Original Research ARTICLE
Pch Genes Control Biofilm and Cell Adhesion in a Clinical Serotype O157:H7 Isolate
- Molecular Characterization of Foodborne Pathogens Research Unit, Eastern Regional Research Center, Agricultural Research Service, United States Department of Agriculture, Wyndmoor, PA, United States
In a previous study, induction of the Escherichia coli serotype O157:H7 SOS response decreased csgD expression in the clinical isolate PA20 at 30∘C but strongly induced genes in the horizontally transferred-DNA regions (HTR), including many known virulence regulators. To determine the role of HTR regulators in the control of csgD and curli, specific regulators were plasmid-expressed in the wild-type and mutant strains of PA20 and its biofilm-forming derivative, 20R2R. At 30∘C, plasmid over-expression of the O157:H7 group 3 perC homolog, pchE, strongly repressed PA20 csgD transcription (>7-fold) while the group 1 homologs, pchA and pchB, resulted in smaller reductions (<2.5-fold). However, SOS induction decreased rather than increased pchE expression (>6-fold) making group 1 pch, which are enhanced by the SOS response, the likely SOS-induced csgD repressors. Plasmid-based pchE over-expression also reduced 20R2R biofilm formation (>6-fold) and the curli-dependent, Congo red affinity of both PA20 and 20R2R. However, to properly appreciate the regulatory direction, expression patterns, and environmental consequences of these and other CsgD-controlled functions, a better understanding of natural pchE regulation will be required. The effects of HTR regulators on PA20 and 20R2R adhesion to HEp-2 cell at host temperature were also studied. Under conditions where prophage genes were not induced, curli, rather than espA, contributed to host cell adhesion in strain 20R2R. High levels of pchE expression in trans reduced curli-dependent cell adherence (>2-fold) to both 20R2R and the clinical isolate PA20, providing a host-adapting adhesion control mechanism. Expression of pchE was also repressed by induction of the SOS response at 37∘C, providing a mechanism by which curli expression might complement EspA-dependent intimate adhesion initiated by the group1 pch homologs. This study has increased our understanding of the O157 pch genes at both host and environment temperatures, identifying pchE as a strong regulator of csgD and CsgD-dependent properties.
Infection with Shiga toxin-producing Escherichia coli (STEC) cause sporadic cases or large outbreaks of hemorrhagic colitis that can progress to the severe renal-associated syndrome, hemolytic uremic syndrome (HUS) (Tarr et al., 2005). Although Shiga toxin(s) are the most important virulence determinants, the prophage-encoded locus of enterocyte effacement (LEE) also contributes to STEC virulence (Frankel et al., 1998). In the United States, serotype O157:H7 is responsible for the highest numbers of reported STEC cases, hospitalizations, and morbidities (Scallan et al., 2011). Ruminants are the predominant STEC reservoir and fecal contamination that leads to contaminated carcasses and agricultural environments is a primary source for transmission to humans (Lim et al., 2010). A critical step in the transmission process is the transition from the reservoir GI tract to the environment where the bacterium must survive until returning to GI conditions of the host or a different reservoir. While outside of the reservoir host, formation of biofilms increases stress resistance, prolongs pathogen survival time, and increases the opportunity for reservoir to host transmission (Kumar and Anand, 1998).
In E. coli biofilm production, initial attachment of motile bacteria to surfaces is followed by the formation of irreversible attachments to the surface and surrounding bacteria (Kostakioti et al., 2013). This stage is dependent on amyloid-containing curli fimbriae, and the exopolysaccharide, cellulose (Zogaj et al., 2001). Curli are assembled from the CsgA subunit and CsgB nucleator proteins encoded in the csgBAC operon. The CsgD transcription factor controls curli formation and is encoded along with export proteins in the csgDEFG operon (Hammar et al., 1995; Robinson et al., 2006). Expression of csgD at environmental temperatures (≤30°C) utilizes the RpoS sigma factor and requires the transcription factor, mlrA (Brown et al., 2001). MlrA binds to sites upstream of the −35 promoter region and positively regulates csgD transcription in E. coli strains that depend on RpoS for curli expression (Brown et al., 2001; Ogasawara et al., 2010a). How MlrA is activated is currently unknown. A complex network of regulatory proteins, small RNAs, and small signaling molecules controls the rpoS-dependent expression of csgD (Gerstel and Römling, 2003; Sommerfeldt et al., 2009; Ogasawara et al., 2010a,b; Jørgensen et al., 2012). Congo red (CR) dye stains amyloid and its inclusion in agar plates allows easy identification of curli production (Zogaj et al., 2001). There is marked strain and serovar variability in the expression of curli and cellulose, CR affinity, and the production of biofilm among STEC strains (Chen et al., 2013; Uhlich et al., 2013, 2014). However, CsgD appears to retain an essential role in STEC curli and biofilm formation.
The low incidence of biofilm production in O157:H7 strains isolated from the human host suggests that biofilm structural or regulatory components may have a negative effect on viability in the human host (Biscola et al., 2011). Attenuation of biofilm properties in clinical strains generally results from genome modifications that lower csgD expression causing reductions in curli production (Uhlich et al., 2013). In a study of 55 clinical O157:H7 strains, 53 carried a prophage inserted in mlrA and two strains carried rpoS mutations that reduced csgD expression and prevented biofilm formation. Although insufficient to support biofilm formation, many of the clinical strains produced sufficient curli to bind detectable CR dye at 37°C in a csgD-dependent manner suggesting that reduction rather than elimination of csgD expression was favored (Uhlich et al., 2014). A different study confirmed that strains carrying a prophage in mlrA still generate considerable levels of csgD expression, even when curli expression is below the threshold required to produce observable CR affinity (Uhlich et al., 2016). Whether this level of csgD expression is utilized for controlling processes other than curli expression that are important for host colonization and disease pathogenesis is currently unknown. When LEE-generated effacing lesions are initiated, STEC require cell attachment mediated by the EspA protein, which is encoded along with other effector proteins in the LEE operon (Ebel et al., 1998; Nataro and Kaper, 1998). Transcription of espA depends on LEE activator, Ler, and production of EspA filaments requires a post-transcriptional mechanism allowing translation of espABD transcripts (Roe et al., 2003). The requirement for EspA in adhesion of O157:H7 to cultured cells has been clearly demonstrated but the effect of curli on cell adhesion is still unclear and likely varies with STEC serotype, strain genetic background, and growth conditions (Richter et al., 2014; Sharma et al., 2016; Kudva et al., 2017).
