Shigella flexneri is a highly contagious facultative intracellular pathogen causing acute inflammatory enteritis in human. Following infection of epithelial cells and macrophages, S. flexneri escapes from the phagocytic vacuoles via Ipa-mediated vacuole membrane lysis and enters the cytoplasm, where active proliferation takes place (Philpott, Edgeworth & Sansonetti, 2000; Schroeder & Hilbi, 2008). Bacteria then spread intra- and intercellularly by recruiting the cellular actin polymerization machinery with the help of the intra/intercellular spread factor, IcsA (Lett et al., 1989; Suzuki & Sasakawa, 2001). While the invasion process and immune evasion of S. flexneri have been extensively studied, the early adhesion process has not been adequately understood since Shigella flexneri lacks general adhesion machinery and exhibits relatively poor adhesiveness compared with other pathogenic enterobacteria (Brotcke Zumsteg et al., 2014; Carayol & Tran Van Nhieu, 2013; Phalipon & Sansonetti, 2007; Pizarro-Cerdá & Cossart, 2006).
LPS is a glycolipid located in the outer membrane of Gram-negative bacteria. It is composed of three covalently linked domains: lipid A, which is embedded in the outer membrane; the oligosaccharide core including inner and outer parts; and repeats of the O-polysaccharide or O-antigen, which cover the bacterial surface. As an essential pathogenic component, LPS of gram-negative bacteria triggers strong immune responses, which are directly related to the adverse clinical outcomes (Alexander & Rietschel, 2001; Wang & Quinn, 2010). In contrast to the highly variable and antigenic O-antigen portion, the core oligosaccharide (OS), especially the inner (lipid A-proximal) core, composed of two 3-deoxy-Dmanno-oct-2-ulosonic acids (Kdo) and three L-glycero-D-mannoheptose (Hep), called HepI, HepII, and HepIII, is conserved across E. coli, Shigella and Salmonella and possesses limited structural variation. Therefore, targeting the core OS for general therapeutic application has been considered as an alternative strategy against antibiotics-resistant Gram-negative bacterial infection (Desroy et al., 2009; Di Padova et al., 1993; Moreau et al., 2008). Although inhibition of Kdo biosynthesis is usually lethal to bacteria, a defect in Hep biosynthesis results in a viable bacterial cell with a characteristic “deep rough” phenotype (Grizot et al., 2006; Klena et al., 2005).
Biofilm, a microorganism community formed on an environmental surface and by cell aggregation has been implicated in around 80% of microbial infections in vivo (Hall-Stoodley, Costerton & Stoodley, 2004) (Davies, 2003). Nevertheless, the relevance of biofilm formation to Shigella virulence has not been thoroughly interrogated. Recent studies have shown that LPS composition regulates biofilm formation besides the previously reported association with variations in salt concentration, starvation or changes in pH (Ellafi et al., 2012). For example, deficiency in Hep synthesis in E. coli resulted in dramatic biofilm formation on abiotic surface, which is caused by enhanced hydrophobicity of the bacteria surface due to the loss of oligosaccharide (Nakao et al., 2012). Although Shigella LPS has been extensively studied through deletion of a serious of genes involved in LPS synthesis, disruption of Hep biosynthesis has never been reported in Shigella so far (Hong & Payne, 1997; Martini et al., 2011; Sandlin et al., 1995).
In this study, we characterized biofilm forming potentials and pathological behaviors of various LPS-truncated Shigella flexneri strains. Analysis of the LPS mutants revealed that the autoaggregation and biofilm forming capacity of Shigella negatively correlated with the LPS chain length in general. The deep-rough LPS mutant ΔrfaC, characteristic of strong biofilm formation abilities, exhibited much more adhesive and invasive than the parental strain and other LPS mutants, albeit with undermined fitness. Immunofluorescence analysis revealed that the ΔrfaC strain exhibited distinct patterns of IcsA distribution and F-actin recruitment. Finally, using the guinea pig keratoconjunctivitis model, we showed that the biofilm-forming Shigella strain failed to colonize in vivo, indicating that the fitness gain on host adhesion resulted from biofilm formation is not sufficient to offset the loss of fitness on survivability caused by LPS deletion.
