H. pylori mutants lacking TlpB swim away from acid gradients

H. pylori encounters many chemical gradients in the stomach that serve as cues to identify microniches that are safe for colonization. It must be able to integrate both repellents and attractants to optimize its chemotactic response. Since H. pylori’s TlpB chemoreceptor has been reported to detect HCl as a repellent [12, 13], and we found that it detects urea as a high-sensitivity attractant [15], we wondered how H. pylori would respond if it were simultaneously exposed to both urea and HCl gradients emanating from one point source.

We used our previously described microgradient chemotaxis assay [7, 15] to record the swimming responses of a live culture of H. pylori (strain PMSS1) exposed to a microscopic gradient of a mixture of 50 mM HCl and 5 mM urea emanating from the tip of a microinjection needle. Prior to the assay, H. pylori were grown in Brucella broth with 10% FBS (BB10), pH 6.7–6.8 to an OD₆₀₀ of 0.3. During culture, bacterial urease depletes urea from the surrounding medium (S1A Fig) and the pH remains at a range of 6.6–6.74 (S1B Fig). A 270 μl volume of media with motile bacteria is placed onto a coverslip chamber and a microinjection needle is then rapidly inserted via a micromanipulator into the viewing field to produce a microscopic gradient of chemoeffectors. Using this method, we observed that H. pylori are attracted to the urea in the gradient until they reach a boundary approximately 60 micrometers away from the needle tip (Fig 1A). Within this boundary is a zone of clearance avoided by the bacteria, representing a threshold concentration of acid that acts as a chemorepellant. When bacteria swim into this zone of clearance, they quickly stop, reverse direction, and swim away (S1 Movie). As a negative control, we tested a chemotaxis null mutant ΔcheW H. pylori for its response to the same mixed microgradient. The density of swimming ΔcheW H. pylori remained constant throughout the field (Fig 1A) consistent with this mutant’s inability to respond to either the attractant or the repellent. These observations indicate that H. pylori is capable of simultaneously sensing and integrating multiple signals from one point source. To test whether the chemotactic response is dependent on the magnitude of these chemical gradients, we altered the concentration of acid within the needle while maintaining the same concentration of urea. We found that, indeed, the bacteria respond by increasing the distance of the boundary between repulsion and attraction and the needle tip as the concentration of HCl increases (S2 Fig).

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Fig 1. H. pylori simultaneously responds to chemoattractants and repellents and does not require TlpB to swim away from an acid gradient.

(A) Still images of bacterial motility traces (lasting 1.5 seconds) of PMSS1 wild-type (WT) H. pylori and ΔcheW H. pylori within the field of view 1.5 seconds before and 18.5 seconds after exposure to a combined gradient of 5 mM urea and 50 mM hydrochloric acid. The position of the microinjection needle tip is highlighted in yellow. (B) Still images of bacterial motility traces (lasting 1.5 seconds) of ΔtlpB H. pylori within the field of view 1.5 seconds before and 18.5 seconds after exposure to a gradient of 5 mM urea and 50 mM hydrochloric acid. (C) Quantification of the responses of WT H. pylori vs. ΔtlpB vs ΔcheW to a 100 mM hydrochloric acid gradient. Each point represents the percent of swimming bacteria remaining in the field of view at each time point in the digitized video microscopy movie frames. Points for three to five movies are plotted per condition and grouped by color as indicated. Time zero is defined as the moment the needle is introduced and the gradient is initiated. p-value for scatter plot indicates significance of time by group interaction via a 2-way repeated measures ANOVA.

https://doi.org/10.1371/journal.ppat.1006118.g001

Because H. pylori abundantly expresses a urease enzyme that degrades urea into ammonia to buffer its cytoplasmic and periplasmic pH, we wondered whether urease may play a role in acid sensing. We first tested a urease mutant (ΔureAB) for its response to a solution of urea and HCl. Unlike the WT H. pylori culture, which is depleted of urea due to urease activity, the ΔureAB culture contains levels of urea in the medium comparable to fresh media (S1A). We observed that ΔureAB cleared the field of view completely (S3A Fig), indicating that it was unable to sense urea because the surrounding urea in the medium interferes with chemotactic sensing as we had previously reported [15] but was able to sense acid. We further tested for ΔureAB’s response to a solution of 100 mM HCl in water (no urea). We found that it cleared the field of view like wild-type (S3B Fig). These results suggest that urease activity is not required for acid sensing.