Exposure of clinical O157:H7 strains to DNA-damaging antibiotics, such as sulfamethoxazole-trimethoprim (SMX-TM), can potentiate HUS by increasing the expression of virulence genes encoded in prophage and prophage-like elements (e. g. stx2 and LEE) (Herold et al., 2005; Landstorfer et al., 2014; Uhlich et al., 2018). SMX-TM can also induce prophage excision from mlrA, making restoration of CsgD function a possible additional consequence of antibiotic treatment in the host (Shaikh and Tarr, 2003; Uhlich et al., 2016). However, in an RNA-seq study testing SMX-TM effects on a clinical O157:H7 transcriptome, SMX-TM had a slight repressive, rather than enhancing, effect on csgD functions in spite of strong induction of prophage and prophage-like genes (Uhlich et al., 2018). The mechanism controlling the unexpected repressive csgD effects following SMX-TM exposure were not apparent but we reasoned that transcription factors differentially expressed during SMX-TM exposure might antagonize csgD. Regulators in the horizontally transferred-regions (HTR) associated with control of LEE, including grlA, ler, and the pch genes, were among the transcription factors most strongly affected by SMX-TM exposure. In STEC, five different pch genes (perC homologs) are encoded within various prophage (Sp) or prophage-like regions (SpLE) (Porter et al., 2005). The pch genes can be assigned into three groups based on DNA similarity, size, and functionality: group1 (pchA, pchB, pchC), group 2 (pchD), and group 3 (pchE). The group 1 pch, but not groups 2 and 3, were found to be essential for the full expression of ler, espA, and attachment of O157:H7 to cultured HEp-2 cells (Iyoda and Watanabe, 2004).
In this study we tested several transcription factors encoded in HTR that were induced during SMX-TM treatment of O157:H7 clinical isolate PA20 (Uhlich et al., 2018) for an effect on csgD, csgD-dependent cell adhesion, and biofilm properties.
Materials and Methods
Strains, Growth Conditions, and Molecular Biology Techniques
All strains used in the study are listed in Supplementary Table S1. E. coli serotype O157:H7 PA20 is a clinical isolate that produces Stx1 and Stx2, and carries a prophage insertion in mlrA (Uhlich et al., 2013). Strain 20R2R was created by the spontaneous loss of the PA20 Stx1 prophage that restored mlrA function and RpoS-dependent csgD expression (Uhlich et al., 2016). NEB 5-alpha (New England Biolabs Inc.) and One Shot PIR1 (Invitrogen) were used as E. coli host strains for intermediary cloning steps. Strains were cultured in lysogeny broth (LB) prepared using the Miller formulation or LB without added NaCl (LB-NS).
Chromosomal DNA was isolated using the DNeasy Blood and Tissue Kit (Qiagen) or Qiagen Genomic-tip 100/G (Qiagen). The Qiagen multiplex PCR kit was used for routine PCR amplifications (Qiagen). Primers utilized in this research are listed in Supplementary Table S2.
Mutant Strain Construction
Deletions of the ler, glrA, pchA, pchB, pchC, pchD, pchE genes in the indicated strains were made as previously described replacing major portions of the coding regions with neomycin or chloramphenicol cassettes (Uhlich et al., 2009; primers shown in Supplementary Table S2). The cassettes were removed in strains bearing ler, pchC, and pchE deletions to avoid polar effects on downstream genes, except for the neomycin cassette in strain PA20Δler (GeneBridges GmbH). All deletions were verified by PCR using primers (not listed) designed from areas flanking the homologous recombination regions.
The open-reading-frames, along with sufficient immediate 5′ sequence to include the native ribosomal binding sites of glrA, pchA, pchB, pchC, pchD, and pchE were cloned into plasmid pSE380 (primers in Supplementary Table S2). During testing, strong IPTG induction of certain regulators inhibited host strain growth. Therefore, only un-induced results are shown, taking advantage of the leaky nature of the pSE380 trc promoter to generate cloned insert expression sufficient to observe phenotypic differences.
CR Dye Affinity and Biofilm Assays
Curli expression was tested by monitoring strain CR affinity. Three microliters of LB overnight cultures were spotted on T-medium agar containing 20 mg/l CR dye and 10 mg/l Coomassie brilliant blue G (TA) as described (Collinson et al., 1991; Chen et al., 2013). Plates were incubated for the designated times, imaged using Epson Perfection 3200 Photo Scanner/Epson Scan software (Professional mode) with a light blue background at 600 dots per inch, and compared visually for differences in red color intensity. Biofilm formation was assayed in 96-well format stained with crystal violet (CV) dye, slightly modifying the method described by Chen et al. (2013): plates were covered with sterile adhesive porous rayon films (VWR, Avantor) instead of plastic lids to allow equal gas exchange. Plates were incubated at 30°C for 48 h in humidity chambers and biofilms were heat-fixed at 60°C for 30 min after removing non-adhered bacteria by washing with water.