Materials & Methods
Bacterial strains and plasmids
Bacterial strains and plasmids used in this study are listed in Table 1. Shigella strains were cultured aerobically at 37°C in Tryptic Soy (TS) broth (Aoboxing, Beijing, China) or on TS agar plates with 0.1% Congo Red. Antibiotics (Sigma) were used as follows: ampicillin 100 µg/ml; kanamycin 100 µg/ml.
|Strains||Relevant genetype, phenotype and description||Reference|
|Sf301||Shigella flexneri 2a strain||(Jin et al., 2002)|
|301ΔicsA||Sf301 ΔicsA (+51 to +3255): KRC||This work|
|301Δwzy||Sf301 Δwzy (+26 to +1075): KRC||This work|
|301ΔwaaL||Sf301 ΔwaaL (+6 to +1155): KRC||This work|
|301ΔrfaC||Sf301 ΔrfaC (+33 to +832): KRC||This work|
|pKD4||Template plasmid for λ Red recombination system||(Datsenko & Wanner, 2000)|
|pKD46||λ Red recombinase expression plasmid||(Datsenko & Wanner, 2000)|
|pCP20||λ Red FLP-recombinase expression plasmid||(Datsenko & Wanner, 2000)|
Bacterial gene knockout was performed using the λ Red recombination system (Datsenko & Wanner, 2000). Briefly, bacterial cells transformed with pKD46 were grown in the presence of L-arabinose to induce the expression of the lambda Red recombinase. A linear PCR product, amplified using the primers listed in Table 2, containing a kanamycin-resistance cassette (KRC) flanked by FLP and 50 bp of the 5′- and 3′-end homologous sequences of the target gene was electroporated into the bacterial cells and kanamycin was used to select the transformants. The plasmid pKD46 was eliminated by incubation at 37°C. To cure the kanamycin maker, pCP20 was introduced into kanamycin-resistant cells to elicit the recombination of flanking FLP sequences at both ends of the kanamycin cassettes. PCR screening for cured colonies were performed using specific primers listed in Table 2.
|icsARedF||ATGAATCAAATTCACAAATTTTTTTGTAATATGACCCAAT GTTCACAGGGGTGTAGGCTGGAGCTGCTTC||KRC targeting icsA|
|icsARedR||AAGGTATATTTCACACCCAAAATACCTTGGGTGTCTCTGT AACTGTTATTATGGGAATTAGCCATGGTCC||KRC targeting icsA|
|wzyRedF||ATAACTTCCCTATTTTTAACATCCTTTATTTTGCTCCAGAA GTGAGGTTAGTGTAGGCTGGAGCTGCTTC||KRC targeting wzy|
|wzyRedR||ATAACATTTTTATGTATTGAACTGATTATTGGTGGTGGTGG AAGATTACTATGGGAATTAGCCATGGTCC||KRC targeting wzy|
|waaLRedF||CTCAACATTATTTTTCTCTCTCGAGAAAAAAAACTGGATAGC GTACTGGAGTGTAGGCTGGAGCTGCTTC||KRC targeting waaL|
|waaLRedR||TTGTTTTTCATCGCTAATAATAAGCCGGCGTAAACGCCTAAT AAATTTGGATGGGAATTAGCCATGGTCC||KRC targeting waaL|
|rfaCRedF||CACTGATGCCCAGCAGGCAATCCCAGGGATTAAGTTTGACTG GGTGGTGGGTGTAGGCTGGAGCTGCTTC||KRC targeting rfaC|
|rfaCRedR||AAGAGACATACTTGTAGAACGACACTCTACTTGATTCTTCCCA TACCCACATGGGAATTAGCCATGGTCC||KRC targeting rfaC|
LPS preparation and electrophoresis
LPS was prepared from Shigella strains as described by Hitchcock & Brown (1983). Bacteria grown overnight on TSA were resuspended in PBS to an OD600 of 0.8. The bacterial pellet from 1.5 ml of the suspension was then resuspended in 125 ml lysis buffer (0.1 M Tris/HCl pH 6.8, 2% SDS, 4% β-mercaptoethanol and 10%, v/v, glycerol) and boiled for 10 min. Proteinase K (50 mg, Sigma) was added and the mixture incubated for 1 h at 60°C. Samples were run on a Tris-Tricine gel) and visualized by silver staining (Hitchcock & Brown, 1983).
