- Research article
- Open Access
Zinc protects against shiga-toxigenic Escherichia coli by acting on host tissues as well as on bacteria
BMC Microbiology volume 14, Article number: 145 (2014)
Zinc supplements can treat or prevent enteric infections and diarrheal disease. Many articles on zinc in bacteria, however, highlight the essential nature of this metal for bacterial growth and virulence, suggesting that zinc should make infections worse, not better. To address this paradox, we tested whether zinc might have protective effects on intestinal epithelium as well as on the pathogen.
Using polarized monolayers of T84 cells we found that zinc protected against damage induced by hydrogen peroxide, as measured by trans-epithelial electrical resistance. Zinc also reduced peroxide-induced translocation of Shiga toxin (Stx) across T84 monolayers from the apical to basolateral side. Zinc was superior to other divalent metals to (iron, manganese, and nickel) in protecting against peroxide-induced epithelial damage, while copper also showed a protective effect.
The SOS bacterial stress response pathway is a powerful regulator of Stx production in STEC. We examined whether zinc’s known inhibitory effects on Stx might be mediated by blocking the SOS response. Zinc reduced expression of recA, a reliable marker of the SOS. Zinc was more potent and more efficacious than other metals tested in inhibiting recA expression induced by hydrogen peroxide, xanthine oxidase, or the antibiotic ciprofloxacin. The close correlation between zinc’s effects on recA/SOS and on Stx suggested that inhibition of the SOS response is one mechanism by which zinc protects against STEC infection.
Zinc’s ability to protect against enteric bacterial pathogens may be the result of its combined effects on host tissues as well as inhibition of virulence in some pathogens. Research focused solely on the effects of zinc on pathogenic microbes may give an incomplete picture by failing to account for protective effects of zinc on host epithelia.
Zinc has been tested for its ability to treat and prevent diarrheal diseases in many large field trials over a period of over 4 decades[1–3] and has generally been found effective. Nevertheless, the protective mechanism of zinc has remained elusive. For example, most of the articles on zinc and enteric pathogens emphasize the essential nature of this metal and imply that zinc would enhance enhance the virulence of the pathogen[4, 5] rather than help the host. It is often suggested that zinc acts via the immune system, but actual studies on zinc and immune responses are more nuanced and show that zinc can impair as well as enhance immune functions[7–10]. Instead of invoking zinc effects on immunity, we and others have shown that zinc can have pathogen-specific protective effects by acting directly on enteric bacteria including enteropathogenic E. coli (EPEC), Shiga-toxigenic E. coli (STEC), and enteroaggregative E. coli (EAEC)[11–13]. Recently, Mukhopadhyay and Linstedt reported that manganese could block the intracellular trafficking of Shiga toxin 1 (Stx1) and thus inhibit its ability to kill susceptible host cells. This prompted us to reexamine the effects of zinc on host cells and to compare the effects of zinc with that of other divalent metals, including manganese.
STEC includes older names and subsets including enterohemorrhagic E. coli, EHEC, and Verotoxigenic E. coli, VTEC. STEC is the main cause of episodic “E. coli outbreaks” which are usually food-borne and often attract a great deal of attention in the news media[15–17]. As the name implies, these strains produce potent cytotoxins such as Stx1 or Stx2, or both. Absorption of Stx from the gastrointestinal tract can lead to severe extra-intestinal effects, including kidney failure, brain damage, and death. Antibiotics often make STEC infections worse by virtue of their ability to induce Stx production[18, 19] and so are considered contraindicated in STEC infection. The severe sequelae of STEC infection has prompted many to seek additional treatments, sometimes by heroic measures that might rescue patients from the throes of full-blown disease, such as hemolytic-uremic syndrome (HUS)[20, 21]. In contrast, we thought it would make more sense to intervene earlier in the course of STEC infection and prevent STEC infections from progressing to severe disease. Safe and inexpensive measures such as supplementation with oral zinc or other metals therefore seemed attractive as options. In contrast to our previous studies emphasizing the effects of zinc and other metals on the pathogenic bacteria, in this study we began by comparing zinc and other metals for protective effects on host epithelial cells, using T84 colonic cells grown as polarized monolayers. We found that zinc increased the trans-epithelial electrical resistance (TER) of the T84 cell monolayers; TER serves as a measure of epithelial integrity and of the barrier function provided by tight junctions. Zinc also protected monolayers from damage induced by hydrogen peroxide, an oxidant host defense that is released in response to EPEC and STEC infection[22, 23]. We also examined if zinc and other metals had any effect of the translocation of Stx across T84 monolayers and found that it reduced toxin translocation as well. We also reexamined the ability of zinc to inhibit Stx production from STEC bacteria and correlated it with zinc’s ability to block the onset of the SOS bacterial stress response, as measured by recA expression, an early and quantifiable marker of the SOS response. While other metals occasionally mimicked zinc’s effects in one particular attribute or another, zinc was unique in its ability to simultaneously exert protective effects on host tissues while also inhibiting multiple bacterial pathways associated with STEC virulence such as the recA/SOS response, EHEC secreted proteins (Esps), the adhesins intimin and Tir, and Stx production. No other metal tested showed the same broad combination of beneficial effects as did zinc.
Bacterial strains used
Bacterial strains used are listed in Table 1. Bacteria were grown overnight in LB broth at 37°C with 300 rpm shaking, then subcultured into the medium for the expression studies, usually DMEM medium or minimal medium. In this report, when bacteria were subcultured in “DMEM” this refers to DMEM/F12 medium supplemented with 18 mM NaHCO3 and 25 mM HEPES, pH 7.4, but without serum or antibiotics.
Assays using T84 cells grown in polarized monolayers in Transwell inserts
T84 cells were grown to confluency over 7 to 10 days on 12 mm Transwell inserts (Corning Life Sciences, Lowell, MA) in T84 medium with 8% fetal bovine serum and antibiotics as described. The Transwells were of 0.4 μm pore size polycarbonate plastic, and were not coated with collagen or other proteins. Trans-epithelial electrical resistance (TER) was measured using an Evom2 meter (World Precision Instruments, Tampa, FL) and the STX2 chopstick electrode. (It is mere coincidence that the electrode has a name similar to the toxin we were studying.) We adjusted the concentration of hydrogen peroxide used to damage the monolayers based on the TER at the start of the experiment: 2 mM H2O2 was used for monolayers with resistances of 1000–1500 Ω, and 3 mM H2O2 for monolayers with resistances above 1500 Ω. TER values are reported in ohms (Ω). To obtain values in Ω · cm2, one would multiply by the area (1.12 cm2). For monolayer experiments, we removed serum-containing medium and performed the experiments in serum-free medium. Delta TER (ΔTER) is defined as the TERfinal – TERinitial; TER and Stx translocation measurements were done in quadruplicate wells and are shown as means ± SD.