RNA Isolation, cDNA Preparation, and qRT-PCR
In order to study the effect of over-expression of HTR regulators on genes involved in curli and biofilm formation (csgD, csgA), a relative quantification of gene expression was carried out on PA20 and 20R2R strains transformed with pSE380 plasmids carrying different HTR regulatory genes. One milliliter of LB overnight culture of each strain was centrifuged at 7,000 × g for 5 min, re-suspended in 100 μl LB, spin-plated on 30°C-pre-warmed T-medium agar containing ampicillin (100 μg/ml), and incubated for 8 h at 37°C or 12 h at 30°C. Every strain was plated in triplicate. Bacteria were harvested with a sterile cotton swab (Puritan Medical Products Company, LLC) and suspended in RNAzol RT (Molecular Research Center). Extraction of total RNA was performed following the manufacturer’s instruction (including phase separation with 4-bromoanisole) and re-suspended in 40 μl nuclease-free water. TURBO DNA-free kit (Ambion) was used to eliminate contaminating DNA from isolated RNA samples. The High Capacity cDNA Reverse Transcriptase Kit (Thermo Fisher Scientific) was used to make cDNA from 1 μg total RNA.
In order to compare pchE expression in PA20 grown on agar surfaces at 30°C and 37°C, with and without exposure to 27× SMX-TM, total RNA was isolated and cDNA was made as previously reported (Uhlich et al., 2018). Samples were tested in triplicate.
qRT-PCR was performed by adding 1 μl (20 ng) of cDNA or DNase-treated RNA (negative control) to 19 μl reaction mixture consisting of 0.5 μM of each primer (Integrated DNA Technologies) and 10 μl Fast SYBR Green Master Mix (Applied Biosystems). Primers are listed in Supplementary Table S2. Amplification was carried out on a 7500 Fast Real Time PCR System (Applied Biosystems) using the following parameters: denaturation at 95°C for 20 s followed by 40 cycles (3 s at 95°C, 30 s at 60°C). Melt curve analysis was used to verify the specificity of the amplification products. The gyrA gene was used as a reference to normalize the results and PA20+pSE380 or 20R2R+pSE380 were used as calibrator strains. qRT-PCR data were analyzed using the fold change (FC) = 2−ΔΔCT method (Livak and Schmittgen, 2001). The mean FC for three trials of qRT-PCR for the selected genes along with standard deviations (SD) were reported.
Bacterial Adhesion/Invasion Assay on HEp-2 Cells
The influence of the HTR regulators on bacterial attachment to eukaryotic cells was tested using a HEp-2 cell line (ATCC CCL-23) grown in EMEM, supplemented with 10% fetal bovine serum (all from ATCC), at 37°C in a humidified 5% CO2 atmosphere. For adhesion assays, 500 μl of 1 × 105 cells/ml were seeded in a tissue culture treated polystyrene 24-well plates (Sigma-Aldrich) and cultivated until an 85–95% confluent monolayer was formed.
Bacterial strains were grown standing in LB broth with or without ampicillin (100 μg/ml) overnight at 37°C or on T-medium agar with or without ampicillin (100 μg/ml) for 2 days at 30°C. Bacteria were centrifuged and re-suspended (broth cultures) or directly harvested (agar plates) in phosphate buffer saline (PBS). Dilutions in EMEM, with or without ampicillin (100 μg/ml), corresponding to an optical density (OD600) of ∼0.07 were prepared for eukaryotic cell exposure. The EMEM covering HEp-2 monolayers was replaced with 1 ml/well of EMEM bacterial suspension and the cells were incubated at 37°C with 5% CO2 for 3 h. Afterward, cells were washed five times with PBS to remove unbound bacteria and infected monolayers were treated with 1 ml of 0.1% Triton X-100 for 30 min.
The numbers of cell-associated bacteria was detected by plate count assay. Serial 10-fold dilutions of lysed cells were prepared in PBS and five 10 μl drops of each dilution were placed onto LB agar plates. CFU count was performed after incubation at 37°C for 24 h. The wash PBS was saved and used for CFU counts of unattached bacteria. The percentage of attached bacteria was calculated as follows: n. adhered bacteria × 100/n. adhered bacteria + n. unbound bacteria.
Curli Extraction, Gel Separation, and Measurement
Escherichia coli strains were grown on T-medium agar for 24 h at 37°C. Cells were collected from individual plates and analyzed for total soluble proteins as described previously (Uhlich et al., 2009) with modifications. It is necessary to treat polymerized curli with formic acid (pH 2.0) before gel separation (Collinson et al., 1991). Additionally, it is also our experience that the treated samples must be maintained on ice for all steps of the extraction and gel sample preparation process. Cells were collected from plates into sterile water and the optical densities for all strains were adjusted to 0.5 (600 nm). Additionally, aliquots were taken from each individual strain sample and plated onto LB agar to ensure that equal numbers of cells were present in each preparation (data not shown). One milliliter of cells were pelleted for each strain by centrifugation and resuspended in 100 μl of 98% formic acid and incubated for 30 min on ice. After incubation the formic acid solutions were evaporated under a stream of nitrogen while the tubes remained on ice. Dried samples were resuspended in 20 μl LDS buffer (Thermo Fisher Scientific), plus 8 μl 50 mM 1,4-dithiothreitol (DTT) solution and 52 μl water. Samples were incubated for 10 min on ice and 20 μl of each sample were loaded directly onto the gel without exposure to heat. Samples were separated on a 12% Nu-PAGE Bis-Tris gel (Thermo Fisher Scientific) as described previously (Laemmli, 1970) and then stained with Bio-Safe Coomassie stain (Bio-Rad Laboratories, Hercules, CA, United States). The gel was visualized using a Gel DocTM EZ Imager (Bio-Rad Laboratories) and the relative amounts of the gel bands, for each strain, containing the major curli subunit CsgA were determined using the densitometry function of the Image LabTM (version 6.0) program (Bio-Rad Laboratories).