Overnight-cultured bacteria were harvested by centrifugation (10,000× g for 2 min) and two ml of whole cells standardized at OD600 = 1 after suspension in PBS were placed in a 14-ml polyethylene tube and incubated at 4°C under a static condition. The OD600 of the phase above the sediment by aggregation was recorded at different time points.
Biofilm formation assays
Biofilm formation by Shigella strains was assayed as previously described with some modifications. For biofilm analysis on polystyrene surface, 107 CFU of Shigella in 100 µl of TSB broth was inoculated into the wells of a 96-well flat-bottom polystyrene microtiter plate. The bacterial strains were grown at 37°C for 48 h under a static condition and the planktonic cells in liquid medium were discarded. The plate or tube was washed twice with distilled water and air-dried. Attached biofilms were stained with 0.1% crystal violet for 20 min. Then, the plates were rinsed twice with distilled water to remove excess stain and air-dried. In order to quantify the amount of biofilm on a 96-well plate, all stain associated with the attached biofilms was dissolved with 95% ethanol, then OD595 absorbance was measured using a microplate reader.
To prepare the biofilm sample for Confocal laser scanning microscopy (CLSM) analysis, GFP-expressing plasmid was electroporated into Shigella strains. 108 CFU of GFP-Shigella was added in 1 ml of TSB broth per well and incubated at 37°C sunder a static condition. Biofilms were grown on cover glass (φ = 14 mm) placed in 24-well polystyrene cell culture plates. After 48 h, the cover glass was rinsed twice with PBS to remove any planktonic cells. After washing, the cells were fixed in 3% paraformaldehyde/PBS and mounted with Anti-Fade solution (Invitrogen) containing DAPI onto glass slides. After the preparation, the samples were examined under the confocal laser scanning microscope ZEISS LSM 710 (Carl-Zeiss), and images were processed by LSM software ZEN (Carl-Zeiss, Oberkochen, Germany).
To prepare the biofilm sample for scanning electron microscopy (SEM), the biofilms grown in the cover glass dehydrated in graded ethanol, critical point dried with CO2 and coated with gold-palladium beads with a diameter of 15 nm. Samples were photographed using a Philips XL-30 scanning electron microscope at 20 kV.
In vitro adhesion and invasion assays and microscopy
One day before the assays, HeLa cells (ATCC CCL-2) were seeded into 24-well plates at a density of ∼105 cells per well. One hour before the infection, cell culture medium were changed into serum-free medium and ∼106 CFU Sf301 or its LPS mutants from mid-exponential phase was added to the cells together. Bacteria were centrifuged (2,000 rpm, 10 min, RT) onto HeLa cells (moi 10:1, or indicated moi) to synchronize the infection. For adhesion assay, after washing, the cells were lysed with distilled water and the CFU was enumerated after plating. For invasion and proliferation assays, bacteria/HeLa mixtures were incubated for 40 min after centrifugation and then washed, treated with gentamycin-containing (25 µg/ml) medium for another 1 h (invasion) or 4 h (proliferation) before lysed for plating. Adhesion was defined as the total number of HeLa cell-associated bacteria and is shown as the percentage of input. Invasion and proliferation was defined as the total number of intracellular bacteria in cells (extracellular bacteria was killed by gentamycin, a cell-impermeable antibiotic). Average results of three independent experiments are shown as mean ± SD.
For fluorescent microscopy of bacterial adhesion to HeLa cells, cells were plated onto glass coverslips and adhesion assays were performed as described using Sf301 harboring the GFPUV-expressing plasmid (moi 100:1). Cells were fixed in 3% paraformaldehyde/PBS at room temperature for 15 min, washed in PBS and mounted with Anti-Fade solution (Invitrogen) containing DAPI onto glass slides and visualized under Zeiss confocal microscope. For scanning electron microscopy (SEM), the cover glass was dehydrated in graded ethanol, critical point dried with CO2 and coated with gold-palladium beads with a diameter of 15 nm. Samples were photographed using a Philips XL-30 scanning electron microscope at 20 kV.