Stx toxin translocation assay
We measured translocation of Stx2 from the upper chamber to lower chamber in T84 cells grown in Transwell inserts (apical-to-basolateral) as described by Acheson et al.. T84 cells are insensitive to the toxic effects of Stx, at least in part due to low or absent expression of the Gb3 glycolipid receptors for Stx1 and Stx2; intestinal epithelia in humans and other mammals also show nil expression of Gb3. As a source of Stx2 we used crude supernatants of STEC strain Popeye-1, subjected to sterile filtration, and containing 1 to 1.5 μg/mL of Stx2. Crude supernatant was used because other soluble factors present in STEC supernatants, including EHEC secreted protein P (EspP) increase the ability of Stx to translocate across monolayers by the trans-cellular route[29, 30]. This crude supernatant would be expected to contain Stx2c as well as Stx2. Stx supernatants were diluted to a final concentration of Stx2 in the upper chamber of between 50,000 to 100,000 pg/mL in various experiments done over several months. Stx2 addition was delayed until 2 h after the oxidant in order to avoid denaturing the Stx by oxidation. Medium from the lower chambers was collected at various times and Stx2 measured by enzyme immunoassay (EIA) as described using the Premier EHEC toxin EIA kit (Meridian Biosciences, Cincinnati, OH). Purified Shiga toxin 2 toxoid was a kind gift of Dr. Alison Weiss, Univ. of Cincinnati, and was used to create standard curves to allow better quantitation. To provide context, in monolayers damaged with 3 mM H2O2, the amount of Stx2 translocated across the monolayer at 24 h averaged 7.0 ± 4.8% of the amount originally added. Hypoxanthine + XO triggered a similar amount of Stx2 translocation: 8.5 ± 3.0% at 24 h (mean ± SD of 5 experiments).
Miller assay for expression of β-galactosidase in bacterial reporter strains
Strain JLM281, the reporter strain containing the recA-lacZ construct was used to measure recA expression in response to inducing antibiotics, zinc and other metals. We used a version of the Miller assay adapted to 96 well plates for higher throughput. However, we used 0.1% hexadecyltrimethylammonium bromide (HTA-Br) detergent alone, without chloroform or sodium dodecyl sulfate (SDS), to permeabilize the bacteria. The buffers used are described in a Open WetWare website at http://openwetware.org/wiki/Beta-Galactosidase_Assay_%28A_better_Miller%29.
Briefly, we subcultured strain JLM281 at a dilution of 1:100 from an overnight culture in DMEM into a 96 well plate containing minimal medium, 150 μl per well, on a Bioshake iQ thermal mixer (Quantifoil Instruments GmbH, Jena, Germany) at 37°C with mixing at 1200 rpm. We used DMEM for these expression experiments because induction of recA, LEE4, and LEE5 were higher in DMEM than in LB broth. The 96 well plate was sealed with gas-permeable plate sealing film to prevent evaporation during the growth phase. At 4 h when the cultures reached an OD600 in the 0.2 to 0.3 range, 20 μl of bacterial culture was transferred to the wells of a a second 96 well plate containing 80 μl of permeabilization buffer and allowed to permeabilize for at least 10 min at room temperature. The β-galactosidase reaction was initiated by transferring 25 μl of permeabilized bacteria into a third 96 well plate containing 150 μl of substrate solution with 1 g/L o-nitrophenyl-β-galactoside (ONPG). The enzyme reaction plate was incubated at 30°C for 30 min, and then A420 was measured on the 96 well plate reader. We usually omitted the addition of the Na2CO3 stop solution. Miller units were calculated using the simplified equation:
Agar overlay assay for bacteriophage plaques by modified spot assay
We used wild-type STEC strains as the source of bacteriophage for these experiments. STEC bacteria were subcultured at a dilution of 1:100 into antibiotic-free DMEM medium from an overnight culture. After 1 h of growth at 37°C with 300 rpm shaking, additions such as ciprofloxacin or zinc were made and the tubes returned to the shaker incubator for 5 h total. The STEC suspension was clarified by centrifugation, then subjected to sterile filtration using syringe-tip filters. The STEC filtrate was diluted 1:10 in DMEM medium, then serial 2-fold dilutions were made to yield dilutions of 1:20, 1: 40, 1: 80 and so on. The recipient strain, E. coli MG1655, was subcultured at 1: 50 from overnight and grown in LB broth for 3 hours. Soft LB agar was prepared using LB broth supplemented with 0.5% agar and 0.5 mM MgSO4. The soft agar was melted by microwave heating, and kept warm at 45°C on a heater block. The MG1655 culture was diluted 1: 10 into the soft agar and 5 ml of the bacteria-containing agar was overlaid on top of the agar of regular LB agar plate and allowed to solidify. Then 3 μl aliquots of the diluted STEC filtrates were spotted on top of the agar overlay. Plaques were visualized after 16 h of additional incubation at 37°C. Any faint zone of clearing was counted as a plaque. The highest dilution of STEC filtrate that produced a plaque was recorded as the plaque titer.
Rabbit infection experiments
No new rabbit infection experiments were performed for this study. We used photographs from the archives of our previous animal experiments to create the illustration in final figure. Nevertheless, all of our past and ongoing animal work has been scrutinized and approved by the animal care committee (IACUC) of the University at Buffalo.
Data analysis and statistics
Error bars shown on graphs and in Tables are standard deviations. Statistical signficance was tested by ANOVA using the Tukey-Kramer post-test for multiple comparisons.
We recently reported that the xanthine oxidase (XO) enzyme pathway is activated in response to EPEC and STEC infection. Infection with these pathogens triggers a release of nucleotides and nucleosides into the gut lumen, and XO itself is also released into the lumen of the intestine as a result of damage inflicted by these pathogens. XO catalyzes the conversion of hypoxanthine to xanthine and xanthine to uric acid, with both steps creating one molecule of hydrogen peroxide. As previously reported by Wagner for oxidant molecules generated from neutrophils, XO-generated H2O2 increases the production of Stx from STEC strains. Since H2O2 is known to be able to damage intestinal epithelia[32, 33], we thought this would be a relevant model to test whether zinc or other metals could protect against oxidant damage, since zinc has been reported to reported to help restore intestinal barrier function following other insults. We used T84 cells grown to confluency in polarized monolayers in Transwell inserts as previously reported. We measured trans-epithelial electrical resistance (TER), an index of intestinal barrier function, as well as H2O2-induced translocation of Stx2 from apical to basolateral chambers.