Next, we tested ΔtlpB H. pylori’s response to this mixed solution. As the urea and acid sensor, we predicted that this mutant would respond to neither compound and that its swimming behavior would be like that of ΔcheW H. pylori. We were surprised to find instead that ΔtlpB H. pylori rapidly swims away and clears from the field of view like ΔureAB (Fig 1B, S3A Fig, and S1 Movie). This observation that the bacteria swim away from the urea and acid microgradient suggests that the ΔtlpB mutant is unable to detect urea as we had previously reported [15] but is able to detect HCl as a repellent.

We proceeded to test ΔtlpB’s response to a solution of HCl in water without urea. We found that, indeed, ΔtlpB efficiently swims away from an acid gradient (Fig 1C and S2 Movie). We plotted the bacterial density in the viewing field every fifth of a second before and after introduction of the needle tip injecting HCl, and by ten seconds post-exposure to the acid gradient, the ΔtlpB mutant has mostly cleared from the field of view (Fig 1C). Interestingly, we note from the clearance curves (Fig 1C) that ΔtlpB clears from the field of view faster than wild-type upon acid exposure. This result suggests that TlpB does affect H. pylori’s response to acid since ΔtlpB has response kinetics different from wild-type. To verify that the ΔtlpB response to acid is not specific to a particular H. pylori strain, we constructed ΔtlpB mutants in other strains of H. pylori and tested them in the same assay. We found that the ΔtlpB mutants in all strains tested (strains G27, SS1, PMSS1 (a second independent clone), and 7.13) are still able to respond to an acid gradient like their wild-type counterparts by swimming away upon exposure to HCl and maintain the fast clearing phenotype (S4 Fig). This result indicates that ΔtlpB’s response to HCl is not strain specific. For the rest of the experiments we use H. pylori PMSS1 as the strain background.

H. pylori expresses two chemoreceptors that are each acid sensors

Our finding that ΔtlpB responds to an HCl gradient suggests that other chemoreceptors may be acid sensors. We tested the response of mutants lacking each of the other three chemoreceptors, ΔtlpA, ΔtlpC, ΔtlpD, by videomicroscopy in the same assay. To simplify the comparisons of the movies showing the escape from acid of different mutants, we graphed the percent of bacteria present in the viewing field 4 seconds before and 10 seconds after exposure to the acid gradient (Fig 2A). We found that each mutant was still able to respond and swim away from acid, indicating that either there is a novel unidentified chemoreceptor that senses acid or there are multiple chemoreceptors that can function redundantly in sensing acid.

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Fig 2. H. pylori expresses two chemoreceptors that rapidly sense acid gradients.

(A) Quantification of the responses of wild-type (WT) H. pylori vs. ΔtlpA, ΔtlpB, ΔtlpC, ΔtlpD to a 100 mM hydrochloric acid gradient. Temporal data of motility responses were collected by videomicroscopy and quantified as in Fig 1C. The difference in bacterial density within the field of view at two time points, four seconds before the acid gradient (pre) and ten seconds after exposure to the acid gradient (post) is represented by bar graphs. (B) Quantification of the responses of WT H. pylori vs. ΔcheW, ΔtlpAD, ΔtlpAB, ΔtlpAC, ΔtlpBC, ΔtlpBD, ΔtlpCD to a 100 mM hydrochloric acid gradient. Each bar represents the percent of bacteria in the field of view at four seconds pre-exposure and 10 seconds post-exposure to the gradient. (C) Still images of bacterial motility traces (lasting 1.5 seconds) of WT, ΔtlpAD, and ΔtlpB H. pylori within the field of view before and after exposure to a gradient of 5 mM urea and 50 mM hydrochloric acid. (n = 3 movies per condition). Bars represent the mean. Error bars represent s.d. NS indicates no statistical significance, **** P < 0.0001 (2-way repeated measures ANOVA).

