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Infection and Immunity, March 2008, p. 1048-1058, Vol. 76, No. 3
0019-9567/08/$08.00+0     doi:10.1128/IAI.01383-07
Copyright © 2008, American Society for Microbiology. All Rights Reserved.

Aggregation via the Red, Dry, and Rough Morphotype Is Not a Virulence Adaptation in Salmonella enterica Serovar Typhimurium

A. P. White,¹ D. L. Gibson,^2, G. A. Grassl,^3, W. W. Kay,⁴ B. B. Finlay,^3,5 B. A. Vallance,² and M. G. Surette^1*

Department of Microbiology and Infectious Diseases, University of Calgary, Calgary, Alberta T2N 4N1, Canada,¹ Division of Gastroenterology, BC's Children's Hospital, University of British Columbia, Vancouver BC V5Z 4H4, Canada,² Michael Smith Laboratories, University of British Columbia, Vancouver BC V6T 1Z4, Canada,³ Department of Biochemistry and Microbiology, University of Victoria, Victoria BC V8W 3P6, Canada,⁴ Department of Microbiology and Immunology, University of British Columbia, Vancouver BC V6T 1Z4, Canada⁵

Received 16 October 2007/ Returned for modification 19 November 2007/ Accepted 19 December 2007

Top ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
The Salmonella rdar (red, dry, and rough) morphotype is an aggregative and resistant physiology that has been linked to survival in nutrient-limited environments. Growth of Salmonella enterica serovar Typhimurium was analyzed in a variety of nutrient-limiting conditions to determine whether aggregation would occur at low cell densities and whether the rdar morphotype was involved in this process. The resulting cultures consisted of two populations of cells, aggregated and nonaggregated, with the aggregated cells preferentially displaying rdar morphotype gene expression. The two groups of cells could be separated based on the principle that aggregated cells were producing greater amounts of thin aggregative fimbriae (Tafi or curli). In addition, the aggregated cells retained some physiological characteristics of the rdar morphotype, such as increased resistance to sodium hypochlorite. Competitive infection experiments in mice showed that nonaggregative agfA cells outcompeted rdar-positive wild-type cells in all tissues analyzed, indicating that aggregation via the rdar morphotype was not a virulence adaptation in Salmonella enterica serovar Typhimurium. Furthermore, in vivo imaging experiments showed that Tafi genes were not expressed during infection but were expressed once Salmonella was passed out of the mice into the feces. We hypothesize that the primary role of the rdar morphotype is to enhance Salmonella survival outside the host, thereby aiding in transmission.

Top ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Thin aggregative fimbriae (Tafi), also known as curli fimbriae, mediate cell-cell aggregation in Salmonella spp. These cell surface organelles are produced together with cellulose (58, 63), as well as additional polysaccharides (19) and proteins (BapA [26]), to form an extracellular matrix that links individual cells together. The phenotype associated with matrix production has been termed the rdar morphotype, characterized by the formation of colonies with red, dry, and rough morphology when cells are grown on agar media containing Congo red (11, 42). When Salmonella bacteria are grown statically in liquid media, cells can aggregate through similar physiology to form pellicles at the air-liquid interface (10, 42, 50, 60). Collectively, these phenotypes have been referred to as multicellular behaviors (41, 42).

Regulatory control of the rdar morphotype has been the subject of numerous recent studies (47, 55, 60). Genetic control is primarily focused at the level of expression of AgfD (CsgD), a transcriptional regulatory protein. AgfD activates the production of Tafi and cellulose polymers, as well as additional extracellular matrix components, such as O-antigen (O-Ag) capsule and BapA. The agfD promoter has low basal activity, relying on several accessory proteins to activate gene expression (16, 18, 60). This enables cells to respond quickly to environmental cues. The underlying patterns of gene expression are conserved in most Salmonella isolates (40, 50, 51, 60) as well as other enterobacterial species (62). One of the key signaling molecules involved in this process is cyclic diguanosine monophosphate (c-di-GMP). Kader et al. and Simm et al. have recently shown that AgfD expression and subsequent Tafi production are regulated by c-di-GMP (22, 47), through the action of several proteins containing c-di-GMP-generating, diguanylate cyclase (GGDEF) domains (43) and/or c-di-GMP-degrading, phosphodiesterase (EAL) domains (45). AdrA, a GGDEF domain-containing protein whose expression is dependent on AgfD, is required for cellulose production (41, 63). Additional GGDEF-EAL proteins may also regulate cellulose production (15), contributing to an AgfD-independent pathway (12). Some of the effects of c-di-GMP in control of the rdar morphotype may be specific to Salmonella. However, the association between high intracellular levels of c-di-GMP and sessile modes of growth is common in many bacterial species (9, 21, 25, 30, 48).

In most Salmonella isolates, the rdar morphotype is expressed under conditions of low osmolarity, nutrient limitation, and temperatures below 30°C (11, 17). This fits with current hypotheses that the rdar morphotype is important for persistence and survival of Salmonella in nonhost environments (44, 59). Cells of the rdar morphotype have enhanced resistance to desiccation as well as resistance to various antimicrobial agents (1, 19, 44, 59). Many studies have also implicated roles for Tafi, and presumably the rdar morphotype, during pathogenesis (reviewed in reference 3). Tafi have been shown to bind human extracellular matrix proteins (2, 10, 33), contact-phase proteins (4, 20, 34), plasminogen (49), and major histocompatibility complex class I (35) and appear to be recognized by Toll-like receptor 2 (TLR2) (53). In addition, Salmonella isolates can express Tafi at 37°C under specific conditions, such as iron limitation, or as the result of acquired agfD promoter mutations (42, 60).