Figure 1 shows the effects of H2O2 on TER and Stx2 translocation. H2O2 damages tight junctions and increases permeability via the paracellular pathway. Figure 1A shows that H2O2 has concentration-dependent and time-dependent effects on TER in the T84 monolayers. 1 mM H2O2 paradoxically increased TER slightly, but 2 mM H2O2 caused a moderate drop in TER. H2O2 at 3 mM and above damaged the monolayers severely, with TER falling to ~100 Ω, which is equivalent to that of the Transwell filters alone without any cells. Figure 1B shows that H2O2 also had a concentration dependent effect on Stx2 translocation, with Stx2 translocation detectable at H2O2 concentrations of 3 mM or higher. The inset in Figure 1B shows that H2O2 was also able to trigger a flux of fluorescein-labeled dextran-4000 across the monolayer, and that the monolayer damage could be prevented by the addition of catalase. Figure 1C shows that zinc could increase the TER in T84 cells not subjected to hydrogen peroxide or any other noxious stimulus, and Figure 1D shows that zinc could protect against the drop in TER induced by treatment with 2% dimethylsulfoxide (DMSO), at least at intermediate concentrations. Zinc acetate seemed to reduce the drop in TER (∆ TER) induced by 3 mM H2O2, although this protective effect did not reach statistical significance (Figure 1E). Figure 1F shows, however, that intermediate concentrations of zinc (0.1 to 0.3 mM) did significantly reduce Stx2 translocation across the T84 monolayers. At zinc concentrations of 0.4 mM and higher, however, the protective effect was lost, resulting in a U-shaped curve in Figure 1F (data not shown for concentrations greater than 0.4 mM). The U shape in Figure 1F seemed to mirror the arch shape of the curves in Figure 1D and E, and suggested that zinc might have interesting protective effects against insults to the intestinal epithelium.
In Figure 1 the hydrogen peroxide was added once at fairly high concentrations, but in an actual infection the hydrogen peroxide (and other oxidants, such as superoxide and sodium hypochlorite) is generated gradually from enzymatic conversion of substrates over many hours. Therefore we repeated experiments similar to those shown in Figure 1, but instead using H2O2 we added hypoxanthine plus XO. Figure 2A shows that, in the presence of XO, hypoxanthine has a concentration-dependent effect on ∆ TER. Adding 100 μM hypoxanthine actually increased TER compared to vehicle control, with higher concentrations of hypoxanthine inducing a progressive fall in TER. The increase in TER observed in Figure 2A at 100 μM hypoxanthine was reminiscent of the small increase in TER seen with 1 mM H2O2 in Figure 1A (top curve). Figure 2, Panels B, shows that the effect of zinc on T84 cell monolayers was additive with the known protective effects of 5 mM sodium butyrate on colon cell monolayers. The concentration of butyrate we used is well within the concentrations known to occur in the lumen of the lower gastrointestinal tract. Figure 2C shows that zinc at 0.1 to 0.5 mM significantly protected cells from the drop in TER inflicted by XO + 400 μM hypoxanthine. Likewise, Figure 2D shows that 0.1 to 0.3 mM zinc, but not 0.4 mM zinc, reduced Stx2 translocation triggered by XO + 400 µM hypoxanthine. Thus, while Figure 2C did not show the arch shape seen in Figure 1C, Figure 2D does have the “U” shape similar to that seen in Figure 1D with hydrogen peroxide as the injuring oxidant. In monolayers treated with hypoxanthine + XO, the amount of Stx2 that translocated across the monolayer in 24 h was 8.5 ± 3.0% (mean ± SD of 5 experiments) of the total amount added to the upper chamber. Figures 1 and2 showed that zinc acetate could protect against oxidant-induced drop in TER, a measure of intestinal barrier function, and inhibit the translocation of Stx2 across T84 cell monolayers as well.
In Figure 3 we examined the effects of other metals on TER and Stx2 translocation. We focused on the transition metals nearest to zinc in atomic number, including manganese, iron, nickel, and copper. Figure 3A shows the effects of two of these metals on TER, while Panels B-D show the effects on Stx2 translocation. Figure 3A shows that in contrast to zinc (top curve), FeSO4 and MnCl2 had no protective effect against the drop in TER triggered by XO + hypoxanthine. Copper (as CuSO4) also failed to protect against the drop in TER (data not shown). When Stx2 translocation was measured, FeSO4 seemed to slightly enhance Stx2 translocation triggered by H2O2 (Figure 3B), but this did not reach statistical significance. Nevertheless, iron has been shown to be able to potentiate oxidant-induced damage, and this has often been attributed to iron’s ability to catalyze the Fenton reaction, in which H2O2 is split into 2 molecules of hydroxyl radical (HO•). Figure 3C shows that manganese (as MnCl2) failed to protect against Stx22 translocation, and at 0.5 mM manganese significantly increased the amount of Stx2 crossing the monolayers. Notably, 0.5 mM was the effective concentration of manganese used by Mukhopadhyay and Linstedt in their study of Stx1 trafficking in HeLa cells. Figure 3D shows that CuSO4, like zinc, significantly reduced Stx2 translocation. This was a surprise because of the lack of protection by CuSO4 on TER. Nickel chloride also had no protective effect on TER and none on Stx2 translocation at 0.1 to 0.5 mM (data not shown).
To summarize Figures 1,2 and3, zinc increased the TER in undamaged cells, and protected intestinal monolayers against the drop in TER induced by DMSO, by hydrogen peroxide, and that induced by XO plus hypoxanthine. Zinc also protected against oxidant-induced translocation of Stx2 across the monolayers at 0.1 to 0.3 mM concentration. These protective effects of zinc are attributable to actions of zinc on the host tissues, not on bacteria. None of the four other metals tested (iron, manganese, copper, or nickel) protected against oxidant-induced decrease in TER, but copper was still able to reduce Stx2 translocation across monolayers (Figure 3D). Our results did not support the idea, advanced by Mukhopadhyay and Linstedt, that manganese was the metal with the greatest promise for protection against STEC infection in the clinical setting. Zinc still seemed to be a candidate for such studies, but to address this more fully we compared zinc and other metals for their ability to block bacterial signaling and stress-response pathways associated with virulence.
Stx production and release in STEC bacteria is strongly regulated by the SOS stress response system in E. coli[18, 38]. In contrast, Stx production is quite insensitive to commonly mentioned signaling pathways such as quorum sensing, and to transcription factors such as the LEE-encoded regulator (Ler) and Plasmid-encoded regulator (Per)[25, 39–41]. This is not surprising since stx1 and stx2 are encoded on phages similar to phage lambda, and these phage genes are strongly activated by the DNA damage triggered by certain antibiotics, hydrogen peroxide[22, 42], or ultraviolet light. An early, reliable, and quantifiable marker of the SOS response is the expression of recA[43, 44]. We hypothesized that zinc’s ability to inhibit Stx production arises from its ability to inhibit the SOS response and recA. To test this, we measured recA expression using a recA-lacZ reporter gene construct using the Miller assay method and compared those results with metals ability to inhibit Stx production.