https://doi.org/10.1371/journal.ppat.1006118.g002

To test the hypothesis that there may be redundancy in acid-sensing chemoreceptors, we made mutants lacking two of the four chemoreceptors in all possible combinations. We discovered that of all the six combinations of chemoreceptor knock-outs, only the mutant lacking both TlpA and TlpD (ΔtlpAD H. pylori) lost the ability to respond to HCl gradients (Fig 2B and S3 Movie). This result indicates that TlpA and TlpD function as acid sensors, each capable of compensating for the loss of the other in acid sensing.

Furthermore, when we tested for the response of ΔtlpAD H. pylori to the solution containing a mixture of urea and HCl, we observed that the bacteria are attracted towards the needle tip with no zone of clearance (Fig 2C). This result indicates that the ΔtlpAD mutant can detect and respond to urea as an attractant (through TlpB), but is unable to detect the HCl as a repellent. This result suggests that TlpB is not sufficient to sense acid in our assay, and TlpA and TlpD are acid sensors that detect acid gradients.

We next asked whether the response to acid is a response to low pH or a response specifically to HCl. To determine this, we tested the responses of WT, ΔtlpA, ΔtlpB, ΔtlpD, and ΔtlpAD to sulfuric acid (H₂SO₄) and phosphoric acid (H₃PO₄). As with HCl, we observed that H. pylori responds to both of these acids as repellents and requires either TlpA or TlpD for the response (S5 Fig). This result suggests that these two chemoreceptors allow H. pylori to sense and escape from conditions of low pH.

TlpD is more sensitive than TlpA in detecting hydrochloric acid

Several chemoeffectors have been described for TlpA and TlpD. The TlpA receptor was reported to mediate attraction to arginine and bicarbonate [16]. The TlpD chemoreceptor was reported to mediate repulsion from conditions that induce low-energy in the bacterium [17] or conditions that promote oxidative stress [18, 19]. These conditions may be triggered by low pH. One key difference between TlpA and TlpD is the location of these chemoreceptors within the bacterium. The TlpD chemoreceptor is cytoplasmic as it lacks a transmembrane domain [17] whereas the sensing domain of TlpA is periplasmic like that of the TlpB and TlpC chemoreceptors. Therefore, TlpD may be sensing changes in external pH indirectly. Given the difference in the location of these two chemoreceptors, we wondered if the two receptors may have distinguishable responses to the same HCl gradient.

To assess if there is a difference in sensitivity for detecting HCl between the two chemoreceptors, we determined the threshold concentration of HCl necessary to elicit a response (arbitrarily defined as a 60 microns clearance zone from the point source) for each mutant. We empirically determined that 25 mM HCl loaded in the microinjection needle is the minimum concentration required to repel wild-type H. pylori from the point source by 60 microns (Fig 3). ΔtlpA H. pylori, like wild-type, responds to a minimal effective concentration of 25 mM HCl while ΔtlpD H. pylori requires 50 mM HCl to respond (Fig 3). It is worth noting, however, that the actual minimal effective concentration of HCl that H. pylori is capable of detecting is markedly below 25 mM, since only a minute volume of HCl on the order of 1 picoliter/minute is injected into the solution, and the culture medium surrounding the bacteria consists of Brucella broth with 10% fetal bovine serum, which has a buffering capacity that we empirically determined to be about 4,000 fold greater than water (S6 Fig). Thus the gradient of free hydrogen ions would drop rapidly away from the needle tip. Since we observe the bacteria responding 60 microns away from the point source, the change in HCl concentration that the bacteria can sense is substantially less than the concentration of the solution in the needle. Indeed, when we expose the bacteria to a gradient starting from 15 mM HCl at the needle tip, we also see the bacteria being repelled but at approximately 30 microns away from the point source (S7 Fig).

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Fig 3. TlpD is more sensitive to a hydrochloric acid gradient than TlpA.