Mass Spectroscopy and CsgA Major Peptide Quantification
The protein bands for each strain containing CsgA and previously measured by densitometry were excised from the gel with sterile scalpels. The gel bands were destained with a methanol solution and the proteins extracted from the gel using 50% acetonitrile, 5% trifluoroacetic acid (TFA) solution. The extracted proteins were digested overnight using Trypsin Gold (Promega, Madison, WI, United States) following the manufacturers’ protocol. Samples were treated with 2% TFA to stop trypsin digestion. Each of the resulting three digested gel extracts were analyzed in triplicate. This process used a Nano-Acquity UHPLC (Waters Co., Milford, MA, United States) running in the trap mode and equipped with a 20 mm × 180 μm, 5 μm Symetry C18 trap column (Waters) and a 200 mm × 75 μm, 1.8 μm HSS T3 (Waters) analytical column using a gradient of water:acetonitrile (0.1% formic acid) running with the composition from 95:5 to 50:50 with a duration of 30 min and a flow rate of 450 nl/min. The nano-UHPLC flow was directed to a Q-Exactive Plus orbitrap mass spectrometer (Thermo Fisher Scientific, Madison, WI, United States) using a nanospray Flex Ion source (Thermo Fisher Scientific). The mass spectrometer data was analyzed with Proteome Discover 2.2 (Thermo Fisher Scientific) using SEQUEST as the database search algorithm and the E. coli protein database from UniProt. In order to compare the concentration of the identified protein (CsgA, P28307) the triple charged most abundant peptide with the sequence NSDLTITQHGGGNGADVGQGSDDSSIDLTQR was selected for area integration on the total ion current (TIC) chromatogram. Sample variation was controlled for with protein P11457, expressed at similar levels in each of the three samples. Additionally, prior to HPLC separation and mass spectrometer injection samples were spiked with equal concentrations of rabbit glycogen phosphorylase protein (P00489) for normalizing one MS run to the next.
For biofilms, the mean optical density values of eluted CV at 590 nm (OD590) for each sample were analyzed as follows. For large screening assays testing the effects of multiple HTR regulators, samples were analyzed in R (R Core Team, 2017) as previously described (Uhlich et al., 2018). Strain variance was assessed with the Bartlett’s test and OD value differences were determined using the non-parametric Kruskal–Wallis test. Multiple pairwise t-test comparisons were performed to determine the dye retention differences between grouped strains. The t-tests were performed without the assumption of equal variance (pairwise.t.test option pool.SD = F) and the resulting P-values were adjusted with the Benjamini-Hochberg procedure. For comparison of HTR deletions in 20R2R and for the focused studies comparing over-expression of pchA and pchE, data were analyzed using an analysis of variance (ANOVA) for a randomized complete block design. The blocks were identified as the independent replicates. The appropriate term for testing for treatment effects and separating treatment means is the mean square for treatment by block, ignoring the within block well-to-well variation. Treatment means were separated using a Bonferroni least significant difference (LSD) method with P < 0.05.
For adhesion/invasion assays, strain samples were tested in triplicate to establish challenge-dose culturing parameters and in quadruplicate for the assays testing the effects of PchA and PchE. For the challenge-dose culturing parameters assay, data were analyzed in R (R Core Team, 2017) as described for the large screening biofilm assays testing the effects of multiple HTR. For the assays testing the effects of PchA and PchE, data were transformed by the square root transformation to correct for non-additivity. The transformed data were analyzed by anova using well-to-well variation as an error term to test for treatment effects and for treatment means separation. The Bonferroni LSD method was used to separate the treatment means (P < 0.05). The inferences based on the transformed values were then applied to the untransformed treatment means. As above, any two treatment means with no letter in common are significantly (P < 0.05) different by the Bonferroni LSD method.
Clinical isolate PA20 (stx1+, stx2+) carries a prophage insertion in mlrA that restricts csgD expression, eliminates biofilm formation, and reduces curli production and CR dye affinity (Uhlich et al., 2013). A spontaneous excision of the PA20 Stx1 prophage reformed the mlrA gene and created strain 20R2R (stx1−, stx2+), which has restored csgD expression, full CR affinity, and produces strong biofilms (Uhlich et al., 2016). Strain 20R2R is used in this study to show the effects of the tested regulators on an O157:H7 strain that maintains temperature-dependent (≤30°C) csgD regulation and strong curli expression driven from the typical mlrA/rpoS regulatory network; a strain type isolated more frequently from non-clinical isolates (Biscola et al., 2011; Uhlich et al., 2013).
Plasmid Induced pchE Represses Curli-Dependent CR Affinity in PA20 and 20R2R
In a previous study, certain SMX-TM concentrations decreased PA20 csgD expression at 30°C but strongly induced genes in HTR, including virulence regulators ler, grlA, and pch group 1 genes (Uhlich et al., 2018). To determine whether HTR-encoded LEE regulators control csgD, we expressed pSE380-cloned grlA, pchA, pchB, pchC, pchD, or pchE in wild-type and mutant strains of PA20 and 20R2R, and tested for differences in csgD-dependent phenotypes.
At 30°C, PA20 pSE380 showed a light red color on TA (Figure 1A). Deletion of csgBA (PA20ΔcsgBA pSE380) resulted in loss of all color but deletion of ler (PA20Δler pSE380) elicited little change in CR affinity. Expression of pchE eliminated all red color in PA20 and PA20Δler indicating a strong pchE repressive effect on curli that is independent of ler. Plasmid expression of pchA, pchB, and pchC caused a slight reduction in PA20 red color but pchD and grlA did not change the curli-dependent dye affinity. In PA20Δler, none of the cloned regulators, other than pchE, affected the dye affinity indicating that the pchA, pchB, and pchC reductions were ler-dependent. At 37°C, a non-permissive temperature for rpoS-dependent curli expression, dye affinity was minimal in PA20 pSE380 and the mutants, whether carrying cloned regulators or the control plasmid. Only pchC expression produced a small color increase in PA20Δler that was more brown than red.
FIGURE 1. Comparison of the effects of over-expression (A) or deletion (B) of different horizontally transferred-regions (HTR) on the Congo red dye affinity of strains PA20 and 20R2R. (A) Wild-type, Δler, and ΔcsgBA strains of PA20 and 20R2R, transformed with control plasmid pSE380 or pSE380 carrying cloned HTR regulator genes, spotted on TA and incubated at 30 or 37°C for 24 h. (B) PA20, 20R2R, and strains of each with deletion of ler, grlA, pchC, and pchE genes spotted on TA and incubated at 30 and 37°C for 24 h.