The apparent polyfunctional nature of Tafi led us to question the role of the rdar morphotype in the life cycle of Salmonella. Since nonhost environments are generally assumed to represent nutrient-poor conditions (61), we investigated whether aggregation would occur at low cell densities and whether the rdar morphotype was involved in this process. In addition, we tested whether aggregation would provide a competitive advantage for infection in mice. We discovered that cultures grown under nutrient-limiting conditions consisted of two populations of cells, aggregated and nonaggregated, with the aggregated cells possessing resistant properties that were characteristic of the rdar morphotype. Competition experiments between aggregative wild-type (wt) and Tafi-negative, nonaggregative agfA strains showed that aggregation was a disadvantage for murine infection. Moreover, the agfB promoter controlling Tafi expression was not activated during murine infection as determined by in vivo imaging. However, agfD and yihU (O-Ag capsule) were activated in vivo, revealing that some components of the rdar morphotype could be involved in virulence.

Top ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Bacterial strains, media, and growth conditions. Salmonella enterica serovar Typhimurium strain ATCC 14028 (American Type Culture Collection, Manassas, VA) was used as the wild-type strain in this study. The isogenic agfA strain has been described previously (59). Strains were routinely grown for 16 to 20 h at 37 °C with agitation in Miller's Luria broth (Miller's LB) (1.0% salt), supplemented with 50 µg/ml kanamycin (Kan) if necessary, before additional experiments were performed. To induce microcolony formation, overnight cultures were inoculated at a dilution of 1 in 500 into 50 ml of 1/10 LB without salt (LBns) supplemented with 40 µM 2,2'-dipyridyl (Dp) (1/10 LBns-Dp) and 50 µg/ml Kan, if necessary, and grown for 2 to 5 days at 28°C without agitation. For mixed reporter experiments, overnight cultures were normalized to an A₆₀₀ of 1.0, and equal volumes were mixed prior to inoculation of the final cultures. For lux assays, overnight cultures were diluted 1 in 600 in LBns, 1% tryptone, minimal medium containing morpholinepropanesulfonic acid (MOPS) (28, 31), M9 minimal medium (Difco), or EPS medium (0.05% yeast extract, 10 mM Na₂HPO₄, 0.1% NH₄Cl, and 0.3% KH₂PO₄) (19) supplemented with 50 µg/ml Kan to a final volume of 150 µl in 96-well clear-bottom black plates (9520 Costar; Corning Inc.). The culture in each well was overlaid with 50 µl mineral oil before the assays were started (assays performed at 28°C).

Preparation of fibronectin-coated magnetic beads (FN-beads). Tosyl-activated magnetic beads (4.5 µm) (M450; Invitrogen Canada Inc.) were coated with human plasma fibronectin (catalog no. 33016-015; Invitrogen Canada Inc.) following the procedures outlined in reference 29, adding 50 µg of fibronectin to 1 ml of bead solution. Final bead solutions contained approximately 3 x 10⁹ beads per ml.

Magnetic bead-based fractionation of S. enterica serovar Typhimurium strain ATCC 14028 cultures. Ten microliters of FN-beads was added to each 1-ml aliquot of 1/10 LBns-Dp culture in 1.5-ml microcentrifuge tubes and mixed continuously at 28°C for 30 to 60 min. FN-beads and attached cells were bound to the tube edge using a Dynal MPC-96 magnet, and the supernatant was carefully removed into a new tube. Each FN-bead fraction was resuspended in 1 ml of spent medium. Spent medium was prepared from 1/10 LBns-Dp cultures by sedimentation of cells by centrifugation (6,000 x g, 15 min) and filtration of the culture supernatant (0.22-µm-pore-size filter; Millipore). For all experiments, five replicate 1-ml aliquots were analyzed.

Luminescence, total DNA, and CFU measurements. Promoter-luciferase fusions for agfB, agfD, adrA, and yihU in pCS26-Pac or pU220 reporter vectors (5) have been described previously (19, 59). Luminescence (counts per second [cps]) from three 200-µl aliquots from each 1-ml sample of final culture, FN-bead, or supernatant fraction was measured in a 96-well clear-bottom black plate (9520 Costar; Corning Inc.) using a Wallac Victor² (Perkin-Elmer Life Sciences, Boston, MA). After measurement, cells were recovered from the wells and combined with initial samples. Total DNA levels were measured by the method of Kim and Surette (24). Briefly, 500 µl of cells from the initial samples was sedimented by centrifugation (8,000 x g, 2 min), resuspended in 150 µl of filter-sterilized water, boiled for 4 min, and cooled on ice. One hundred microliters of this cell slurry was added to a 96-well plate, and 10-fold serial dilutions were performed to a final volume of 90 µl per well. Ten microliters of a 3.4 µM solution of Syto-9 (Molecular Probes, Invitrogen Canada Inc.) was added to each well, and the plate was incubated for 1 h at room temperature in the dark with agitation. Fluorescence measurements (1 s per well; 485-nm excitation, 525-nm emission) were performed in a Fusion microplate reader (Perkin-Elmer). Normalized expression values were compared by two-way analysis of variance with the sample type and number of days of growth representing independent variables; P values of <0.05 or <0.01 were considered significant.