Lactate dehydrogenase (LDH) activity assay
The LDH assay was performed using the LDH cytotoxicity assay detection kit (Beyotime, China), according to the manufacturer’s instructions. The assay measures the conversion of a tetrazolium salt to a red formazan product, detectable by absorbance measurement at 490 nm. For this, a SpectraMax 190 Microplate Reader (Molecular Devices) was used.
Phalloidin staining assay
For phalloidin staining of F-actin in Shigella-infected HeLa cells, cells were plated onto glass coverslips and invasion assay was performed as described using Sf301 harboring the GFPUV-expressing plasmid (moi 100:1) for two hours. Cells were fixed in 3% paraformaldehyde/PBS at room temperature for 15 min, washed in PBS and permeabilized in 0.1% Triton-X100 in PBS for 1 min. F-actin were stained with 80nM TRITC-phalloidin (Yeasen, Shanghai, China) for 30 min. The coverslips was mounted with Anti-Fade solution (Invitrogen) containing DAPI onto glass slides and visualized under Zeiss confocal microscope.
This was carried out according to Oaks, Wingfield & Formal (1985) using confluent HeLa cell monolayers. Briefly, HeLa cells to be used in the plaque assay were grown to 100% confluency in 6-well polystyrene plates (Corning) in DMEM supplemented with 10% FBS. One hour before the infection, cell culture medium were changed into fresh medium and Sf301 or its LPS mutants from mid-exponential phase (m.o.i 100:1) was added to the cells and subsequently incubated at 37°C for 90 min. During this adsorption or attachment phase, the plates were rocked every 30 min to assure uniform distribution of the plaque-forming bacteria. Next, an agarose overlay (5 ml) consisting of DMEM, 5%FBS, 25 µg of gentamicin per ml, and 0.5% agarose was added to each plate. The plates were incubated at 37°C in a humidified 5% CO2 and examined daily for up to 3 days for plaque formation. The agar was carefully removed three days later and the HeLa monolayers were stained by Giemsa staining kit (Yeasen, Shanghai, China) in order to visualize the plaques.
Female Hartley guinea pigs, aged 6–8 weeks, weighing 200–300 g, were inoculated with 107 CFU/eye of mid-log phase Sf301 and its LPS mutants via conjunctival route as described, with 3 animals in each group. The protocol has been approved by the Animal Research Ethical Committee of School of Life Science and Technology the Xi’an Jiaotong University (Approval No. 201411). Inoculated animals were observed and scored for 7 consecutive days for development of the conjunctivitis. Eyes were blindly scored by three individuals (DX, YPS, YC) on a scale of 0–3 defined as follows: grade 0 (no disease or mild irritation), grade 1 (mild conjunctivitis or late development and/or rapid clearing of symptoms), grade 2 (keratoconjunctivitis without purulence), grade 3 (fully developed keratoconjunctivitis with purulence).
Guinea pigs were anesthetized using chloral hydrate (10 mg/kg of body weight) before being inoculated via an intrarectal (i.r.) route with 108 CFU of Sf301 and its LPS mutants in 100 µl PBS, with 3 animals in each group. The protocol has been approved by the Animal Research Ethical Committee of the Xi’an Jiaotong University. Three pieces of feces of each inoculated animal were collected at the same time of the day for 18 days. Each piece of the feces were dispersed and 1 ml PBS. After centrifuge, 100 µl of the supernatant was plated onto MaConkey plates. Shigella bacteria were recognized as smooth, white colonies on MaConkey plates and further confirmed by PCR of spa33 gene.
All data are presented as means ± SEMs. Statistical analysis was performed within the subgroups by using Student’s t-test for autoaggregation assays, biofilm formation assays, in vitro adhesion/invasion assays and LDH assays in this study. p values of less than 0.05 were regarded as statistically significant. Statistical analysis was performed with GraphPad Instat 3 software (GraphPad Software, Inc, La Jolla, Calif).