The curli-producing strain, 20R2R, and its mutant derivative, 20R2RΔler, displayed strong red colony staining when carrying pSE380 at both 30 and 37°C (Figure 1A). All red color was lost in 20R2RΔcsgBA carrying pSE380 at either temperature confirming the complete dependence of CR affinity on curli. At 37°C, plasmid expression of pchE eliminated all CR binding in strains 20R2R and 20R2RΔler. At 30°C, the optimum temperature for RpoS-dependent gene expression, 20R2R and its ler mutant would be expected to show their strongest CR affinity. Under such conditions, pchE expression reduced but did not eliminate CR staining. All other tested regulators had little effect on CR affinity at either 30 or 37°C. Therefore, pchE was the only tested HTR regulator that strongly affected CR binding in strains PA20 and 20R2R, repressing dye affinity at both temperatures in a ler-independent manner.
Basal pchE Expression Represses PA20 CR Affinity
The expression level of certain HTR regulators, such as the group 1 pch, from plasmid pSE380 would be similar to that expected following strong induction of the SOS response (Uhlich et al., 2018). However, HTR-encoded regulators could also influence csgD-dependent properties during non-inducing conditions. To test for such effects, CR affinity differences between parent strains and strains bearing deletions of ler, grlA, pchE, or group 1 pch representative, pchC, were determined under non-inducing conditions (Figure 1B). Loss of each regulator had minimal effect of PA20 CR affinity except for pchE whose deletion resulted in slightly increased red colony color at 37°C, indicating that basal expression of pchE represses curli formation at host temperatures (additional images of the effect of pchE deletion on CR affinity are shown in Supplementary Figure S1). Deletion of regulator grlA also resulted in a color change compared to the parent but it was weaker in intensity and more brown than that induced by pchE deletion. In 20R2R, deletion of individual regulators caused no visible color changes at either 30 or 37°C. It is not clear whether pchE failed to repress curli production in 20R2R or whether pchE-induced reductions were too subtle to be visible in the stronger curli-producing strain. Therefore, pchE was the only pch homolog controlling curli production under conditions where prophage elements were not induced by DNA damage, maintaining a slight repression in strain PA20.
PchE Is a Strong Repressor of Biofilm at 30°C
The effects of HTR regulators on biofilm formation at 30°C and 37°C were tested by expressing the cloned regulators in strains PA20, 20R2R, and mutant strains of each with deletion of ler and espA. 20R2R pSE380 did not produce biofilm at 37°C and PA20 pSE380 failed to form biofilm at either temperature (data not shown). Over-expression of the HTR regulators and deletions of ler and espA did not alter CV binding appreciably under those same strain/temperature conditions (data not shown). Therefore, only the results of strains 20R2R, 20R2RΔler, and 20R2RΔespA carrying the control plasmid or cloned regulators at 30°C are shown (Figure 2). To test multiple regulators in several different strain backgrounds under identical conditions we screened two independent samples per strain in a 96-well format and report mean CV dye absorbance values (Figure 2). A statistical analysis of every possible strain pair comparison is shown in the supplemental information (Supplementary Table S3). Deletion of ler in 20R2R slightly increased mean CV retention (P > 0.05) but espA deletion did not affect biofilm formation. Expression of the group 1 pch genes, except for pchC, lowered mean CV retention of both the wild-type 20R2R and the EspA mutant but not of the ler-deletion strain suggesting that strong group 1 gene induction causes modest biofilm reductions (<50%) by a ler-dependent, but espA independent, mechanism. In contrast, group 3 regulator, pchE, strongly reduced CV retention (>3-fold) in 20R2R, 20R2RΔler, and 20R2RΔespA (P < 0.05) indicating an espA- and ler-independent mechanism. Regulators GrlA and PchD also slightly reduced the mean CV binding in 20R2R and the mutants, but variation between replicates made interpretation more difficult. A second study with additional independent samples was conducted to confirm the observed trends focusing on the group 1 and group 3 pch regulators and the suppressive mechanisms associated with ler. Regulator pchA was tested alone as a representative of group 1 pch. As shown in Figure 3, no significant difference in CV binding was observed between 20R2R and 20R2RΔler (P > 0.05) but plasmid-based pchA expression reduced (P < 0.05) 20R2R CV binding. The reduction was not evident when pchA was plasmid expressed in 20R2RΔler, confirming a ler-dependent suppressive action for PchA. Over-expression of pchE reduced biofilm formation nearly sevenfold in both 20R2R and 20R2RΔler confirming the strong, ler-independent, pchE biofilm suppression.
FIGURE 2. Comparison of the effect of different HTR regulators on E. coli O157:H7 strain 20R2R biofilm formation on polystyrene. Crystal violet dye retention by strains 20R2R, 20R2RΔler, and 20R2RΔespA transformed with control plasmid pSE380 or pSE380 carrying cloned HTR regulatory genes following 48 h incubation in polystyrene 96-well plates at 30°C in LB-NS. Bars represent the mean CV absorbance measured at 590 nm (OD590) ± standard deviation (SD) of two independent samples. Stars indicate statistical differences (P ≤ 0.01) between each sample and the relative control (star color indicates the relative control). P-values for every sample are reported in Supplementary Table S3.
FIGURE 3. Comparison of the effect of regulators PchA and PchE on E. coli O157:H7 strain 20R2R biofilm formation on polystyrene. Crystal violet dye retention by strains 20R2R and 20R2RΔler transformed with control plasmid pSE380 or pSE380 carrying cloned pchA or pchE following 48 h incubation in polystyrene 96-well plates at 30°C in LB-NS. Bars represent the mean CV absorbance measured at 590 nm (OD590) ± SD of four independent samples. Any two means with no letter in common are significantly (P < 0.05) different by the Bonferroni LSD method.
To test for regulatory effects by the various HTR regulators under conditions where the prophage elements were not induced, we compared biofilm formation between wild-type 20R2R and strains with deletions of the individual regulators at 30°C (Figure 4). We tested a deletion of ler rather than pchD in our 8-strain test protocol. There were no significant differences attributed to deletion of any regulator compared to controls indicating that the tested regulators have little effect on biofilm formation under non-SOS-inducing, environmental growth conditions.
