruginosa PAO1 (MOI 1000). At that time, non-adherent bacteria were removed by three washes with PBS, and monolayers were then infected with S. maltophilia strain OBGTC9 (MOI 1000) and incubated for further 2 hours. At the end of the experiment infected IB3-1 cells were removed by a treatment with 0.25% trypsin/EDTA, vortexed, serially diluted and plated on MH agar to determine the number (cfu chamber-1) of the two bacteria bound to IB3-1 cells. P. aeruginosa PAO1 and S. maltophilia OBGTC10 colonies were easily differentiated on the basis of their colonial morphology. As controls we used IB3-1 cell monolayers infected separately with each of the two bacterial strains.
Swimming motility assays were performed with single well-isolated colonies grown overnight on MH agar plates, according to a modification of the technique described by Rashid et al. . Briefly, tryptone swim plates (1% tryptone, 0.5% NaCl, 0.3% agar; Oxoid) were inoculated with bacteria at the surface by using a sterile needle. Plates were incubated for 24 hours at 37°C. Motility was assessed by calculating the diameter (mm) of the circular turbid zone formed by bacterial cells migrating away from the point of inoculation at the agar surface.
Scanning electron microscopy
Biofilm formation was assessed by scanning electron microscopy (SEM). Samples were air-dried, and fixed with a solution of 2.5% glutaraldehyde in 0.1 M sodium cacodylate buffer for 90 minutes. After washing with buffer, samples were post-fixed in osmium tetroxide and then dehydrated in a series of aqueous ethanol solutions (30 to 70%). Specimens were mounted on aluminum stubs with conductive carbon cement, allowed to dry for 3 hours, and coated with 15-nm Au film with an agar automatic sputter coater. After processing, samples were observed with a Philips XL30CP scanning electron microscope in the high-vacuum mode at 15 kV.
Confocal laser scanning microscopy (CLSM)
CLSM was carried out on fresh and formaldehyde-paraformaldehyde fixed samples. Briefly, infected IB3-1 cell monolayers, prepared as stated above, were stained with Live/Dead BacLight kit (Molecular Probes Inc.) and Concanavalin A (Alexa Fluor 647 coniugate; Molecular Probes Inc.). IB3-1 monolayer not exposed to S. maltophilia was used as control. CLSM analysis was performed with an LSM 510 META laser scanning microscope attached to an Axioplan II microscope (Zeiss). Three-dimensional reconstructions of imaged samples were obtained by Amira 3.1.1 (Mercury Computer Systems; Chelmsford, MA) software. Images were captured and processed for display using Adobe Photoshop (Adobe Systems Inc.) software.
All experiments were performed in triplicate and repeated on two different occasions. Results were expressed as means ± SDs. Analyses of statistical significance were performed by ANOVA-test followed by Newman-Keuls multiple comparison post-test (adhesiveness and biofilm formation on IB3-1 cells, adhesiveness of fliI mutants, internalization within IB3-1 cell monolayers and co-infection experiments) or Kruskall-Wallis + Dunn's multiple comparison post-test (adhesiveness and biofilm formation on polystyrene). Interdependency between variables was evaluated by Pearson's linear correlation coefficient. P values < 0.05 were considered as statistically significant.
This work was partially supported by the Italian Cystic Fibrosis Research Foundation (grant #7/2007, adopted by Vicenzi Biscotti S.p.A.) and by the Italian Ministry of Education, University, and Research (PRIN 2007). We gratefully thank Ester D'Addetta for technical assistance and Andreina Santoro for reviewing the manuscript.