Generation and characterization of the LPS mutants of Shigella flexneri
To generate Shigella LPS mutants of different chain length, we knocked out wzy, waaL and rfaC individually using the lambda red system (Fig. S1). As shown in Fig. 1A, the wzy mutant contains a complete core and one copy of the O-antigen; the waaL mutant has a complete core but no O-antigen; the rfaC mutant is deficient of Hep but retains the Kdo. SDS-PAGE analysis confirmed that the all mutant strains produced proper LPS variants as expected (Fig. 1A). The Δwzy and ΔwaaL strains formed WT-like colonies on Tryptone Soya Agar, while the ΔrfaC strain grew round and smooth colonies with smaller size. In accordance with this, the ΔrfaC mutant grew slightly slower in liquid tryptone soya broth medium than other strains (Fig. 1B). LPS truncation had no apparent impact on the morphology of individual bacteria cells as illustrated by transmission electron microscopy (TEM) (Fig. 1C).
Biofilm formation is enhanced in the rfaC-deleted Shigella strain
The aggregation tendency of LPS mutants was initially evaluated in PBS and the results showed that LPS truncation led to enhanced bacterial aggregation (Fig. 2A). Next, we examined the biofilm formation of the LPS mutants on the polystyrene surface under a static culture condition. While the WT strain had a poor ability to form biofilm, the LPS mutants showed improved potential to do so (Fig. 2B). Moreover, the ability to form biofilm appeared to be negatively correlated with the LPS length with the ΔrfaC strain (shortest LPS) being the most effective one (Fig. 2B). Fluorescence microscopy and scanning electron microscopy (SEM) further confirmed the enhanced biofilm formation by the ΔrfaC strain on glass surface (Figs. 2C–2D). To test the involvement of extracellular DNA in the biofilm formation by the ΔrfaC strain, DNase I was added when the bacteria were seeded into the polystyrene plates. Disruption of extracellular DNA significantly abolished the formation of biofilm without affecting the viability of the bacteria (Fig. 2E and Fig. S2). In addition, SEM analysis demonstrated that there were fibrous connections among bacterial cells in the biofilm (Fig. 2F).
In vitro adhesiveness and thus invasiveness is promoted in biofilm-forming rfaC-deleted Shigella flexneri strain independent of activation of type III secretion system
Since biofilm formation is often associated with bacterial virulence, we set out to evaluate the pathogenic activities of the biofilm-forming LPS mutants using the gentamicin protection assay. The Δwzy and ΔwaaL strains showed almost identical host invasion efficiency to the WT strain. By contrast, the ΔrfaC strain showed a much stronger invasiveness and intracellular proliferation than wild type (Fig. 3A). Further dissection of time-dependent infection process revealed that the improved invasiveness came from enhanced adhesion during the initial host cell-Shigella contact (within 10 min), which was further confirmed by fluorescence microscopy and scanning electron microscopy (Figs. 3B–3D). To be specific, ΔrfaC mutant exhibited pronounced adhesiveness even when the type III secretion system (T3SS), responsible for bacterial invasion and virulence, was inactivated transcriptionally at low growth temperature (28–30°C). Of note, the invasion of low temperature-cultured bacteria was totally abolished as expected since no intracellular bacteria were recovered. To verify the cell-lysing ability of ΔrfaC mutant, we assayed the level of LDH in the cell culture medium 90 min post-infection. LDH is a stable cytoplasmic enzyme that is only released on loss of membrane integrity. The LDH level in the supernatant of ΔrfaC-infected HeLa cells was more than twice that of the M90TS-infected cell supernatant (Fig. 3E).
rfaC-deleted strain showed different actin-based motility from other LPS-truncated strains
To examine the distribution of IcsA in the LPS-truncated mutants, intracellular F-actin of the infected host cells were visualized by fluorescent phalloidin, which binds to F-actin of mammalian cells. Although F-actins could be recruited by all the Shigella strains except the icsA-deleted strain (Fig. 4A and Fig. S3), their cellular distribution varies between WT and LPS mutants. Typical “actin comets” and long protrusion were observed with the wild type strain (Fig. 4A), indicating a normal polar distribution of IcsA, which was further confirmed by the competence to form regular plaques on HeLa cell monolayer in a plaque assay (Fig. 4B). By contrast, the Δwzy and ΔwaaL mutants assembled F-actins all around the bacteria cell (Fig. S3), implying a circumferential distribution of IcsA, which caused aberrant actin-based motility (ABM) and thus failure to form plaques on HeLa cells monolayer (Fig. 4B). The ΔrfaC bacteria also recruited F-actin in a circumferential pattern as other LPS-truncated strains do. Nevertheless, a small amount of bacteria could assemble short and curly “actin-tail” behind the bacteria (as arrows indicated in Fig. 4A). Although ΔrfaC mutant could not form classical plaques on HeLa cell monolayer in 3 days, the integrity of the monolayer were destroyed due to massive cell detachment (Fig. 4B).