FIGURE 4. Comparison of the effect of the deletion of different HTR regulators on E. coli O157:H7 strain 20R2R biofilm formation on polystyrene. Crystal violet dye retention by strains 20R2R and 20R2R carrying deletions of certain HTR regulators following 48 h incubation in polystyrene 96-well plates at 30°C in LB-NS. Bars represent the mean CV absorbance measured at 590 nm (OD590) ± SD of two independent samples. Any two means with no letter in common are significantly (P < 0.05) different by the Bonferroni LSD method.
Prophage Induction Reduces pchE Expression at 37 and 30°C
The strong CR affinity and biofilm effects of pchE being the result of plasmid expression, it was deemed necessary to confirm transcription and regulation of pchE when it is encoded on the chromosome. In the previous RNA-Seq study of PA20 (Uhlich et al., 2018), pchE transcripts were identified in broth samples grown at 30°C and SMX-TM induction reduced their expression nearly twofold. We extended the pchE expression studies to include host temperatures using qRT-PCR, comparing PA20 grown on agar surfaces at 30 and 37°C, with and without exposure to SMX-TM. At 30°C, there was a greater than sixfold (SD = 1.5) decrease in pchE expression in SMX-TM-treated samples compared to the un-treated controls. When tested at 37°C, pchE expression was reduced more than sevenfold (SD = 0.4) by SMX-TM exposure. Therefore, pchE is expressed in PA20 at both host and environmental temperatures and prophage-inducing antibiotics reduce its expression at both temperatures (data not shown).
PchE Represses csgD and csgBA Expression
A likely control point for the regulation of curli-dependent functions by the HTR regulatory genes would be the csgBA structural genes or their master regulator, csgD. Expression of csgD and csgA were compared between strains carrying plasmid expressed pch regulators and the control plasmid (Figures 5, 6). At 30°C, pchE decreased PA20 csgD expression >7-fold and csgA expression >280-fold compared to the control, findings that correlate well with the complete loss of CR affinity in PA20 under those conditions (Figure 5A). At 37°C, pchE decreased PA20 csgD expression ≥6-fold and csgA expression nearly 10-fold (Figure 5B). The five other pch genes caused only small changes in csgD and csgA expression at either temperature (Figure 5).
FIGURE 5. Comparison of the effect of Pch regulators on csgD and csgA expression in strain PA20. Fold change (FC) csgD and csgA expression differences between PA20 carrying control plasmid pSE380 and PA20 carrying pSE380 with cloned pch homologs at 30°C (A) and 37°C (B). qRT-PCR was performed on cDNA derived from three independent samples of strains PA20 or 20R2R grown on T-medium agar at 30 or 37°C and analyzed using the 2–ΔΔCT method. Bars represent the mean FC of the three independent samples along with SD.
FIGURE 6. Comparison of the effect of Pch regulators on csgD and csgA expression in strain 20R2R. Fold change (FC) csgD and csgA expression differences between 20R2R carrying control plasmid pSE380 and 20R2R carrying pSE380 with cloned pch homologs at 30°C (A) and 37°C (B). qRT-PCR was performed on cDNA derived from three independent samples of PA20 or 20R2R strains grown on T-medium agar and analyzed using the 2−ΔΔCT method. Bars represent the mean FC of the three independent samples along with SD.
In strain 20R2R at 30°C, both csgD and csgA expression were increased by the pchA, pchB, pchC, and pchD but decreased by pchE. However, all changes were <2-fold compared to the control strain (Figure 6A). At 37°C, where plasmid-based expression of pchE strongly reduced CR affinity, each of the five pch resulted in only slight csgD repression (<2-fold). csgA was also affected little by the pch genes at 37°C. Only pchA induced a csgA expression decrease greater than twofold and there was substantial replicate variability in that comparison (Figure 6B). Therefore, while pchE strongly repressed PA20 csgD and csgA transcripts at both host and environmental temperatures, a similar response did not accompany the marked reduction of CR binding in 20R2R at 37°C. While it is possible that pchE controls 20R2R CR affinity through a different pathway than in PA20, a more likely explanation is that the time-point at which 20R2R transcripts were harvested was not appropriate to capture the expression changes.
Induced pchE Represses CsgA
To confirm that curli expression was responsible for the CR affinity differences in strain 20R2R following expression of pchE at 37°C we compared the concentrations of the major subunit of curli, CsgA, produced by 20R2R containing either pSE380 or pSE380::pchE, each isolated from equal numbers of cells. The SDS–PAGE separation of total formic acid soluble proteins is shown in Figure 7. Strain 43894OR, known to greatly overexpress curli, was included in this assay to help localize CsgA on the gel (Uhlich et al., 2001). Strain 43894OR and 20R2R each produced a protein band that migrated to a position corresponding to approximately 16 kDa. This size band was significantly decreased in appearance when strain 20R2R carried pSE380::pchE. The relative amounts of the CsgA containing bands produced by the different strains were quantitated by using densitometry to measure the mean value of pixels present in the CsgA containing band in the gel image (Figure 7). The CsgA containing band of 20R2R was determined to contain a significantly greater pixel amount compared to 20R2R+pSE380::pchE suggesting that the band possessed a greater concentration of that protein (Figure 7). To confirm this, the CsgA containing bands previously measured by densitometry were excised, trypsin digested and the resulting majority CsgA peptide identified and quantitated by measuring the resulting area under the peak of the peptide by using UHPLC separation and mass spectrometry. The majority CsgA peptide was specifically determined to be present in significantly greater amounts in the proteins derived from the gel band specific to 20R2R compared to those of 20R2R pSE380::pchE, as shown in the table in Figure 7.