Still images of bacterial motility traces (lasting 1.5 seconds) of wild-type H. pylori vs. ΔtlpB vs. ΔtlpA vs. ΔtlpD before (panels in left column) and after exposure to a gradient of either 25 mM (panels in middle column) or 50 mM hydrochloric acid (panels in right column). The positions of the needle tips are marked in yellow.

https://doi.org/10.1371/journal.ppat.1006118.g003

Since H. pylori is exposed to both urea and HCl in vivo, we wondered whether urea sensing would affect the sensitivities of TlpA and TlpD in sensing acid. We exposed ΔtlpA and ΔtlpD to a gradient of a mixture of 5 mM urea and 50 mM HCl in the microinjection needle. We observed that both mutants are attracted to the urea but form a zone of clearance as they sense HCl like wild-type H. pylori. However, with urea present we could elucidate small differences in sensitivity because the attraction to urea highlights TlpD’s ability to detect lower concentrations of acid than TlpA. This is illustrated by the ΔtlpA mutant remaining at a farther distance away from the acid point source at the needle tip compared to ΔtlpD (S8 Fig). This result indicates that urea sensing does not alter the sensitivity hierarchy of TlpD and TlpA in acid sensing.

H. pylori senses and responds to both acidic and basic changes in pH with nanomolar sensitivity

As chemotaxis is a result of detecting a change in the concentration of a chemical, we next sought to determine the smallest change in hydrogen ion concentration ([H+]) that H. pylori is able to detect and respond to. By comparing the pH of the Brucella broth culture medium in which the bacteria are grown with the pH of a buffer solution that elicits a repulsion response, we determined the smallest difference in [H+] that H. pylori is capable of detecting. To more accurately control the range of [H+] concentrations experienced by the bacteria, we loaded the microinjection needle with 1M phosphate buffer solutions with defined pHs made by combining different proportions of dibasic and monobasic phosphate solutions. We measured the pH of the Brucella broth medium that the bacteria are grown in to be pH 6.7 (S1B Fig). We then tested wild-type bacteria’s response to buffer solutions ranging from pH 4.2 to 7.1.

As shown in Fig 4A, buffers with pH 4.2, 6.0, 6.3, and 6.5 all elicited an escape response in the microgradient assay. The increase in [H+] between the solution released from the microinjection needle and the culture medium was approximately 63 μM, 800 nM, 360 nM, and 110 nM, respectively. For the lower pH measurements between pH 4 and pH 6 we also confirmed our results using citrate buffer, which buffers acidic pH more effectively than phosphate buffer (S9 Fig). Phosphate buffer solutions of pH 6.6 and 7.0, which locally changed the [H+] by + 35 nM or -100 nM, did not elicit a response, indicating that the differences were below the limit of detection of the receptors. Unexpectedly, a buffer solution with pH 7.1, (about -120nM change in [H+]) elicited an opposite response with bacteria attracted and forming a swarm at the needle tip (Fig 4B and S4 Movie). Thus, we discovered that H. pylori can sense and respond to small changes in both acidic and basic pH when the change in [H+] is greater than 100 nM.

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Fig 4. H. pylori can respond to acidic and basic changes in pH with nanomolar sensitivity.

(A) Quantification of the responses of wild-type (WT) H. pylori to phosphate buffer solutions with pH ranging from 4.2 to 7.1. The addition (+) or depletion (-) of hydrogen ions relative to the hydrogen ion concentration in the culture medium (pH 6.7) is indicated next to the pH of the buffer solution introduced. Each point represents the percent of swimming bacteria remaining in the field of view at each time point in the digitized video microscopy movie frames. Points for one movie are plotted per condition. Time zero is defined as the moment the needle is introduced and the gradient is initiated. (B) Still images of bacterial motility traces (lasting 5 seconds) of WT H. pylori before (panels in left column) and after injection of a phosphate buffer solution with pH 7.1, 6.5 or 6.6 (panels in right column). The pH of the culture medium was 6.7. The positions of the needle tips are marked in yellow.