Figure 4A shows that zinc inhibits ciprofloxacin-induced Stx2 production strongly and in a dose-dependent manner. In contrast, MnCl2 had no such ability to inhibit either ciprofloxacin-induced Stx2 production (Figure 4B) or basal (non-antibiotic treated) Stx release. Figure 4C shows that recA expression increased in reporter strain JLM281 when hypoxanthine is added in the presence of the enzyme XO, but not in the absence of XO. Hydrogen peroxide itself showed a recA activation curve with a similar shape (Figure 4D). Zinc acetate inhibited ciprofloxacin-induced recA expression (Figure 4E) as well as hydrogen-peroxide induced recA expression (data not shown). Zinc acetate was more efficacious and more potent in inhibition of ciprofloxacin-induced recA expression that MnCl2 or NiCl2 (Figure 4F) and more than FeSO4, CuSO4, or gallium nitrate (Figure 4G). Gallium was tested because of its position next to zinc on the Periodic Table and because others had reported it had anti-virulence activity. Figure 4H shows that zinc acetate was more potent than zinc oxide nanoparticles, CoCl2, or bismuth subcitrate in inhibition of recA induced by ciprofloxacin. Bismuth was tested because of its long use as a treatment for infectious diarrhea[46, 47], and zinc oxide nanoparticles were reported to have activity against Campylobacter jejuni. In summary, zinc acetate was more potent and more effective in inhibiting ciprofloxacin-induced recA than any other metal shown in Figure 4. Zinc also blocked recA induced by mitomycin C (data not shown). As controls, zinc did not block the induction of other genes, including a β-lactamase-lacZ reporter gene (see final figure below), or the ability of isopropyl-thio-galactose (IPTG) to induce beta-galactosidase in wild-type E. coli strains (data not shown). We did not test metals such as cadmium, mercury, or lead, because we are interested in the translational use of these findings and felt those metals were too toxic to be considered for use in humans or animals.
Since our finding that zinc-mediated inhibition of recA expression had not been previously reported, we tested whether zinc was actually blocking the entire bacterial SOS response, or merely preventing recA expression in an artefactual way. A reliable “downstream” marker of the SOS stress response in E. coli is a marked elongation of the bacterial cells, sometimes called filamentation, which is due to inhibition of the fission ring formed by FtsZ. We tested whether zinc inhibited antibiotic-induced elongation of bacteria. Additional file1: Figure S1 shows that zinc reversed ciprofloxacin-induced bacterial elongation in EPEC E2348/69 and in STEC strain Popeye-1, as well as mitomycin C-induced elongation in Popeye-1. In contrast to zinc, manganese and nickel did not have any effect on antibiotic-induced elongation (Additional file1: Figure S1B and 1C). Zinc also blocked the production of infectious bacteriophage from STEC strains Popeye-1, EDL933, and TSA14, as assessed by phage plaque assays on laboratory E. coli strain MG1655 (Figure 5 and Table 2). Therefore we conclude that zinc blocks all the core features of the SOS response, and not merely recA induction.
Stx is an important virulence factor in STEC, but it is not the only one. Therefore, we also tested whether operons in the locus for enterocyte effacement (LEE) were activated by oxidant stress, and if so, whether, they were susceptible to inhibition by zinc. We used LEE4-lacZ and LEE5-lacZ reporter strains; LEE4 encodes the EPEC and EHEC secreted proteins (Esps), and LEE5 encodes the critical adhesins Tir and intimin, and the CesT chaperone. Figure 6 shows that, in the presence of XO, hypoxanthine substrate does modestly activate expression of both LEE4 (Figure 6A) and LEE5 (Figure 6B). Figure 6C shows that H2O2 also induced LEE5 expression in a manner similar to that triggered hypoxanthine plus XO, and as previously shown for ciprofloxacin. Figure 6D shows that zinc acetate inhibited LEE4 expression, but unfortunately manganese chloride showed no such ability. Figure 6 shows first that LEE operons may be up-regulated by oxidant stress, and second that the virulence-inhibiting abilities of zinc extend to factors other than Stx including critical adhesins and Type III secreted proteins encoded in the LEE. While Figures 1,2 and3 focused on the protective effects of zinc and other metals on intestinal cells, Figures 4,5 and6 extend our previous understanding of zinc’s direct effects on bacteria[11, 12], showing zinc’s ability to inhibit the SOS response as measured by recA expression (Figure 4), a property not matched by any other metal tested. The good correlation between zinc’s inhibition of recA expression (Figure 4), filamentation (Additional file1: Figure S1), phage production, and zinc’s inhibition of Stx toxin protein (Figure 4A) and stx RNA suggests that zinc’s ability to block recA activation is an important part of the mechanism of action of this metal in STEC and EPEC infection.
Discussion and conclusions
Our understanding of the roles of divalent metals as regulators of bacterial pathogenesis has lagged behind that of other molecules such as quorum sensing auto-inducers and transcriptional regulators such as H-NS and Ler. Most of the work on transporters and metabolism of zinc and other metals has been done with non-pathogenic laboratory strains of E. coli[50–52], which makes the results difficult to extrapolate to strains which are professional intestinal or extra-intestinal pathogens. For example, STEC expresses several different metal uptake and zinc export genes not present in laboratory E. coli strains[4, 5, 53, 54] so STEC’s response to bioactive metals often differs from non-pathogenic E. coli. In addition, the specialized Type III secretion system (and Type VI secretion system in EAEC) used to deliver effectors into host cells may serve as an “Achilles’ heel” in these pathotypes because the membrane secretion machinery causes them to become hypersusceptible to some stressful stimuli such as the envelope stress response[27, 56]. Furthermore, many of the reports on zinc in enteric bacteria only focus on the essential nature of this metal for the pathogen[4, 57], without consideration of how zinc might also benefit the host. In addition, many reports do not distinguish between the growth-and-fitness promoting effects of zinc on pathogens at the low concentrations usually present (1 to 50 μM) versus the higher, stress-inducing concentrations of zinc that can occur during zinc supplementation (0.1 to 0.4 mM). In general, it appears that host cells are better able to survive--- and thrive--- in the presence of these higher zinc concentrations that are deleterious to E.coli and other enteric bacteria ([58, 59], and Figures 1,2 and3 of this study). Moreover, studies that have actually tested zinc for infection outcomes using cultured cell models or animal models have generally shown that zinc benefits the host more than the pathogen, resulting in a reduction in severity of disease[11, 13, 48, 60]. Indeed, Botella et al. recently showed that zinc is mobilized in macrophages and concentrated in phagosomes as part of the host defense against Mycobacterium tuberculosis. This is relevant to the gut because zinc is also concentrated in the secretory granules of Paneth cells[62, 63], specialized cells in the intestinal crypts involved in antimicrobial defenses.
The discovery that zinc specifically inhibits virulence factor expression by some pathogens and not others has led us to emphasize that zinc’s effects may be pathogen-specific. We may have to temper that emphasis, however, because Figures 1 and2 of this study show zinc may strengthen the intestinal epithelial barrier against oxidant damage and this might extend zinc’s protection to organisms that are not specifically affected by zinc. Zinc may have mild protective effects against multiple diarrheal pathogens via its effects on enterocytes, and then also have additional protective activity against specific pathogens such as EPEC, STEC, EAEC, and Campylobacter.