- Boucher RC: New concepts of the pathogenesis of cystic fibrosis lung disease. Eur Respir J. 2004, 23: 146-158. 10.1183/09031936.03.00057003.View ArticlePubMedGoogle Scholar
- Saiman L, Siegel J: Infection control in cystic fibrosis. Clin Microbiol Rev. 2004, 17: 57-71. 10.1128/CMR.17.1.57-71.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Yoon SS, Hassett DJ: Chronic Pseudomonas aeruginosa infection in cystic fibrosis airway disease: metabolic changes that unravel novel drug targets. Expert Rev Anti Infect Ther. 2004, 2: 611-623. 10.1586/14787184.108.40.2061.View ArticlePubMedGoogle Scholar
- Lyczak JB, Cannon CL, Pier GB: Establishment of Pseudomonas aeruginosa infection: lessons from a versatile opportunist. Microbes Infect. 2000, 2: 1051-1060. 10.1016/S1286-4579(00)01259-4.View ArticlePubMedGoogle Scholar
- Waters VJ, Gómez MI, Soong G, Amin S, Ernst R, Prince A: Immunostimulatory properties of the emerging pathogen Stenotrophomonas maltophilia. Infect Immun. 2007, 75: 1698-1672. 10.1128/IAI.01469-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Denton M, Kerr KG: Microbiological and clinical aspects of infections associated with Stenotrophomonas maltophilia . Clin Microbiol Rev. 1998, 11: 57-80.PubMed CentralPubMedGoogle Scholar
- Steinkamp G, Wiedemann B, Rietschel E, Krahl A, Gielen J, Barmeier H, Ratjen F: Prospective evaluation of emerging bacteria in cystic fibrosis. J Cyst Fibros. 2005, 4: 41-48. 10.1016/j.jcf.2004.10.002.View ArticlePubMedGoogle Scholar
- Goss CH, Mayer-Hamblett N, Aitken ML, Rubenfeld GD, Ramsey BW: Association between Stenotrophomonas maltophilia and lung function in cystic fibrosis. Thorax. 2004, 59: 955-959. 10.1136/thx.2003.017707.PubMed CentralView ArticlePubMedGoogle Scholar
- Hadjiliadis D, Steele MP, Chaparro C, Singer LG, Waddell TK, Hutcheon MA, Davis RD, Tullis DE, Palmer SM, Keshavjee S: Survival of lung transplant patients with cystic fibrosis harbouring panresistant bacteria other than Burkholderia cepacia, compared with patients harboring sensitive bacteria. J Heart Lung Transplant. 2007, 26: 834-838. 10.1016/j.healun.2007.05.018.View ArticlePubMedGoogle Scholar
- De Abreu Vidipò L, De Andrade Marques E, Puchelle E, Plotkowski MC: Stenotrophomonas maltophilia interaction with human epithelial respiratory cells in vitro. Microbiol Immunol. 2001, 45: 563-569.View ArticleGoogle Scholar
- Karpati F, Malmborg AS, Alfredsson H, Hjelte L, Strandvik B: Bacterial colonisation with Xanthomonas maltophilia : a retrospective study in a cystic fibrosis patient population. Infection. 1994, 22: 258-263. 10.1007/BF01739911.View ArticlePubMedGoogle Scholar
- Costerton JW, Stewart PS, Greenberg EP: Bacterial biofilms: a common cause of persistent infections. Science. 1999, 284: 1318-1322. 10.1126/science.284.5418.1318.View ArticlePubMedGoogle Scholar
- Parsek MR, Singh PK: Bacterial biofilms: an emerging link to disease pathogenesis. Ann Rev Microbiol. 2003, 57: 677-701. 10.1146/annurev.micro.57.030502.090720.View ArticleGoogle Scholar
- Lam J, Chan R, Lam K, Costerton JW: Production of mucoid microcolonies by Pseudomonas aeruginosa within infected lungs in cystic fibrosis. Infect Immun. 1980, 28: 546-556.PubMed CentralPubMedGoogle Scholar
- Singh PK, Schaefer AL, Parsek MR, Moninger TO, Welsh MJ, Greenberg EP: Quorum-sensing signals indicate that cystic fibrosis lungs are infected with bacterial biofilms. Nature. 2000, 407: 762-764. 10.1038/35037627.View ArticlePubMedGoogle Scholar
- Nickel JC, Ruseska I, Wright JB, Costerton JW: Tobramycin resistance of Pseudomonas aeruginosa cells growing as a biofilm on urinary catheter material. Antimicrob Agents Chemother. 1985, 27: 619-624.PubMed CentralView ArticlePubMedGoogle Scholar