Truncation of LPS rendered bacteria susceptible in vitro and in vivo
LPS, especially long-chain LPS of gram-negative bacteria, provides protection for the bacteria against unfavorable environment. While loss of LPS may contribute to biofilm formation and pathogenic activities such as adhesion and invasion, the adverse effects associated with LPS deletion must also be taken into consideration to accurately gauge the overall influences on bacterial fitness. To do this, we measured the susceptibility of the LPS mutants to distilled water (to mimic the low osmotic shock in environment) and 10% pooled human serum (to mimic the adverse environment in vivo). While WT bacteria well survived the low osmotic shock (water) during the experiment, all three LPS mutants showed severely compromised viabilities after two hours in water. The ΔrfaC mutant in particular, even begun to exhibit significantly reduced viability within 30 min (Fig. 5A). Human serum showed much stronger killing activity than water toward Δwzy, ΔwaaL and ΔrfaC strains (Table 3). It is interesting to note that although most of the bacteria were killed by the serum, a small number of colonies were recovered for the ΔrfaC strain versus no colony for Δwzy and ΔwaaL strains (Fig. 5B). Whether this improved survivability of the ΔrfaC strain against serum is related to its biofilm-forming ability warrants further investigation.
|Treatment||Heated inactivated serum (%)||Pooled human serum (%)|
|WT||90.6 ± 13.5||63.4 ± 6.4|
|Δwzy||85.5 ± 7.6||0|
|ΔwaaL||111.1 ± 11.4||0|
|ΔrfaC||89.9 ± 10.5||0.0023 ± 0.0004|
Given the dramatic virulence-boosting phenotype of the ΔrfaC mutant in vitro, we next examined the in vivo effects of LPS mutants on virulence using two independent animal models. The Sereny test (guinea pig keratoconjunctivitis) indicated that Δwzy, ΔwaaL and Δrfac strains failed to cause any manifestation of conjunctivitis during a period of 2 weeks’ infection. Wild type, on the other hand, provoked a typical keratoconjunctivitis 72 h post-infection (Table 4). To test the colonizing ability of the “super-adhesive” ΔrfaC mutant in the intestine, guniea pigs were inoculated with 108 CFU of Shigella via intrarectal route. Feces analysis revealed that Δwzy, ΔwaaL and ΔrfaC failed to colonize the intestines of guinea pigs, and bacteria were evacuated in three days without any exhibited symptoms. Nevertheless, animals inoculated with wild type stably excreted bacteria in 18 tested days, albeit without observed symptoms either (Fig. 5B).
In the present study, we described a new and unusual phenotype of Shigella flexneri that is characteristic of enhanced biofilm formation. Deficiency in Hep synthesis in LPS due to deletion of rfaC gene resulted in “deep-rough” LPS with an incomplete inner core containing only the Kdo moieties. Although various LPS truncations have been studied for their effects on the biological activities of Shigella, the deep-rough mutant has never been tested. In this work, we found that the deep-rough Shigella (ΔrfaC) exhibited significantly enhanced biofilm-forming ability and strong adhesiveness toward host cells, which is in sharp contrast to the WT strain (Brotcke Zumsteg et al., 2014; Kline et al., 2009; Mahmoud et al., 2016; Schroeder & Hilbi, 2008). Besides, this deep-rough mutant could efficiently proliferate in the host cells and cause extensive cell lysis in few hours after infection. However, the pronounced in vitro virulence observed with this mutant was not recapitulated in vivo, most likely due to its increased vulnerability to environmental stress caused by LPS loss.