Sodium hypochlorite experiments. FN-bead and supernatant fractions from 15 1-ml aliquots of 48-h 1/10 LBns-Dp cultures were combined prior to analysis. Aliquots (500 µl) of FN-bead or supernatant fractions were combined with 100 µl of sterile water (pH 7) (Invitrogen Canada Inc.) or sodium hypochlorite solutions (bleach; to a final concentration of 20, 40, 60, or 100 ppm) and mixed continuously for 10 min at room temperature. Cells were sedimented by centrifugation (7,000 x g, 2 min), the supernatant was removed, and 500 µl of phosphate-buffered saline (PBS), pH 7.4, was added. For CFU determination, each individual sample was homogenized in a tissue grinder for 15 to 20 s, serially diluted in triplicate in PBS, and plated in duplicate in 5-µl drops onto LB agar and incubated at 28°C overnight. The initial CFU values were 4.8 x 10⁵ ± 1.8 x 10⁵ CFU for FN-beads and 1.7 x 10⁷ ± 0.1 x 10⁷ CFU for supernatants. The survival values (log CFU after treatment/log CFU before treatment) at each concentration of sodium hypochlorite were compared by unpaired t tests; P values of <0.05 were considered significant.

Fluorescence microscopy. Fluorescence reporters for agfB, adrA, and yihU were generated from the corresponding pCS26 or pU220 vector by replacing the NotI-NotI fragment containing luxCDABE with NotI-NotI fragments containing either gfp from pCS21 (5) or eCherry PCR amplified from pFFUNR (M. Elowitz) using primers eCherryF (CTGATTGCGGCCGCGTTTAACTTTAAGAAGGAGCACCTG) and eCherryR (CTGATTGCGGCCGCGTTATTATTATTTGTACAGCTCATCCATG) (NotI restriction sites are underlined). For phase-contrast microscopy, differential interference contrast microscopy (DICM), or fluorescence microscopy (FM), 30-µl aliquots of culture, FN-bead, or supernatant fractions were pipetted onto glass slides, covered with 9- by 9-mm glass coverslips pretreated with poly-L-lysine (Sigma) following established procedures (14), and sealed with Mowiol glue (EMD Biosciences Inc.). Cells and reporters were visualized with Leica DM IRE2 and DM RXA2 fluorescence microscopes using 470-nm excitation and 525-nm emission for green fluorescent protein (GFP) and 575-nm excitation and 640-nm emission for eCherry.

Competitive infection of mice. Female C57BL/6 (Salmonella-susceptible) mice (6 to 10 weeks old) were purchased from Jackson Laboratory (Bar Harbor, ME) and housed in the animal facilities at the University of British Columbia in direct accordance with guidelines drafted by the University of British Columbia's Animal Care Committee and the Canadian Council on the Use of Laboratory Animals. Groups of five mice were infected orally with approximately 2 x 10⁶ CFU total of a mixed inoculum in 100 µl of 100 mM HEPES containing an approximate 1:1 ratio of strain ATCC 14028 and agfA strain. Strains used in the inoculum were grown in either nutrient-rich (NR) conditions (Miller's LB at 37°C for 16 h; A₆₀₀ of 3.0 to 3.1) or nutrient-limiting (NL) conditions (1/10 LBns-Dp at 28°C for 48 h; A₆₀₀ of 0.25 to 0.29). The appropriate dilutions for each strain under each growth condition were determined by total DNA measurements, and the doses administered were determined by serial dilution and plating. The ratios of strains administered (CFU of agfA strain/CFU of strain ATCC 14028) were 1.10 for the mice under NR conditions and 1.24 for the mice under NL conditions. Infected mice were humanely euthanized 96 h postinfection, prior to homogenization of the spleen, mesenteric lymph nodes (MLN), small intestine, and colon in PBS using a high-speed mixer mill (MM301; Retsch, Newtown, PA). Organ homogenates were serially diluted in PBS and plated on XLD agar (Oxoid, United Kingdom) for determination of total Salmonella CFU. Colonies were replica plated onto 1% tryptone agar containing 100 µg/ml Congo red, and cells were grown at 28°C to differentiate between wt and agfA bacteria. The competitive index (CI) was calculated as [CFU mutant/CFU wild-type]_output/[CFU mutant/CFU wild-type]_input. CI data were analyzed using the Mann-Whitney U test; P values of <0.05 were considered significant.

Bioluminescence imaging of Salmonella reporter strains during murine infection. Female C57BL/6 mice were infected orally with 10⁷ CFU of strain ATCC 14028 agfD, agfB, yihU, sig70_16, or sig38H4 luciferase reporter strains grown for 16 h in Miller's LB at 37°C. sig70_16 and sig38H4 reporters contain control promoters dependent on RpoD (⁷⁰) and RpoS (^s), respectively, and have been described previously (23, 59). Infected mice were euthanized, and their gastrointestinal tracts and organs were removed and imaged for 4 min using an IVIS 100 (Xenogen, Alameda, CA). Grayscale reference images were overlaid with images capturing the emission of photons from the ATCC 14028 reporter strains using LIVING IMAGE software (Xenogen) and Igor (Wavemetrics, Seattle, WA). To determine the total number (CFU) of bioluminescent Salmonella, the spleen, liver, MLN, ileum, cecum, and colon were homogenized in PBS using a high-speed mixer mill (MM301; Retsch, Newtown, PA), diluted, and plated on LB agar supplemented with 50 µg/ml Kan. To determine the prevalence of plasmid loss, ground tissue mixtures were grown on XLD agar (Oxoid, United Kingdom), and the colonies were imaged for bioluminescence production.

Top ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

 
Salmonella aggregation occurs at low cell densities in NL liquid media. Although the rdar morphotype is easily studied during Salmonella growth in rich media, such as LB, problems arise when trying to compare aggregative strains that form large, recalcitrant cell aggregates to nonaggregative strains where the cells can be easily dispersed. If starvation could be induced at low cell densities, we hypothesized that cell aggregates formed would remain small enough to facilitate comparisons between strains and allow us to evaluate the role of aggregation in Salmonella virulence. Furthermore, we reasoned that starvation at low cell densities would represent a more natural growth state for Salmonella.