Mukhopadhyay and Linstedt reported that manganese was able to block the intracellular trafficking of Stx1 through the Golgi apparatus of Stx-susceptible HeLa cells engineered to overexpress the glycolipid Gb3; by doing so MnCl2 appeared to block the toxic effects of Stx1. Hope that manganese could be used as a treatment for STEC infection diminished, however, when Gaston et al. and additional work by Mukhopadhyay et al. showed that the protective effects of manganese did not extend to Stx2[65, 66]. Gaston and colleagues also showed that manganese was more toxic, both in cultured cells and in mice, than was reported by Mukhopadhyay and Linstedt. Our results show that manganese, unlike zinc, shows no protective effects on epithelial barrier function (measured as TER) or on Stx2 translocation across intestinal monolayers (Figure 3). Manganese did not inhibit ciprofloxacin-stimulated Stx2 production from STEC bacteria, unlike zinc (Figure 3A and B) and copper, and did not have any effect on recA expression (Figure 4F) or the SOS- induced bacterial elongation response (Additional file1: Figure S1). Manganese has been shown to up-regulate expression of the Esps in STEC and to increase basal Stx toxin production, so manganese has real potential to cause more harm than good in STEC infection. In addition, the neurotoxicity of manganese, which is worse in children and young animals, could exacerbate the Stx-induced encephalopathy that can accompany severe cases of STEC infection. Based on the literature mentioned and our results here, it appears that zinc is more likely to have therapeutic effects against STEC than manganese.
Copper also appears to have the ability to inhibit Stx production in an recA-independent fashion (Figure 4G and Ref.), which is plausible given that recA-independent pathways are known to regulate Stx. Copper, like zinc, also was able to block Stx2 translocation across intestinal monolayers (Figure 3F). Although copper is more toxic to humans than is zinc (based on the inverse ratios of the tolerable Upper Limits of these metals from the Food and Nutrition Board of the Institute of Medicine, available at https://fnic.nal.usda.gov/dietary-guidance/dietary-reference-intakes/dri-tables it is possible that copper might be combined with zinc to obtain additive effects via recA- dependent and recA-independent effects on STEC bacteria.
Mukhopadhyay and Linstedt focused their attention narrowly on the Gb3-expressing cells that are the target of Stx, while we believe that it may be more helpful to consider multiple steps in the natural history of STEC infection where interventions might help (Figure 7). Figure 7 and Additional file2: Table S1 show that there are at least three separate phases at which zinc, other metals, or oral drugs might affect STEC after the pathogen enters the body. In the first phase, in the intestinal lumen, metals or other drugs might be able to prevent the expression of adhesins, virulence factors, and Stx (Figure 7, top portion). If the treatment was delayed, STEC infection was established, and Stx was produced, zinc or other interventions might still be able to reduce the amount of Stx which crosses the intestinal barrier (Figure 7, Phase 2). Previous literature on oxidant-mediated damage to intestinal epithelium has shown that tight junctions are the target of hydrogen peroxide[35, 70, 71] as well as the damage induced by nutrient deprivation[34, 72]. Tight junctions are known to be regulated by extracellular divalent metals, especially calcium and zinc[34, 73–77]. Based on previous research, therefore, we believe the effect of zinc on Stx translocation seen in Figures 1 and2, and in Phase 2 of Figure 7, is likely due do its protective effect on the paracellular pathway rather than the transcellular/macropinocytosis pathway for Stx translocation that has also been well described[29, 30].
Additional file2: Table S1 summarizes the effects of zinc and four other metals in STEC and EPEC infection, based on results reported in this study as well as previous work by other investigators and our own laboratory. As can be seen from Additional file2: Table S1, no other metal quite matches zinc in the wide number of different beneficial effects it exerts on host cells and inhibitory effects it exerts on the pathogen, although copper also shows some beneficial effects. In contrast, manganese, iron, and nickel all have the potential to worsen one or more aspects of STEC’s interactions with host cell (Additional file2: Table S1).
EPEC adherence to host intestinal cells is heaviest in the ileum and cecum, and STEC adheres most strongly in the cecum and large intestine. Therefore, drugs or metals with limited absorption in the upper gastrointestinal tract would be ideal candidates for intervening at Phases 1 or 2 of Figure 7, because they would have to attain sufficient concentrations in the lumen of the distal gut; zinc salts fall into this category.
In the 3rd phase of Figure 7, Stx which has crossed the epithelial barrier binds to and begins to kill susceptible host cells, especially endothelial cells. Figure 7, lower portion, shows a higher power view of an intestinal blood vessel which has been affected by Stx2, showing adherence of polymorphonuclear leukocytes on the lumen of the endothelium (green arrows), as well as leukocytes which have been recruited into the wall of the vessel itself (blue arrow, showing a true vasculitis). When a similar process occurs in blood vessels elsewhere severe extra-intestinal complications can ensue. It appears that more research will be needed before we can declare we have drugs capable of blocking the 3rd Phase of Stx action[14, 65], and Additional file2: Table S1.
Figure 7 illustrates possible points at which metals might act after STEC enters the intestinal tract of the host. Metals which prove too toxic to use in vivo in humans might still find use, however, in the “pre-ingestion” phase of STEC, i.e., in agricultural practices, during germination of sprouts, or during food processing to limit STEC adherence to fresh foods or block virulence. Indeed, copper has already attracted attention for its antimicrobial properties in this regard[78, 79]. Divalent metals deserve additional research attention as inhibitors of bacterial virulence and enhancers of host defenses.
Bhutta ZA, Bird SM, Black RE, Brown KH, Gardner JM, Hidayat A, Khatun F, Martorell R, Ninh NX, Penny ME, Rosado JL, Roy SK, Ruel M, Sazawal S, Shankar A: Therapeutic effects of oral zinc in acute and persistent diarrhea in children in developing countries: pooled analysis of randomized controlled trials. Am J Clin Nutr. 2000, 72: 1516-1522.
Sazawal S, Black R, Bhan M, Bhandari N, Sinha A, Jalla S: Zinc supplementation in young children with acute diarrhea in India. N Engl J Med. 1995, 333: 839-844.
Patel A, Mamtani M, Dibley MJ, Badhoniya N, Kulkarni H: Therapeutic value of zinc supplementation in acute and persistent diarrhea: a systematic review. PLoS One. 2010, 5: e10386-
Gabbianelli R, Scotti R, Ammendola S, Petrarca P, Nicolini L, Battistoni A: Role of ZnuABC and ZinT in Escherichia coli O157:H7 zinc acquisition and interaction with epithelial cells. BMC Microbiol. 2011, 11: 36-
Porcheron G, Garenaux A, Proulx J, Sabri M, Dozois CM: Iron, copper, zinc, and manganese transport and regulation in pathogenic Enterobacteria: correlations between strains, site of infection and the relative importance of the different metal transport systems for virulence. Front Cell Infect Microbiol. 2013, 3: 90-
Prasad AS: Zinc: mechanisms of host defense. J Nutr. 2007, 137: 1345-1349.
Karlsen TH, Sommerfelt H, Klomstad S, Andersen PK, Strand TA, Ulvik RJ, Åhrén C, Grewal HMS: Intestinal and systemic immune responses to an oral cholera toxoid B subunit whole-cell vaccine administered during zinc supplementation. Infect Immun. 2003, 71: 3909-3913.