The biofilm of ΔrfaC Shigella showed a typical mesh-like structure and its formation is dependent on extracellular DNA as proven by DNase I treatment experiment. Previous studies have shown that LPS truncations in E. coli and Porphyromonas gingivalis also promoted biofilm formation (Nakao et al., 2012; Nakao, Senpuku & Watanabe, 2006), suggesting that the correlation between LPS loss and biofilm-forming capacity might be a common feature in gram-negative bacteria. Bacterial surface hydrophobicity is a major determinant for biofilm formation (Donlan, 2002; Mitzel et al., 2016). LPS truncation reduced the hydrophilic sugar moieties from bacteria surface and increased the exposure of the hydrophopic outer membrane lipid layer, thus enhancing the hydrophobicity on bacteria surface and facilitating biofilm formation.
WT Shigella flexneri adheres to host cells much less efficiently in vitro than other enterobacteria due to the lack of general adhesion apparatus like fimbriae (Edwards & Puente, 1998; Pizarro-Cerdá & Cossart, 2006; Snellings, Tall & Venkatesan, 1997). To our surprise, the ΔrfaC mutant exhibited extraordinary adhesion to host cells and manifested normal invasion and proliferation capabilities as well. The molecular mechanism of the hyperadhesiveness of ΔrfaC mutant remains unclear. Interestingly, we noticed that the ΔrfaC Shigella tended to form clusters on abiotic surface or host cells. Whether this cell–cell clustering is also a result of the improved hydrophobicity caused by complete LPS shedding requires further investigation. Nevertheless, it is conceivable that the clustered Shigella may adhere to host cells as one entity, in which numerous weak contacts contributed by each individual bacterium are pooled to improve the overall avidity of the bacterial cluster toward the host cell.
Previous studies have shown that the long-chain LPS was essential for maintaining polar distribution of IcsA (Doyle et al., 2015; Morona, Daniels & Den Bosch, 2003; Sandlin et al., 1995). Indeed, the Δwzy and ΔwaaL mutants with shortened LPS displayed circumferential distribution of IcsA. Interestingly, a small amount of ΔrfaC bacteria could assemble atypical, short and curly actin-tail, implying the heterogeneous distribution of IcsA in this new mutant. Results from plaque assay showed that ΔrfaC bacteria failed to form typical plaque on HeLa monolayer as the WT does, although it did caused mass host cell death eventually. This could be caused by a limited number of correctly assembled ABM in function or by premature killing of the host cell before the actin protrusions could reach adjacent cells due to much enhanced intracellular proliferation. How the ΔrfaC mutant retains certain level of functional IcsA warrants further investigation.
Although the ΔrfaC mutant showed a significantly boosted virulence in vitro, it failed to colonize in vivo. Susceptibility test against low osmotic shock or serum revealed that this mutant is highly sensitive to environmental stress. Clearly, the virulence benefit gained from biofilm formation and/or improved adhesion is not enough to compensate for the loss of fitness on survivability in vivo.
In conclusion, this study characterized a new Shigella flexneri mutant with deficiency in Hep synthesis of LPS. This mutant was capable of forming biofilm on abiotic surface and manifested extraordinary adhesiveness to host cells. Our study established a clear positive relationship between increased surface hydrophobicity and adhesiveness of Shigella flexneri. Although it is not realistic for a pathogenic bacteria to shed off LPS to gain hydrophobicity in vivo, our study raised a possibility that the host adhesiveness of Shigella may be modulated by altering the hydrophobicity of the bacteria.
PCR analysis of constructed S.flexneri LPS mutants in this study by agarose electrophoresis
PCR was performed using the primers listed in Table 2. DNA ladders were shown in Lane M. (A) Δwzy mutant strain. Lane 1, wild type (1238 bp); Lane 2, Δwzy: kana (1600 bp); Lane 3, 4, Δwzy (100 bp); (A) ΔwaaL mutant strain. Lane 1, wild type (1238 bp); Lane 2, ΔwaaL: kana (1600 bp); Lane 3, 4, ΔwaaL (100 bp); (A) ΔrfaC mutant strain. Lane 1, wild type (1238 bp); Lane 2, ΔrfaC: kana (1600 bp); Lane 3, 4, ΔrfaC (100 bp).
Influence of 48-hour DNaseI treatmenton viability of ΔrfaC strains
Fluorescencemicroscopy analysis of F-actin in HeLa infected by Sf301 and its ΔicsA, Δwzy and ΔwaaL mutant strains
Invasion assay was performed as previously described. F-actin is stained by TRITC-phalloidin (red), Shigella bacteria are green and nuclei are blue (DAPI).