We investigated growth of S. enterica serovar Typhimurium ATCC 14028 in a variety of NL conditions. The level of aggregation was estimated by monitoring agfB expression from a promoter-luciferase reporter. As expected, cell density and agfB expression reached the highest level in LBns (Fig. 1, bar 1), which was used as a nutrient-rich control medium. However, when cells were grown in dilute LBns (Fig. 1, bars 2 and 3), cell density was lower (A₆₀₀ < 0.3), but agfB expression remained relatively high. In M9 minimal medium, both cell density and agfB expression measurements were generally low (Fig. 1, bars 4, 5, 6, and 7). Only in M9 minimal medium without sulfate did agfB expression reach higher levels (Fig. 1, bar 8). In minimal medium containing MOPS supplemented with 0.72% glucose, cell density was relatively high, while agfB expression was low (Fig. 1, bar 9). However, in minimal medium containing MOPS supplemented with 0.036% glucose or containing MOPS without bicarbonate, nitrogen, or phosphate (Fig. 1, bars 10, 11, 12, and 13), agfB expression was increased, and cell density was low. Cells grown on EPS medium had intermediate cell density and agfB expression levels (Fig. 1, bar 14). The addition of 5 mM c-di-GMP to dilute LBns or minimal medium containing MOPS had very little effect on agfB expression (data not shown). Further analysis by light microscopy revealed that cultures grown in 1/10 LBns (Fig. 1, bar 3) contained the highest proportion of aggregated cells. Therefore, this medium was chosen for use in subsequent experiments.

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FIG. 1. agfB expression versus cell density during growth of S. enterica serovar Typhimurium strain ATCC 14028 in nutrient-limiting conditions. Expression of an agfB promoter-luciferase fusion was measured during growth of strain ATCC 14028 at 28°C in different media. The strain was grown in different media as follows: bar 1, LB without salt (LBns); bar 2, 1/4 LBns; bar 3, 1/10 LBns; bar 4, M9 minimal medium alone; bars 5 to 7, M9 minimal medium supplemented with 0.5% Casamino Acids (bar 5), 0.05% glycerol (bar 6), or 0.05% glucose (bar 7); bar 8, M9 minimal medium without sulfate; bars 9 and 10, minimal medium containing MOPS supplemented with 0.72% glucose (bar 9) or 0.036% glucose (bar 10); bars 11 to 13, minimal medium containing MOPS without bicarbonate (bar 11), nitrogen (bar 12), or phosphate (bar 13); and bar 14, EPS medium (bar 14). Bars correspond to the average maximum optical density measurements during the 48-h growth period; white circles represent the average maximum luminescence values (counts per second [CPS]). Error bars represent the 95% confidence intervals determined from three replicate samples.

rdar morphotype genes are expressed during growth in NL conditions. Expression of rdar morphotype genes agfD, agfB, adrA, and yihU, a gene required for biosynthesis of O-antigen capsule (19), was monitored during growth of strain ATCC 14028 in 1/10 LBns at 28°C. Activation of yihU occurred before the other genes, within the first 5 h of growth (Fig. 2). Expression of agfD, agfB, and adrA occurred approximately 5 h later and was synchronized (Fig. 2) as previously reported (55, 59). agfB expression was activated at least 10 h earlier in 1/10 LBns than in nutrient-rich LBns medium (Fig. 2, broken line); this same trend was observed for agfD, adrA, and yihU (data not shown). Since iron limitation is known to stimulate agfD expression (41, 42), gene expression was measured in media supplemented with 40 µM Dp, a well-characterized iron chelator (5). Overall growth was unaffected by iron depletion under these conditions (Fig. 2, inset), but the reporter strains had altered gene expression. For each time point between 25 h and 40 h, expression levels for all four reporter strains were significantly higher in the iron-depleted media (P < 0.05; unpaired t tests). Maximum expression was significantly increased only for agfD (P < 0.05; unpaired t test). These experiments indicated that Tafi, cellulose, and O-Ag capsule were being produced under NL conditions.

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FIG. 2. Temporal expression of rdar morphotype genes during growth of strain ATCC 14028 in 1/10 LB without salt at 28°C. Expression of agfD, agfB, adrA, or yihU promoter-luciferase fusions was measured during growth of strain ATCC 14028 in 1/10 LBns (open symbols) or 1/10 LBns supplemented with 40 µM 2,2'-dipyridyl (closed symbols) at 28°C with agitation. Curves represent the average luminescence (counts per second [CPS]) from three biological replicates of each reporter strain as a function of time. Measurements for yihU and adrA are on the right x axis. The broken line represents agfB expression during growth of strain ATCC 14028 in LBns at 28°C with agitation. Inset in upper left represents cell density of cultures (A620) as a function of time.

Tafi are essential for cell-cell aggregation. To investigate the importance of Tafi in the aggregation process, strain ATCC 14028 and agfA cultures were analyzed by DICM. After 6 h of growth in LBns at 28°C, cells in both wt and agfA cultures were dispersed as individual, planktonic cells (Fig. 3A). This result was expected, since 6 h corresponds to a time period when agfD and agfB expression are at background levels (Fig. 2). After 48 h growth in 1/10 LBns-Dp, DICM analysis revealed that strain ATCC 14028 cultures consisted of small clumps of cells (Fig. 3B, ST 14028, top panel), large aggregates of cells or "microcolonies" (Fig. 3B, ST 14028, bottom panel) and individual, planktonic cells. In contrast, agfA cultures consisted entirely of planktonic cells and were devoid of cell clumps (Fig. 3B). This demonstrated that Tafi were essential for cell-cell aggregation under these growth conditions.