Wellinghausen N, Martin M, Rink L: Zinc inhibits interleukin-1-dependent T cell stimulation. Eur J Immunol. 1997, 27: 2529-2535.
Schlesinger L, Arevalo M, Arredondo S, Lonnerdal B, Stekel A: Zinc supplementation impairs monocyte function. Acta Paediatr. 1993, 82: 734-738.
Provinciali M, Montenovo A, Stefano G, Colombo M, Daghetta L, Cairati M, Veroni C, Cassino R, Torre FD, Fabris N: Effect of zinc or zinc plus arginine supplementation on antibody titre and lymphocyte subsets after influenza vaccination in elderly subjects: a randomized controlled trial. Age Ageing. 1998, 27: 715-722.
Crane J, Naeher T, Shulgina I, Zhu C, Boedeker E: Effect of zinc in enteropathogenic Escherichia coli infection. Infect Immun. 2007, 75: 5974-5984.
Crane JK, Byrd IW, Boedeker EC: Virulence inhibition by zinc in shiga-toxigenic escherichia coli. Infect Immun. 2011, 79: 1696-
Medeiros P, Bolick D, Roche J, Noronha F, Pinheiro C, Kolling G, Guerrant R: The micronutrient zinc inhibits EAEC strain 042 adherence, biofilm formation, virulence gene expression and epithelial cytokine responses benefiting the infected host. Virulence. 2013, 4: 624-633.
Mukhopadhyay S, Linstedt AD: Manganese blocks intracellular trafficking of shiga toxin and protects against shiga toxicosis. Science. 2012, 335: 332-335.
Frank C, Werber D, Cramer JP, Askar M, Faber M, Heiden M, Bernard H, Fruth A, Prager R, Spode A, Wadl M, Zoufaly A, Jordan S, Kemper MJ, Follin P, Mueller L, King LA, Rosner B, Buchholz U, Stark K, Krause G: Epidemic profile of shiga-toxin-producing escherichia coli O104:H4 outbreak in Germany. N Eng J Med. 2011, 365: 1771-1780.
Buchholz U, Bernard H, Werber D, Bohmer MM, Remschmidt C, Wilking H, Delere Y, an der Heiden M, Adlhoch C, Dreesman J, Ehlers J, Ethelberg S, Faber M, Frank C, Fricke G, Greiner M, Hohle M, Ivarsson S, Jark U, Kirchner M, Koch J, Krause G, Luber P, Rosner B, Stark K, Kuhne M: German outbreak of Escherichia coli O104:H4 associated with sprouts. N Engl J Med. 2011, 365: 1763-1770.
Gould LH, Mody RK, Ong KL, Clogher P, Cronquist AB, Garman KN, Lathrop S, Medus C, Spina NL, Webb TH, White PL, Wymore K, Gierke RE, Mahon BE, Griffin PM: Increased recognition of non-O157 Shiga toxin-producing Escherichia coli infections in the United States during 2000–2010: epidemiologic features and comparison with E. coli O157 infections. Foodborne Pathog Dis. 2013, 10: 453-460.
Kimmitt P, Harwood C, Barer M: Toxin gene expression by Shiga toxin-producing Escherichia coli: the role of antibiotics and the bacterial SOS response. Emerg Infect Dis. 2000, 6: 458-466.
Zhang X, McDaniel A, Wolf L, Keusch G, Waldor M, Acheson D: Quinolone antibiotics induce Shiga toxin-encoding bacteriophages, toxin production, and death in mice. J Infect Dis. 2000, 181: 664-670.
Colic E, Dieperink H, Titlestad K, Tepel M: Management of an acute outbreak of diarrhoea-associated haemolytic uraemic syndrome with early plasma exchange in adults from southern Denmark: an observational study. Lancet. 2011, 378: 1089-1093.
Andreoli SP, Trachtman H, Acheson DWK, Siegler RL, Obrig TG: Hemolytic uremic syndrome: epidemiology, pathophysiology, and therapy. Pediatr Nephrol. 2002, 17: 293-298.
Wagner PL, Acheson DWK, Waldor MK: Human neutrophils and their products induce shiga toxin production by enterohemorrhagic escherichia coli. Infect Immun. 2001, 69: 1934-1937.
Crane JK, Naeher TM, Broome JE, Boedeker EC: Role of host xanthine oxidase in infection Due to enteropathogenic and shiga-toxigenic escherichia coli. Infect Immun. 2013, 81: 1129-1139.
Mellies JL, Haack KR, Galligan DC: SOS regulation of the type III secretion system of enteropathogenic Escherichia coli. J Bacteriol. 2007, 189: 2863-
Mellies JL, Elliott SJ, Sperandio V, Donnenberg MS, Kaper JB: The Per regulon of enteropathogenic Escherichia coli : identification of a regulatory cascade and a novel transcriptional activator, the locus of enterocyte effacement (LEE)-encoded regulator (Ler). Mol Microbiol. 1999, 33: 296-306.
Haack KR, Robinson CL, Miller KJ, Fowlkes JW, Mellies JL: Interaction of Ler at the LEE5 (tir) operon of enteropathogenic Escherichia coli. Infect Immun. 2003, 71: 384-392.
Mellies J, Thomas K, Turvey M, Evans N, Crane J, Boedeker EC, Benison G: Zinc-induced envelope stress diminishes type III secretion in enteropathogenic Escherichia coli. BMC Microbiol. 2012, 12: 123-
Acheson DWK, Moore R, De Breucker S, Lincicome L, Jacewicz M, Skutelsky E, Keusch GT: Translocation of Shiga toxin across polarized intestinal cells in tissue culture. Infect Immun. 1996, 64: 3294-3300.
In J, Lukyanenko V, Foulke-Abel J, Hubbard AL, Delannoy M, Hansen A-M, Kaper JB, Boisen N, Nataro JP, Zhu C: Serine protease EspP from enterohemorrhagic escherichia coli is sufficient to induce shiga toxin macropinocytosis in intestinal epithelium. PLoS One. 2013, 8: e69196-
Malyukova I, Murray KF, Zhu C, Boedeker E, Kane A, Patterson K, Peterson JR, Donowitz M, Kovbasnjuk O: Macropinocytosis in Shiga toxin 1 uptake by human intestinal epithelial cells and transcellular transcytosis. Am J Physiol. 2008, 296: G78-G92.
Griffith KL, Jr Wolf RE: Measuring beta-galactosidase activity in bacteria: cell growth, permeabilization, and enzyme assays in 96-well arrays. Biochem Biophys Res Commun. 2002, 290: 397-402.
Wang N, Wang G, Hao J, Ma J, Wang Y, Jiang X, Jiang H: Curcumin ameliorates hydrogen peroxide-induced epithelial barrier disruption by upregulating heme oxygenase-1 expression in human intestinal epithelial cells. Dig Dis Sci. 2012, 57: 1792-1801.
Yu W, Beaudry S, Negoro H, Boucher I, Tran M, Kong T, Denker BM: H2O2 activates G protein, α 12 to disrupt the junctional complex and enhance ischemia reperfusion injury. Proc Natl Acad Sci USA. 2012, 109: 6680-6685.