FIGURE 7. A 12% Bis-Tris polyacrylamide gel containing formic acid treated whole cell extracts and the resulting data derived from the CsgA containing band. E. coli strains grown on T-medium agar at 37°C; OR (lane 1), 20R2R (lane 2), 20R2R+pchE (lane 3), molecular weight standards (lane M). Box marks the location of the bands containing the CsgA protein. The mean value of pixels present in the individual CsgA bands were visualized and measured by a Gel DocTM EZ Imager and Image LabTM (Bio-Rad) program. The area under the peak for the major peptide (NSDLTITQHGGGNGADVGQGSDDSSIDLTQR [triple charged]) produced from tryptic digestion of the CsgA containing band were measured by mass spectrometry.
pchE Over-Expression Represses Curli-Dependent HEp-2 Cell Adhesion
The HTR regulators had strong effects on curli-dependent CR affinity on TA, especially in strain 20R2R at 37°C. However, biotic surfaces would be a more relevant target for adhesive curli fibers at 37°C. Both curli and EspA are involved in adhesion to eukaryotic tissue; EspA playing an important role in the intimate cell attachment required for LEE TTSS secretion and curli by more general attachment to a variety of human serum and tissue proteins (Olsén et al., 1993, 1998; Sjöbring et al., 1994; Ben Nasr et al., 1996). Therefore, we also tested the effects of certain HTR regulators on HEp-2 cell adhesion using mutant and wild-type strains of PA20 and 20R2R. Because growth conditions determine curli expression, cell adhesion of parental strains was first compared using two different methods for preparing the challenge dose: growth in LB broth for 18 h at 37°C and growth on T-medium agar for 48 h at 30°C (Figure 8). HEp-2 cell adherence (conducted at 37°C) did not differ (P > 0.05) between PA20 strains cultured by the two different methods but the percentage of adhered 20R2R was more than fourfold greater (P < 0.05) when the bacteria were collected from agar rather than from broth. Therefore, we harvested all challenge strains from T-medium agar after 48 h at 30°C. We focused the adhesion studies on the group 1 pch and pchE, the most active regulators in CR-binding and biofilm assays, and used pchA as the representative for the group 1 genes (Figure 9). We also confirmed the repressive effect of pchE on csgD at 37°C in EMEM using qRT-PCR. Plasmid-based expression of pchE reduced PA20 csgD expression threefold (results not shown).
FIGURE 8. Influence of different growth conditions on the adhesion of strain PA20 and 20R2R to HEp-2 cells. Percentage of adhered PA20 and 20R2R to HEp-2 cells after 3 h exposure at 37°C in 5% CO2. Strains were grown in LB broth or on T-medium agar prior to challenge. Bars represent the mean adhesion percentage ± SD of three independent samples.
FIGURE 9. Comparison of the effect of HTR regulators PchA and PchE on the adhesion of E. coli O157:H7 strain PA20 and 20R2R to HEp-2 cells. Percentage of adhered wild-type, ΔespA, and ΔcsgBA PA20 (A) and 20R2R (B) transformed with control plasmid pSE380 or pSE380 carrying pchA or pchE regulators to HEp-2 cells following 3 h exposure at 37°C in 5% CO2. Bars represent the mean adhesion percentage ± SD of four independent samples. Any two treatment means with no letter in common are significantly (P < 0.05) different by the Bonferroni LSD method.
Elimination of curli fimbriae by csgBA deletion resulted in significant reductions in 20R2R cell adhesion, confirming the curli role in cell adhesion (Figure 9B). In PA20, where curli formation is already restricted by mlrA disruption, csgBA deletion reduced the mean adhesion percentage but it did not meet significance (P > 0.05) (Figure 9A). When pchE was over-expressed, the adhesion percentages of both PA20 and 20R2R were reduced greater than twofold (P < 0.05) compared to the plasmid only controls. When espA was deleted in either PA20 pSE380 or 20R2R pSE380, there was no significant reduction in cell adhesion (P > 0.05) compared to the parent control strains. As group 1 pch are proven enhancers of espA, it is likely that they were not induced under the conditions of this study. However, when pchA was expressed from plasmid pSE380, HEp-2 cell adhesion was indeed increased nearly threefold in both PA20 and 20R2R (Figure 9). Finally, in the weak curli-producing strain PA20, but not in 20R2R, high pchE expression reduced cell adhesion to levels lower than those detected following csgBA deletion, which suggests that pchE may control factors other than curli that are involved in cell adhesion. Collectively, the cell studies indicate that the regulation of O157:H7 adhesion to host tissue requires the coordinated expression of various pch homologs acting on different protein adhesion factors.
A high proportion of O157:H7 clinical strains carry the Stx1 prophage inserted in the gene encoding MlrA, a transcription factor required for RpoS-dependent expression of the E. coli central biofilm regulator, csgD (Uhlich et al., 2013). Stress resistance properties in clinical strains could be enhanced by prophage excision or run-off mlrA transcription that would restore csgD function (Uhlich et al., 2016). However, a past study in strain PA20 showed that SOS induction repressed rather than activated CsgD, while simultaneously activating horizontally transferred prophage and prophage-like elements, including LEE (Uhlich et al., 2018). In the present study, certain HTR regulators were over-expressed from a plasmid to define their role in the observed csgD repression and to test their effect on O157:H7 adhesive properties during environmental and host conditions. In addition to clinical strain PA20, we also tested 20R2R, a derivative of PA20 that had spontaneously excised the Stx2 prophage, reforming mlrA, and restoring a biofilm-proficient state more adapted for environmental conditions. Our results have identified pchE as a negative regulator of csgD expression and CsgD-dependent phenotypes such as curli production, biofilm formation, and adhesion to cultured human epithelial cells. The five EHEC homologs of the EPEC perC gene have been studied extensively and a clear role for pchA, pchB, and pchC in the control of LEE through regulation of ler has been demonstrated. However, pchD and pchE had little effect on the LEE operons and their major function(s) have remained elusive (Iyoda and Watanabe, 2004; Porter et al., 2005; Uhlich et al., 2018).