- Jesaitis AJ, Franklin MJ, Berglund D, Sasaki M, Lord CI, Bleazard JB, Duffy JE, Beyenal H, Lewandowski Z: Compromised host defense on Pseudomonas aeruginosa biofilms: characterization of neutrophil and biofilm interactions. J Immunol. 2003, 171: 4329-4339.View ArticlePubMedGoogle Scholar
- Di Bonaventura G, Spedicato I, D'Antonio D, Robuffo I, Piccolomini R: Biofilm formation by Stenotrophomonas maltophilia : modulation by quinolones, trimethoprim-sulfamethoxazole, and ceftazidime. Antimicrob Agents Chemother. 2004, 48: 151-160. 10.1128/AAC.48.1.151-160.2004.PubMed CentralView ArticlePubMedGoogle Scholar
- Huang TP, Somers EB, Wong AC: Differential biofilm formation and motility associated with lipopolysaccharide/exopolysaccharide-coupled biosynthetic genes in Stenotrophomonas maltophilia. J Bacteriol. 2006, 188: 3116-3120. 10.1128/JB.188.8.3116-3120.2006.PubMed CentralView ArticlePubMedGoogle Scholar
- Di Bonaventura G, Prosseda G, Del Chierico F, Cannavacciuolo S, Cipriani P, Petrucca A, Superti F, Ammendolia MG, Concato C, Fiscarelli E, Casalino M, Piccolomini R, Nicoletti M, Colonna B: Molecular characterization of virulence determinants of Stenotrophomonas maltophilia strains isolated from patients affected by cystic fibrosis. Int J Immunopathol Pharmacol. 2007, 20: 529-537.PubMedGoogle Scholar
- Di Bonaventura G, Pompilio A, Picciani C, Nicoletti M, Zappacosta R, Piccolomini R: Adhesion to and biofilm formation on IB3-1 bronchial cells by Stenotrophomonas maltophilia : implications in cystic fibrosis [abstract]. Clin Microbiol Infect. 2008, 14: s178-Google Scholar
- de Oliveira-Garcia D, Dall'Agnol M, Rosales M, Azzuz AC, Martinez MB, Girón JA: Characterization of flagella produced by clinical strains of Stenotrophomonas maltophilia . Emerg Infect Dis. 2002, 8: 918-923.PubMed CentralView ArticlePubMedGoogle Scholar
- O'Sullivan BP, Freedman SD: Cystic fibrosis. Lancet. 2009, 373: 1891-1904. 10.1016/S0140-6736(09)60327-5.View ArticlePubMedGoogle Scholar
- Ryan RP, Monchy S, Cardinale M, Taghavi S, Crossman L, Avison MB, Berg G, Lelie van der D, Dow JM: The versatility and adaptation of bacteria from the genus Stenotrophomonas . Nat Rev Microbiol. 2009, 7: 514-525. 10.1038/nrmicro2163.View ArticlePubMedGoogle Scholar
- Graff GR, Burns JL: Factors affecting the incidence of Stenotrophomonas maltophilia isolation in cystic fibrosis. Chest. 2002, 121: 1754-1760. 10.1378/chest.121.6.1754.View ArticlePubMedGoogle Scholar
- Goss CH, Otto K, Aitken ML, Rubenfeld GD: Detecting Stenotrophomonas maltophilia does not reduce survival of patients with cystic fibrosis. Am J Respir Crit Care Med. 2002, 166: 356-361. 10.1164/rccm.2109078.View ArticlePubMedGoogle Scholar
- Nicodemo AC, Paez JI: Antimicrobial therapy for Stenotrophomonas maltophilia infections. Eur J Clin Microbiol Infect Dis. 2007, 26: 229-237. 10.1007/s10096-007-0279-3.View ArticlePubMedGoogle Scholar
- Kirisits MJ, Parsek MR: Does Pseudomonas aeruginosa use intercellular signalling to build biofilm communities?. Cell Microbiol. 2006, 8: 1841-1849. 10.1111/j.1462-5822.2006.00817.x.View ArticlePubMedGoogle Scholar
- Ewig S, Soler N, Gonzalez J, Celis R, El-Ebiary M, Torres A: Evaluation of antimicrobial treatment in mechanically ventilated patients with severe chronic obstructive pulmonary disease exacerbations. Crit Care Med. 2000, 28: 692-697. 10.1097/00003246-200003000-00015.View ArticlePubMedGoogle Scholar
- Valdezate S, Vindel A, Maiz L, Baquero F, Escobar H, Cantón R: Persistence and variability of Stenotrophomonas maltophilia in cystic fibrosis patients, Madrid, 1991-1998. Emerg Infect Dis. 2001, 7: 113-122. 10.3201/eid0701.010116.PubMed CentralView ArticlePubMedGoogle Scholar