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FIG. 3. Cell-cell aggregation in strain ATCC 14028 and agfA cultures. S. enterica serovar Typhimurium strain ATCC 14028 (ST 14028) and agfA cultures were analyzed by differential interference contrast microscopy after growth in LBns for 6 h (A) or in 1/10 LBns-Dp for 48 h (B) at 28°C without agitation. Pictures in the top and bottom panels in panel B were taken from the same cultures. A600 values were 0.208 (A) and 0.229 (B) for strain ATCC 14028 cultures and 0.288 (A and B) for agfA cultures. Each picture was magnified 40,000x. Dp, 2,2'-dipyridyl.

Aggregated cells can be isolated from strain ATCC 14028 cultures based on the presence of Tafi. To visualize gene expression in individual cells, cultures of strain ATCC 14028 containing an agfB::gfp reporter were analyzed by FM. After 48 h of growth in 1/10 LBns-Dp at 28°C, GFP expression was primarily localized to the aggregated cell clumps, whereas individual, planktonic cells had little or no expression (Fig. 4A). This indicated that the aggregated cells were producing greater amounts of Tafi than the planktonic cells. Based on the principle that purified Tafi are able to bind fibronectin (K_D of 74 µM [10]), fibronectin-coated magnetic beads (FN-beads) were used to fractionate the cultures. The FN-bead fraction consisted of large "microaggregates" greater than 75 µm in diameter (Fig. 4B) and smaller clumps of 20 to 50 cells (Fig. 4C), with all cells in the aggregates displaying uniform GFP expression. In contrast, cells that did not bind to the FN-beads and remained in the supernatant fraction had little or no GFP expression (Fig. 4D). Recovery of cells after culture fractionation was not 100% efficient; cells in the FN-bead fraction represented 10.4% ± 7.1% of the total cells in the culture based on CFU and 6.5% ± 3.3% based on total DNA measurements, whereas cells in supernatant fraction represented 73.6% ± 21.5% based on CFU and 88.1% ± 8.2% based on total DNA measurements.

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FIG. 4. agfB expression in individual cells from different cell fractions of strain ATCC 14028 cultures. Strain ATCC 14028 agfB::gfp reporter strain cultures grown in 1/10 LBns-Dp for 72 h at 28°C were visualized by light microscopy (images on left) and fluorescence microscopy (images on right) either directly (A) or after fractionation with fibronectin-coated magnetic beads (B, C, and D). Representative cells from bead fractions (B and C) and supernatant fractions (D) are shown; arrowheads indicate beads that are bound to cells. Scale bars are shown at bottom right of the light microscopy images.

Expression differences between the aggregated and planktonic cell fractions were confirmed using strain ATCC 14028 agfB::lux cultures grown for 2, 3, 4, or 5 days. On day 2, agfB expression was approximately 20 times higher in cells from the FN-bead fraction compared to cells in the supernatant fraction (Fig. 5). Expression in the FN-bead fractions remained high on day 3 but dropped to only three times higher than the supernatant fractions by day 5 (Fig. 5). During this time period, there were no visible changes in the cultures and A₆₀₀ measurements remained constant (data not shown). agfB expression in cells from the supernatant fractions was consistently low (<1,000 relative light units) for the duration of the experiment (Fig. 5). Expression levels did fluctuate for the unfractionated cultures but always were intermediate between the FN-bead and supernatant fractions (Fig. 5).

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FIG. 5. Quantification of agfB expression in strain ATCC 14028 cultures fractionated with fibronectin-coated magnetic beads. The ATCC 14028 agfB::lux reporter strain was grown in 1/10 LBns-Dp for 48 to 120 h at 28°C without agitation prior to fractionation with fibronectin-coated magnetic beads (FN-beads). Expression (cps) from cells in unfractionated culture, FN-bead, and supernatant fractions was normalized to the amount of DNA in each sample and is represented as relative light units (RLU). Bars represent the average RLU values ± standard deviations (error bars) from five independent samples measured in triplicate. Statistically significant differences between FN-beads, supernatant, and culture samples are noted by asterisks (**, P < 0.01; *, P < 0.05) as determined by two-way analysis of variance.

Strain ATCC 14028 microaggregates are not clonal. To determine whether strain ATCC 14028 microaggregates were producing cellulose, adrA expression was monitored using a fluorescent eCherry reporter. Cultures were fractionated with FN-beads, and the majority of large cell clumps were positive for eCherry expression (data not shown). This indicated that the cell aggregates were producing cellulose. Some individual cells were eCherry positive, but these were quite rare (data not shown). These results enabled us to perform dual-labeling experiments to test whether the cell aggregates were clonal. When strain ATCC 14028 agfB::gfp and adrA::eCherry reporter strains were grown together and cultures were fractionated with FN-beads, each one of the >50 large cell aggregates examined displayed both GFP and eCherry expression (Fig. 6A and B). GFP expression was often localized to specific clumps of cells in the aggregate, whereas eCherry expression appeared to be spread throughout (Fig. 6A and B). Several regions of the cell aggregates were yellow, with overlapping GFP and eCherry expression; this was due to cells present in different focal planes of the three-dimensional clumps. These experiments showed that the larger cell aggregates were not clonal, indicating that aggregation occurred between adjacent cells during growth.

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FIG. 6. Expression of adrA and agfB in strain ATCC 14028 cell aggregates bound to fibronectin-coated magnetic beads. ATCC 14028 agfB::gfp and adrA::eCherry reporter strains were grown together in 1/10 LBns-Dp for 72 h at 28°C without agitation prior to fractionation with FN-beads and analysis by differential interference contrast microscopy and fluorescence microscopy. (A and B) DICM images of representative cell aggregates with scale bars shown; (C and D) DICM and FM images that have been merged.