At 30°C, plasmid-expression of pchE strongly repressed the expression of both csgD and csgA in PA20 but our previous RNA-Seq study and the qRT-PCR results herein both indicate that SMX-TM treatment reduces rather than increases pchE expression, which would subsequently increase csgD expression. Therefore, it is unlikely that PchE controlled the reductions in csgD expression reported in our previous SMX-TM challenge study. When expressed individually, the group 1 pch genes had minor effects on csgD. However, pchA and pchB both reduced csgA expression and biofilm formation, and a combined regulatory effect by the group 1 members, similar to the strategy used for group 1 enhancement of LEE (Porter et al., 2005), could provide significant csgD repression. Therefore, members of the group 1 pch were more likely to be responsible or partially responsible for the reduced csgD expression following SOS induction.
Although it is unlikely that PchE was responsible for the csgD repression following SMX-TM exposure, these results indicate that it is a strong csgD repressor that functions using a different, Ler-independent, mechanism than the group 1 pch. It is not clear what benefits PchE repression of csgD would provide for O157:H7 strains during growth at 30°C. PchE-imposed inhibition of curli expression seems counter-productive for environment survival; although, SOS initiation during stress could relieve the csgD repression. It is also conceivable that the reduction of csgD expression would minimize energy costs and disperse biofilm communities to aid in survival during extreme nutrient deprivation. A full understanding of the role of PchE in environmental survival will require full elucidation of the initiating cues and regulatory control of this strong curli regulator.
When the HTR regulators were tested for regulatory effects on clinical isolate PA20 at 37°C, both the group 1 pch homologs and group 3, pchE, affected adhesion to cultured HEp-2 cells. The group 1 pch genes, following SOS induction, are proven strong enhancers of adhesion to HEp-2 cells through the ler-dependent expression of espA, but the role of curli in HEp-2 adhesion has been unclear (Iyoda and Watanabe, 2004; Sharma et al., 2016). In this study, a small but consistent increase in CR binding following pchE deletion in clinical strain PA20 indicated that PchE repressed csgD and curli during growth when the SOS response was not induced. When strongly expressed, group 1 pchA generated the highest percentages of adherent PA20 and 20R2R, but under non-inducing conditions, espA was dispensable for the attachment of either strain, and the attachment of 20R2R was clearly supported by curli. Therefore, curli likely maintains a low level of non-specific cell attachment under non-induced conditions. Induction of the SOS would likely increase both curli-mediated adhesion, by decreasing pchE, and intimate adhesion, by increasing the group 1 pch.
The significance of strong curli expression for STEC attachment to host cells and disease pathogenesis was dramatically shown by the serotype 104:H4 strain responsible for a large outbreak of bloody diarrhea with HUS in Germany (Richter et al., 2014). Shiga toxin acquisition by a strain with an enhanced ability to adhere to the gut and initiate inflammation due to unusually high curli production resulted in high death losses and high incidence of HUS. In contrast, typical clinical strains of serotype O157:H7, arguably the most common disease-producing STEC serotype, have more successfully adapted to human hosts through strategies that curtail csgD expression (Uhlich et al., 2013). PchE-mediated repression of curli during non-inducing conditions may provide an additional mechanism to increase that host adaptation. Being capable of repressing CsgD expression and cell adhesion in low curli-expressing clinical strains until reversal by SOS-induction to support group 1 pch initiation of intimate adhesion adds an additional important layer of fine control to serotype O157:H7 virulence regulation.
In this study, we determined that PchE is a strong csgD repressor, defining a function for the group 3 homolog; however, it was clearly not responsible for csgD repression during SOS induction. Moreover, its regulatory role at 30°C is unclear, and will requiring additional studies to identify the specific conditions controlling its expression. Under host conditions when the group 1 pch and espA were not expressed, PchE affected curli-dependent HEp-2 cell adhesion suggesting a role in controlling early host cell attachment. Studies defining the PchE regulon and its regulatory mechanisms will help to define this potentially important O157:H7 regulatory factor.
EA, LR, and GU performed the cell culture and adhesion assays. GU, EA, and BC performed the DNA experiments. NG and AN performed the protein experiments. ER and EA carried out statistical analysis. EA, GU, NG, and ER prepared the manuscript. All authors reviewed the manuscript.
This work was supported by United States Department of Agriculture (USDA), Agricultural Research Service (ARS), National Program 108 Food Safety (Project # 8072-42000-076). This research was supported in part by an appointment to the ARS Research Participation Program administered by the Oak Ridge Institute for Science and Education (ORISE) through an interagency agreement between the U.S. Department of Energy (DOE) and the USDA. ORISE is managed by ORAU under DOE contract number DE-SC0014664. All opinions expressed in this manuscript are the authors’ and do not necessarily reflect the policies and views of USDA, ARS, DOE, or ORAU/ORISE.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
We gratefully acknowledge John Phillips (ERRC emeritus) for assistance with certain statistical analyses. We thank David Needleman (ERRC) and Ly Nguyen (ERRC) for DNA sequencing.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2018.02829/full#supplementary-material
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Keywords: E. coli O157:H7, biofilm control, cell adhesion, curli, horizontally transferred DNA regions, pch regulatory genes, pchE gene, locus of enterocyte effacement
Citation: Andreozzi E, Gunther NW IV, Reichenberger ER, Rotundo L, Cottrell BJ, Nuñez A and Uhlich GA (2018) Pch Genes Control Biofilm and Cell Adhesion in a Clinical Serotype O157:H7 Isolate. Front. Microbiol. 9:2829. doi: 10.3389/fmicb.2018.02829
Received: 03 August 2018; Accepted: 05 November 2018;
Published: 23 November 2018.
Edited by:Alain Pierre Gobert, Vanderbilt University Medical Center, United States
Reviewed by:Maria T. Brandl, Agricultural Research Service, United States Department of Agriculture, United States
Jay Mellies, Reed College, United States
Copyright © 2018 Andreozzi, Gunther, Reichenberger, Rotundo, Cottrell, Nuñez and Uhlich. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Gaylen A. Uhlich, firstname.lastname@example.org
†These authors have contributed equally to this work