Rodriguez P, Darmon N, Chappuis P, Candalh C, Blaton MA, Bouchaud C, Heyman M: Intestinal paracellular permeability during malnutrition in guinea pigs: effect of high dietary zinc. Gut. 1996, 39: 416-422.
Jepson MA: Disruption of epithelial barrier function by H2O2: distinct responses of Caco-2 and Madin-Darby canine kidney (MDCK) strains. Cell Mol Biol (Noisy-le-Grand). 2003, 49: 101-112.
Peng L, He Z, Chen W, Holzman I, Lin J: Effects of butyrate on intestinal barrier function in a Caco-2 cell monolayer model of intestinal barrier. Pediatr Res. 2007, 61: 37-41.
Velazquez OC, Lederer HM, Rombeau JL: Butyrate and the colonocyte. Production, absorption, metabolism, and therapeutic implications. Adv Exp Med Biol. 1997, 427: 123-134.
Bielaszewska M, Idelevich EA, Zhang W, Bauwens A, Schaumburg F, Mellmann A, Peters G, Karch H: Effects of antibiotics on shiga toxin 2 production and bacteriophage induction by epidemic escherichia coli O104:H4 strain. Antimicrob Agents Chemother. 2012, 56: 3277-3282.
Spears K, Roe A, Gally D: A comparison of enteropathogenic and enterohaemorraghic Escherichia coli pathogenesis. FEMS Microbiol Lett. 2006, 255: 187-202.
Elliott S, Sperandio V, Giron J, Shin S, Mellies J, Wainwright L, Jutcheson S, McDaniel T, Kaper J: The locus of enterocyte effacement (LEE)-encoded regulator controls expression of both LEE- and non-LEE encoded virulence factors in enteropathogenic and enterohemorrhagic Escherichia coli. Infect Immun. 2000, 68: 6115-6126.
Sperandio V, Mellies JL, Nguyen W, Shin S, Kaper JB: Quorum sensing controls expression of the type III secretion gene transcription and protein secretion in enterohemorrhagic and enteropathogenic Escherichia coli. Proc Natl Acad Sci USA. 1999, 96: 15196-15201.
Łoś JM, Łoś M, Węgrzyn A, Węgrzyn G: Hydrogen peroxide-mediated induction of the Shiga toxin-converting lambdoid prophage ST2-8624 in Escherichia coli O157:H7. FEMS Immunol Med Microbiol. 2010, 58: 322-329.
Vareille M, de Sablet T, Hindré T, Martin C, Gobert A: Nitric oxide inhibits Shiga-toxin synthesis by enterohemorrhagic Escherichia coli. Proc Natl Acad Sci USA. 2007, 104: 10199-10204.
Fuchs S, Muhldorfer I, Donohue-Rolfe A, Kerenyi M, Emody L, Alexiev R, Nenkov P, Hacker J: Influence of RecA on in vivo virulence and Shiga toxin 2 production in Escherichia coli pathogens. Microb Pathog. 1999, 27: 13-23.
Kaneko Y, Thoendel M, Olakanmi O, Britigan B, Singh P: The transition metal gallium disrupts Pseudomonas aeruginosa iron metabolism and has antimicrobial and antibiofilm activity. J Clin Invest. 2007, 117: 877-888.
DuPont H, Sullivan P, Pickering L, Haynes G, Ackerman P: Symptomatic treatment of diarrhea with bismuth subsalicylate among students attending a Mexican university. Gastroenterology. 1977, 73: 715-718.
Johnson P, Ericsson C, DuPont H, Morgan D, Bitsura J, Wood L: Comparison of loperamide with bismuth subsalicylate for the treatment of acute travelers’ diarrhea. JAMA. 1986, 255: 757-760.
Xie Y, He Y, Irwin PL, Jin T, Shi X: Antibacterial activity and mechanism of action of zinc oxide nanoparticles against Campylobacter jejuni. Appl Environ Microbiol. 2011, 77: 2325-2331.
Mellies JL, Barron AMS, Carmona AM: Enteropathogenic and Enterohemorrhagic Escherichia coli Virulence Gene Regulation. Infect Immun. 2007, 75: 4199-4210.
Outten C, O’Halloran T: Femtomolar sensitivity of metalloregulatory proteins controlling zinc homeostasis. Science. 2001, 292: 2488-2491.
Outten CE, Outten FW, O’Halloran TV: DNA distortion mechanism for transcriptional activation by ZntR, a Zn(II)-responsive MerR homologue in escherichia coli. J Biol Chem. 1999, 274: 37517-37524.
Yamamoto K, Ishihama A: Transcriptional response of escherichia coli to external zinc. J Bacteriol. 2005, 187: 6333-6340.
Torres AG, Payne SM: Haem iron-transport system in enterohaemorrhagic Escherichia coli O157:H7. Mol Microbiol. 1997, 23: 825-833.
Lim J, Lee KM, Kim SH, Kim Y, Kim SH, Park W, Park S: YkgM and ZinT proteins are required for maintaining intracellular zinc concentration and producing curli in enterohemorrhagic Escherichia coli (EHEC) O157:H7 under zinc deficient conditions. Int J Food Microbiol. 2011, 149: 159-170.
Bower S, Rosenthal KS: The bacterial cell wall: the armor, artillery, and achilles heel. Infect Dis Clin Pract. 2006, 14: 309-317. 310.1097/1001.idc.0000240862.0000274564.0000240857
Vogt SL, Raivio TL: Just scratching the surface: an expanding view of the Cpx envelope stress response. FEMS Microbiol Lett. 2012, 326: 2-11.
Gielda LM, DiRita VJ: Zinc competition among the intestinal microbiota. MBio. 2012, 3: 1-7.
Bratz K, Golz G, Riedel C, Janczyk P, Nockler K, Alter T: Inhibitory effect of high-dosage zinc oxide dietary supplementation on Campylobacter coli excretion in weaned piglets. J Appl Microbiol. 2013, 115: 1194-1202.
Zhang P, Carlsson M, Schneider N, Duhamel G: Minimal prophylactic concentration of dietarry zinc compounds in a mouse model off swine dysentery. Anim Health Res Rev. 2001, 2: 67-74.
Roselli M, Finamore A, Garaguso I, Britti MS, Mengheri E: Zinc oxide protects cultured enterocytes from the damage induced by Escherichia coli. J Nutr. 2003, 133: 4077-4082.
Botella H, Peyron P, Levillain F, Poincloux R, Poquet Y, Brandli I, Wang C, Tailleux L, Tilleul S, Charrière GM, Waddell Simon J, Foti M, Lugo-Villarino G, Gao Q, Maridonneau-Parini I, Butcher Philip D, Castagnoli Paola R, Gicquel B, de Chastellier C, Neyrolles O: Mycobacterial P1-type ATPases mediate resistance to zinc poisoning in human macrophages. Cell Host Microbe. 2011, 10: 248-259.