Strain ATCC 14028 microaggregates are more resistant to sodium hypochlorite than planktonic cells. From the observation that strain ATCC 14028 microaggregates were expressing Tafi and cellulose, we hypothesized that aggregated and planktonic cells would have measurable physiological differences. Cells in FN-bead or supernatant fractions from strain ATCC 14028 cultures were exposed to sodium hypochlorite. Cells from both fractions survived equally well when exposed to low concentrations (Fig. 7; 20 ppm) and were killed when exposed to high concentrations (Fig. 7, 100 ppm). However, at 40 ppm, cells in the supernatant fraction had a decrease in survival of 1 log₁₀ unit compared to FN-bead cells, and at 60 ppm, the difference was statistically significant at greater than 4 log₁₀ units (Fig. 7). Therefore, the aggregated cells in FN-bead fractions represented a more resistant physiological state than planktonic cells in the supernatant fractions.

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FIG. 7. Survival of cells in different strain ATCC 14028 culture fractions following exposure to sodium hypochlorite. Strain ATCC 14028 cells were grown in 1/10 LBns-Dp for 48 h at 28°C without agitation prior to fractionation with FN-beads. Cells in the FN-bead and supernatant fractions were exposed to different levels of sodium hypochlorite for 10 min. Each value represents the average relative survival from at least four samples; the error bars reflect the 95% confidence intervals. Statistically significant differences (P < 0.05) between the FN-bead and supernatant fractions at different hypochlorite concentrations are noted by an asterisk.

Competitive index infections in mice. We reasoned that the rdar morphotype might be a common physiological form of Salmonella encountered by susceptible hosts, an idea strengthened by the finding that Tafi are recognized by TLR-2 (53). This theory led us to investigate whether cell aggregates expressing the rdar morphotype would have an advantage over planktonic cells for passage through the murine intestinal tract. The test group of C57BL/6 mice (susceptible) were infected orally with an equal mixture of strain ATCC 14028 and agfA cells grown in NL conditions at 28°C, conditions where the wt culture was a mixture of cell aggregates and planktonic cells, whereas the agfA culture consisted of planktonic cells only. Control mice were infected orally with an equal mixture of strain ATCC 14028 and agfA cells grown in NR conditions at 37°C, conditions where both wt and agfA cultures consisted entirely of planktonic cells. Organ colonization levels and CI ratios were determined at 4 days postinfection.

The numbers of colonizing Salmonella ranged from 10¹ to 10⁵ CFU in spleen and MLN and 10¹ to 10⁶ CFU in the colon and small intestine (Fig. 8A). In general, mice infected with Salmonella grown in nutrient-limiting conditions had higher CFU loads in these organs than mice infected with cells grown in nutrient-rich conditions (Fig. 8A), although the differences were not statistically significant. The average CI for agfA cells was greater than 1 in each of the organs of the mice grown in NL condition (Fig. 8B), indicating that the nonaggregative agfA cells were able to outcompete aggregation-positive wt cells during colonization and infection. In contrast, the CI values measured in organs of the mice grown in NR conditions were close to a value of 1 (Fig. 8B), indicating there was no advantage for the agfA strain compared to the wt when both strains were planktonic. The difference between the NL and NR groups of mice was statistically significant in the spleen (Fig. 8B).

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FIG. 8. Competitive index infections of agfA strain and strain ATCC 14028 in C57BL/6 mice. Groups of mice were infected with a mixed inoculum of agfA strain and strain ATCC 14028 cells that were grown in nutrient-rich conditions at 37°C (NR) or nutrient-limiting conditions at 28°C (NL). The total numbers of colonizing Salmonella (A) and CI for the agfA strain (B) were determined in the spleen, MLN, colon, and small intestine (Sm Int.). Each data point represents one animal, and horizontal bars indicate means. The broken line in panel A represents the limit of detection (10 CFU), and the broken line in panel B represents a CI value of 1, which would result if there was no competitive difference between the agfA strain and strain ATCC 14028. P values are listed above CI results from each organ, The asterisk represents statistical significance (P < 0.05).

Bioluminescence imaging of rdar morphotype gene expression during murine infection. To visualize rdar morphotype gene expression during infection, mice were infected orally with strain ATCC 14028 containing agfD, agfB, or yihU luciferase reporter. Control groups of mice were infected with strain ATCC 14028 containing ⁷⁰ (RpoD)- or RpoS-dependent luciferase reporters. All strains were grown in NR conditions prior to infection. agfD expression was detected from the small intestine, liver, spleen, and MLN (Fig. 9A). Expression of yihU was also detected from the ileum, spleen, and liver (Fig. 9A). In contrast, agfB expression was not detected in any of the infected mice, indicating that Tafi were not produced during murine infection. As expected, bioluminescence corresponding to ⁷⁰ activity was detected in all mice, from the spleen, liver, and MLN, as well as throughout the gastrointestinal tract (Fig. 9A). RpoS activity was also detected but was primarily localized to the ileum, liver, and spleen (Fig. 9A). Colonization levels for the Salmonella reporter strains in C57BL/6 mice ranged from 10⁵ to 10⁹ CFU in the spleen, 10⁵ to 10⁸ CFU in the liver, 10⁵ to 10⁷ CFU in the MLN, 10⁷ to 10⁸ CFU in the small intestine, 10⁵ to 10⁹ CFU in the cecum, and 10⁶ to 10⁹ CFU in the colon. The percentage of plasmids carrying Salmonella recovered from the different tissues ranged between 100 and 10; generally, bacteria isolated from the cecum and colon had more plasmid loss than bacteria isolated from the spleen, liver, and MLN. When plasmid loss values from all tissues were averaged, each ATCC 14028 reporter strain was determined to have plasmid loss of less than 40% with no significant differences between reporters (data not shown). Bioluminescence from all reporters, including agfB, was detected in fecal pellets from the infected mice (Fig. 9B). Shedding of bioluminescent Salmonella occurred as early as 15 h postinfection (data not shown). The strongest signals were detected from agfD and the control ⁷⁰ reporter (Fig. 9B).