- Sampaio SC, Gomes TA, Pichon C, du Merle L, Guadagnini S, Abe CM, Sampaio JL, Le Bouguènec C: The flagella of an atypical enteropathogenic Escherichia coli are required for efficient interaction with and stimulation of IL-8 production by enterocytes in vitro. Infect Immun. 2009, 77 (10): 4406-13. 10.1128/IAI.00177-09.PubMed CentralView ArticlePubMedGoogle Scholar
- Yonekura K, Maki-Yonekura S, Namba K: Growth mechanism of the bacterial flagellar filament. Res Microbiol. 2002, 153: 191-197. 10.1016/S0923-2508(02)01308-6.View ArticlePubMedGoogle Scholar
- Stepanoviæ S, Vukoviæ D, Hola V, Di Bonaventura G, Djukiæ S, Cirkoviæ I, Ruzicka F: Quantification of biofilm in microtiter plates: overview of testing conditions and practical recommendations for assessment of biofilm production by staphylococci. APMIS. 2007, 15: 891-899. 10.1111/j.1600-0463.2007.apm_630.x.View ArticleGoogle Scholar
- Pompilio A, Piccolomini R, Picciani C, D'Antonio D, Savini V, Di Bonaventura G: Factors associated with adherence to and biofilm formation on polystyrene by Stenotrophomonas maltophilia : the role of cell surface hydrophobicity and motility. FEMS Microbiol Lett. 2008, 287: 41-47. 10.1111/j.1574-6968.2008.01292.x.View ArticlePubMedGoogle Scholar
- Hoffman LR, Déziel E, D'Argenio DA, Lépine F, Emerson J, McNamara S, Gibson RL, Ramsey BW, Miller SI: Selection for Staphylococcus aureus small-colony variants due to growth in the presence of Pseudomonas aeruginosa. Proc Natl Acad Sci USA. 2006, 103: 19890-19895. 10.1073/pnas.0606756104.PubMed CentralView ArticlePubMedGoogle Scholar
- Duan K, Dammel C, Stein J, Rabin H, Surette MG: Modulation of Pseudomonas aeruginosa gene expression by host microflora through interspecies communication. Mol Microbiol. 2003, 50: 1477-1491. 10.1046/j.1365-2958.2003.03803.x.View ArticlePubMedGoogle Scholar
- Sibley CD, Rabin H, Surette MG: Cystic fibrosis: a polymicrobial infectious disease. Future Microbiol. 2006, 1: 53-61. 10.2217/174609220.127.116.11.View ArticlePubMedGoogle Scholar
- Ryan RP, Fouhy Y, Garcia BF, Watt SA, Niehaus K, Yang L, Tolker-Nielsen T, Dow JM: Interspecies signalling via the Stenotrophomonas maltophilia diffusible signal factor influences biofilm formation and polymyxin tolerance in Pseudomonas aeruginosa. Mol Microbiol. 2008, 68: 75-86. 10.1111/j.1365-2958.2008.06132.x.View ArticlePubMedGoogle Scholar
- Senol E: Stenotrophomonas maltophilia : the significance and role as a nosocomial pathogen. J Hosp Infect. 2004, 57: 1-7. 10.1016/j.jhin.2004.01.033.View ArticlePubMedGoogle Scholar
- Looney WJ: Role of Stenotrophomonas maltophilia in hospital-acquired infection. Br J Biomed Sci. 2005, 62: 145-154.PubMedGoogle Scholar
- Saiman L, Cacalano G, Prince A: Pseudomonas cepacia adherence to respiratory epithelial cells is enhanced by Pseudomonas aeruginosa. Infect Immun. 1990, 58: 2578-2584.PubMed CentralPubMedGoogle Scholar
- Hoang TT, Karkhoff-Schweizer RR, Kutchma AJ, Schweizer HP: A broad-host-range Flp-FRT recombination system for site-specific excision of chromosomally-located DNA sequences: application for isolation of unmarked Pseudomonas aeruginosa mutants. Gene. 1998, 212: 77-86. 10.1016/S0378-1119(98)00130-9.View ArticlePubMedGoogle Scholar
- Christensen GD, Simpson WA, Younger JJ, Baddour LM, Barrett FF, Melton DM, Beachey EH: Adherence of coagulase-negative staphylococci to plastic tissue culture plates: a quantitative model for the adherence of staphylococci to medical devices. J Clin Microbiol. 1985, 22: 996-1006.PubMed CentralPubMedGoogle Scholar
- Rashid MH, Kornberg A: Inorganic polyphosphate is needed for swimming, swarming, and twitching motilities of Pseudomonas aeruginosa . Proc Natl Acad Sci USA. 2000, 97: 4885-4890. 10.1073/pnas.060030097.PubMed CentralView ArticlePubMedGoogle Scholar
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