Giblin LJ, Chang CJ, Bentley AF, Frederickson C, Lippard SJ, Frederickson CJ: Zinc-secreting paneth cells studied by ZP fluorescence. J Histochem Cytochem. 2006, 54: 311-316.
Dinsdale D: Ultrastructural localization of zinc and calcium within the granules of rat Paneth cells. J Histochem Cytochem. 1984, 32: 139-145.
Patel A, Dibley M, Mamtani M, Badhoniya N, Kulkarni H: Influence of zinc supplementation in acute diarrhea differs by the isolated organism. Int J Pediatr. 2010, 2010: 671587-
Gaston MA, Pellino CA, Weiss AA: Failure of manganese to protect from shiga toxin. PLoS One. 2013, 8: e69823-
Mukhopadhyay S, Redler B, Linstedt AD: Shiga toxin–binding site for host cell receptor GPP130 reveals unexpected divergence in toxin-trafficking mechanisms. Mol Biol Cell. 2013, 24: 2311-2318.
Beltrametti F, Kresse AU, Guzmán CA: Transcriptional regulation of the esp genes of enterohemorrhagic escherichia coli. J Bacteriol. 1999, 181: 3409-3418.
Moreno JA, Yeomans EC, Streifel KM, Brattin BL, Taylor RJ, Tjalkens RB: Age-dependent susceptibility to manganese-induced neurological dysfunction. Toxicol Sci. 2009, 112: 394-
Imamovic L, Muniesa M: Characterizing RecA-independent induction of shiga toxin2-encoding phages by EDTA treatment. PLoS One. 2012, 7: e32393-
Rao RK, Baker RD, Baker SS, Gupta A, Holycross M: Oxidant-induced disruption of intestinal epithelial barrier function: role of protein tyrosine phosphorylation. Am J Physiol. 1997, 273: G812-G823.
Perez LM, Milkiewicz P, Ahmed-Choudhury J, Elias E, Ochoa JE, Sanchez Pozzi EJ, Coleman R, Roma MG: Oxidative stress induces actin-cytoskeletal and tight-junctional alterations in hepatocytes by a Ca2+ -dependent, PKC-mediated mechanism: protective effect of PKA. Free Radic Biol Med. 2005, 40: 2005-2017.
Demehri F, Barrett M, Ralls M, Miyasaka E, Feng Y, Teitelbaum D: Intestinal epithelial cell apoptosis and loss of barrier function in the setting of altered microbiota with enteral nutrient deprivation. Front Cell Microbiol. 2013, 3: 1-15.
Bleich M, Shan Q, Himmerkus N: Calcium regulation of tight junction permeability. Ann N Y Acad Sci. 2012, 1258: 93-99.
Ma TY, Tran D, Hoa N, Nguyen D, Merryfield M, Tarnawski A: Mechanism of extracellular calcium regulation of intestinal epithelial tight junction permeability: role of cytoskeletal involvement. Microsc Res Tech. 2000, 51: 156-168.
Finamore A, Massimi M, Conti Devirgiliis L, Mengheri E: Zinc deficiency induces membrane barrier damage and increases neutrophil transmigration in Caco-2 cells. J Nutr. 2008, 138: 1664-1670.
Wang X, Valenzano MC, Mercado JM, Zurbach EP, Mullin JM: Zinc supplementation modifies tight junctions and alters barrier function of CACO-2 human intestinal epithelial layers. Dig Dis Sci. 2013, 58: 77-87.
Moran JR, Lewis JC: The effects of severe zinc deficiency on intestinal permeability: an ultrastructural study. Pediatr Res. 1985, 19: 968-973.
Warnes SL, Caves V, Keevil CW: Mechanism of copper surface toxicity in Escherichia coli O157:H7 and Salmonella involves immediate membrane depolarization followed by slower rate of DNA destruction which differs from that observed for Gram-positive bacteria. Environ Microbiol. 2012, 14: 1730-1743.
Wilks SA, Michels H, Keevil CW: The survival of Escherichia coli O157 on a range of metal surfaces. Int J Food Microbiol. 2005, 105: 445-454.
We thank Dr. Jay Mellies, Reed College, Portland, OR, for the gift of reporter strains JLM281, JLM165, and KMTIR3. Thomas A. Veeder and Anushila Chatterjee also contributed to this research during their laboratory rotations. We thank the National Institutes of Health (NIH) for financial support via grants RO1 AI 81528 and AI R21 102212.
The authors declare that they have no competing interests.
JB did the translocation experiments; RR developed the Miller assay and started the experiments with metals on recA; BW finished the experiments on recA, and tested metals on LEE4 and LEE5 expression. BW also measured bacterial elongation in response to SOS stimuli. SCB performed the bacteriophage plaque assays; JC planned experiments, compiled the data, and wrote drafts of the manuscript. All authors read and approved the final manuscript.
Electronic supplementary material
Additional file 1: Figure S1: Ability of zinc to block the bacterial elongation (filamentation) response that ccompanies the SOS response. Panel A, Elongation response in STEC strain Popeye-1. Popeye-1 was subcultured at a dilution of 1:100 from an overnight culture in LB into DMEM medium and grown at 37° with 300 rpm shaking. After 1.5 h, ciprofloxacin was added to a final concentration of 4 ng/mL and incubation was continued for an additional 1.5 h. Bacteria were stained by mixing with an equal volume of 0.2% acridine orange in ethanol for 10 min, then the bacteria were washed twice by centrifugation (at 500 g for 10 min) and resuspension in 250 μl of water to remove excess acridine orange. The stained bacteria were spotted on glass microscope slides, allowed to dry, then examined by fluorescence microscopy under oil at 1000 X magnification. Panel B, effect of metals on ciprofloxacin-induced bacterial length in EPEC strain E2348/69. EPEC E2348/69 was grown in the absence or presence of 0.1 μg/mL ciprofloxacin ± various metals as shown. Bacteria were stained with acridine orange as described for Panel A, then photographed using a Retiga digital camera. Digital images were captured or converted to black-and-white, then subjected to image analysis using ImageJ, free image analysis software developed at the NIH. The version we used is called Fiji (ImageJ for MacIntosh, version 1.47n). Detailed instructions on how to open and process the files are available from the author at email@example.com. Bacterial lengths were determined for each condition and expressed as a ratio compared to the no- ciprofloxacin, no-metal control bacteria. Panel C, effect of metals on bacterial elongation in STEC strain Popeye-1, using the same methods described for Panel B. Panel D, effect of zinc on mitomycin C-induced bacterial elongation. In Panel D the actual bacterial length is shown (in micrometers) using 2 micrometer size beads for calibration. (PDF 952 KB)
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Crane, J.K., Broome, J.E., Reddinger, R.M. et al. Zinc protects against shiga-toxigenic Escherichia coli by acting on host tissues as well as on bacteria. BMC Microbiol 14, 145 (2014) doi:10.1186/1471-2180-14-145
- Enterohemorrhagic E. coli
- Hemolytic-uremic syndrome
- SOS response
- Diarrheal diseases
- Xanthine oxidase