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FIG. 9. Bioluminescence imaging of Salmonella rdar morphotype gene expression in mice infected by oral gavage. (A) In vivo bioluminescence of the gastrointestinal tracts and organs of C57BL/6 mice following infection with strain ATCC 14028 agfD, agfB, yihU, sig70_16 (70), and sig38H4 (RpoS) luciferase reporter strains. Images show the relative signal intensity visualized at a given anatomical location within tissue (small intestine [Sm Int], mesenteric lymph nodes[MLN], spleen [Sp], liver [Li], and colon [Co]). In the color bars displayed on the right of each image, red corresponds to the highest signal intensity and blue corresponds to the lowest signal intensity in units of light measurement (photons/second/cm2/seradian). Representative images are shown from 3 (yihU and RpoS) or 13 (agfD, agfB, and 70) mice. (B) Bioluminescent images of fecal pellets from mice infected with strain ATCC 14028 reporter strains. Pellets were collected between 60 h and 84 h postinfection. The scale of signal intensity for each image is located on the right.

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In this study, we analyzed growth of S. enterica serovar Typhimurium under nutrient-limiting conditions, conditions predicted to occur in natural environments, to examine the role of the rdar morphotype in nature. We observed that the formation of microaggregates occurred at low cell densities. The rdar morphotype was directly linked to the aggregation observed; agfD, agfB, adrA, and yihU genes associated with production of Tafi, cellulose, and O-Ag capsule were activated early in growth. Iron depletion caused an increase in agfD expression as reported previously (42), as well as prolonged elevated expression for downstream components agfB, adrA, and yihU. Since the timing of gene expression was not changed by iron depletion, we hypothesized that cells were aggregating in response to the depletion of additional nutrients. We also observed that Salmonella aggregation was associated with a lack of phosphate, bicarbonate, and sulfate. It is assumed that each of these starvation responses converges through the activation of RpoS (36). The addition of exogenous c-di-GMP did not affect agfB gene expression, although this may not accurately mimic production of this signaling molecule by GGDEF domain proteins inside the cell.

At low cell densities, Salmonella cultures consisted of two distinct populations of cells, aggregated and nonaggregated, with the aggregated cells contributing the majority of rdar morphotype gene expression. This is in contrast to Salmonella aggregation during growth in rich media, where the cell population behaves as a multicellular unit (42, 47, 59, 63). We confirmed a difference between aggregated and nonaggregated cells using fluorescence microscopy with GFP and eCherry reporters, isolation of aggregated cells through binding to fibronectin-coated magnetic beads, and quantitation of expression differences using an agfB luciferase reporter. It was determined that large cell aggregates in the wt cultures were formed from clusters of cells that aggregated followed by growth within the aggregates. Many cells in the wt cultures remained planktonic; therefore, aggregation was assumed to be an active process without "trapping" of planktonic cells, which may occur in the formation of large pellicles at the air-liquid interface in mixed cultures (26, 44). We were unable to determine whether smaller cell clumps (i.e., <20 cells) were clonal due to the difficulty in visualizing adrA::eCherry expression in individual cells. This difficulty is most likely explained, because adrA is a weaker promoter than agfB (Fig. 2) (59) and eCherry is not as bright as GFP (46). However, it is possible that adrA expression is activated only after large cell aggregates are formed.

Physiological differences were detected between aggregated cells and nonaggregated cells isolated from strain ATCC 14028 cultures. The aggregated cells had an enhanced resistance to 60 ppm sodium hypochlorite of up to 4 log₁₀ units compared to the nonaggregated cells. Since cellulose is strongly associated with resistance to sodium hypochlorite (44, 50, 59), these results confirmed indirectly that aggregated clumps of cells were producing cellulose. The aggregated cells did not have enhanced resistance to desiccation compared to nonaggregated cells (A. P. White and M. G. Surette, unpublished data). We were unable to determine whether aggregated cells were producing O-Ag capsular polysaccharide, which is of primary importance for desiccation resistance (19), because the yihU promoter was not strong enough to visualize with either the GFP or eCherry reporter (data not shown). Nevertheless, the aggregated cells exhibited some of the same physiological properties as those of the rdar morphotype colonies and pellicles (1, 44, 59), suggesting that the formation of small cell aggregates could enhance Salmonella survival in natural environments.

Competitive infection experiments between wt strain ATCC 14028 and agfA strains indicated that aggregation is a disadvantage for murine infection. This result contradicts previous hypotheses that resistant rdar morphotype components would aid in passage through the stomach and intestinal tract (11, 63). The inclusion of 100 mM HEPES in our inoculums would have buffered the stomach acid, reducing any survival differences between aggregated and planktonic cells (1). This is potentially significant, since tests with human volunteers have demonstrated that buffering of the stomach pH reduces the infectious dose of Salmonella (6). Determination of the CI ratios at the 96-h time point may be more a measure of colonization efficiency and may not accurately assess passage through the stomach; therefore, it is possible that the ratio of strains was different at earlier time points. Despite these potential caveats, the agfA strain was consistently detected at higher levels in the internal organs of the infected mice. If formation of microaggregates provided wt cells an advantage over agfA planktonic cells in passage through the stomach, it is assumed that this would have been detected. One possibility is that phagocytosis is inhibited by the presence of the extracellular matrix and, therefore, fewer Salmonella go systemic. Planktonic cells may also have increased access to host receptors required for systemic spread. The overall conclusion from these CI experiments was that aggregation is not a virulence adaptation in Salmonella.

Analysis of rdar morphotype gene expression during infection revealed unexpected complexities. Although agfD expression was consistently detected inside the infected mice, agfB expression was not detected. This result was unexpected because agfD and agfB expression has been tightly coupled in all culture conditions examined (17, 38, 39, 41, 59) (White and Surette, unpublished). agfD expression in vivo may be below a threshold level required for agfB activation (60). Alternatively, the uncoupling of agfD and agfB expression may indicate the absence of a signaling event or presence of an inhibitory condition or factor that is preventing agfB expression inside the host. agfB was expressed by Salmonella as the bacteria were shed in the feces, however, which indicates that this environment was conducive for Tafi production. The change in agfB expression may be partially due to a drop in temperature, since maximal expression in vitro is achieved at temperatures below 30°C (42, 55).

The finding that Tafi were not expressed during murine infection explains why agfA strains are not attenuated for virulence as reported previously (56). In addition, this result calls into question previous reports on the ability of Tafi to bind various host proteins and associated factors (3). These interactions could conceivably occur if Tafi are present in the initial stages of infection and cells are engulfed and passed into the bloodstream (54) where Tafi could persist for longer time periods. On the other hand, the "sticky" nature of native preparations of Tafi or curli fimbriae, which are mixtures of aggregative protein and polysaccharides (19, 58, 63), could easily cause in vitro binding artifacts. adrA was not included in our in vivo bioluminescence experiments, but it has been shown that cellulose production is also not required for Salmonella virulence in the murine model of infection (50). It is important to consider whether it is suitable to extrapolate results from the systemic infection caused by serovar Typhimurium in mice to the self-limiting gastroenteritis infection that occurs in humans. We hypothesize that the principles of survival and passage through the stomach and intestine are similar and that Tafi and cellulose are not important for Salmonella virulence under infection conditions similar to those reported here.

Expression of agfD inside the host suggested that AgfD could be functioning in a regulatory capacity during murine infection. AgfD is known to regulate yihU (19), bapA (26), and many additional genes in culture (7, 8, 18). The possibility that Salmonella produces an O-Ag capsule during infection is significant. Polysaccharide capsules can mediate resistance to important host defense mechanisms, including phagocytosis and complement-mediated killing, and are important for virulence of diverse pathogenic bacteria, such as S. enterica serovar Typhi (reviewed in reference 37), Streptococcus spp. (27, 32), Haemophilus influenzae (52), Francisella tularensis (57), and Burkholderia mallei (13). AgfD may also be responsible for bapA expression in vivo. BapA was recently shown to be important for initial colonization in mice, and presumably as a result, bapA mutants were attenuated for virulence (26). These results indicate that the rdar morphotype could have a complex role in the life cycle of Salmonella.

In our competitive infection experiments, there was no difference in colonization by cells grown in nutrient-rich versus nutrient-limiting conditions, suggesting that Salmonella infection will occur if enough cells reach the small intestine. Expression of the rdar morphotype would ensure that more cells survive outside the host to be able to cause infection, which may explain why this phenotype has been conserved through evolution (60). The finding that all rdar morphotype genes analyzed were expressed in fecal pellets seems to be consistent with this hypothesis. The few S. enterica serovars that have lost the ability to aggregate via the rdar morphotype, such as serovars Typhi and Choleraesuis (40; A. P. White, S. L. Stocki, K. E. Sanderson, and M. G. Surette, unpublished observations), share an ability to cause systemic disease. It is possible that the loss of the rdar morphotype in these groups of strains represents a biological trade-off for increased virulence or host colonization at the expense of long-term survival in the environment. If the primary role of aggregation in the Salmonella life cycle is for survival in nutrient-limiting conditions, loss of the rdar morphotype could reflect differences in the modes of transmission for different serovars.

 
We thank S. Altman and M. Elowitz for providing the pFUN-R vector and C. H. Collins for cloning the eCherry reporter, K. Sanderson and S. Stocki for critical reading of the manuscript, and J. Wain, A. Weljie, and members of the Surette laboratory for helpful discussions. DICM and FM work was performed with the help of M. Schoel in the Microscopy and Imaging Facility at the University of Calgary and with RD.

This work was supported by grants from the Canadian Institutes of Health Research to M.G.S. and B.A.V. and through Genome Prairie, Genome BC, and Inimex Pharmaceuticals through the Functional Pathogenomics of Mucosal Immunity project. M.G.S. is supported as an Alberta Heritage Foundation for Medical Research (AHFMR) Scientist and Canada Research Chair in Microbial Gene Expression. D.L.G. was supported by postdoctoral fellowships from CAG/CIHR/Astrazenica and the Michael Smith Foundation for Health Research. A.P.W. was supported by a postdoctoral fellowship from AHFMR.

 
* Corresponding author. Mailing address: Department of Microbiology and Infectious Diseases, University of Calgary, Faculty of Medicine, 268 Heritage Medical Research Building, 3330 Hospital Drive NW, Calgary, Alberta T2N 4N1, Canada. Phone: (403) 220-2744. Fax: (403) 270-2772. E-mail: surette{at}ucalgary.ca

Published ahead of print on 14 January 2008.

Editor: A. J. Bäumler

These authors contributed equally to this work.

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Infection and Immunity, March 2008, p. 1048-1058, Vol. 76, No. 3
0019-9567/08/$08.00+0     doi:10.1128/IAI.01383-07
Copyright © 2008, American Society for Microbiology. All Rights Reserved.

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