https://doi.org/10.1371/journal.ppat.1006118.g004

TlpA and TlpD both sense acidic pH while TlpD also detects basic pH

To further characterize wild-type H. pylori’s response to more basic environments, we also tested phosphate buffers with pH 7.25 and 9.2. We found that H. pylori is attracted to basic pH solutions (S10 Fig). By testing the single chemoreceptor mutants, we identified TlpD as the necessary receptor for attraction to higher pH (Fig 5 and S5 Movie). The other receptors, including TlpA, were not necessary. To confirm that the TlpD-dependent attraction is a response to high pH rather than to a specific basic solution, we tested for H. pylori’s response to 40 mM sodium hydroxide (pH 12.6). We also observed H. pylori being attracted to sodium hydroxide, and the response was dependent on TlpD (S11 Fig). Taken together these results suggest that TlpD mediates both repulsion from lower pH and attraction to higher pH while TlpA only detects and mediates repulsion to lower pH.

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Fig 5. H. pylori attraction to basic changes in pH is mediated through TlpD.

Still images of bacterial motility traces (lasting 5 seconds) of wild-type H. pylori vs. ΔtlpA vs. ΔtlpD vs. ΔtlpAD before (panels in left column) and after injection of a phosphate buffer solution with pH 9.2 (panels in right column). The pH of the culture medium was 6.7. The positions of the needle tips are marked in yellow.

https://doi.org/10.1371/journal.ppat.1006118.g005

TlpB alters the response kinetics and sensitivity to changes in pH

We wondered whether the TlpB-dependent defect in acid sensing previously reported and our observation of faster clearance rates of ΔtlpB mutants compared to wild-type may be due to an effect of TlpB in modulating the sensitivity to pH of the other chemoreceptors. In order to see if lacking TlpB enhances the sensitivity to acid, we tested for the response of ΔtlpB H. pylori to low concentrations of HCl and found that the minimal effective concentration of HCl in the needle required to elicit an escape response is the same as that of wild-type at 25 mM HCl (Fig 3). We also tested the responses of the TlpA and TlpD chemoreceptors in the absence of TlpB by determining the sensitivities of the ΔtlpAB and ΔtlpBD double mutants to acid gradients. We found them to have the same sensitivity to HCl as ΔtlpA and ΔtlpD, respectively (S7 Fig).

However, when we tested for H. pylori’s response to higher pH, we noted that ΔtlpB’s attraction was always more pronounced than wild-type with each higher pH solution (S10 Fig); the attraction of ΔtlpB was faster, and the concentration of bacteria around the needle tip was denser than that of wild-type. This observation led us to hypothesize that TlpB may be modulating H. pylori's response to basic pH. We tested for the mutant’s response to a gradient formed by phosphate buffer at pH 7.0 where wild-type H. pylori does not show an attraction. The ΔtlpB mutant is still able to sense and respond to the solution at pH 7.0 (-100nM change in [H+]) (S10 Fig). This result suggests that lacking TlpB increases the bacteria's sensitivity and attraction to higher pH, and thus TlpB may be modulating the pH responses mediated through TlpD.

The mechanism by which TlpB influences pH sensing is unknown. We tested whether TlpB alters the expression levels of TlpA or TlpD, thereby resulting in a change in acid response kinetics. We performed a Western blot to assess expression levels of the chemoreceptors in the single knock-out mutants and ΔtlpAD H. pylori. We found that the expression levels of the remaining chemoreceptors were not affected by the loss of the TlpA, TlpB, or TlpD receptors (S12 Fig).

Our data show that TlpB is not sufficient for sensing acidic pH, but it does alter the kinetics of H. pylori’s response to changes in pH. Taken together, our data suggest that the mechanism of pH sensing in H. pylori is complex, involving multiple chemoreceptors. The difference in sensitivity between TlpA and TlpD and the role of TlpB in modulating pH responses allows H. pylori to discern even small changes in local pH gradients in the nanomolar range. This may have critical implications for H. pylori’s survival in the stomach.

Loss of both TlpA and TlpD creates a deficiency in H. pylori’s ability to colonize the stomach, and this deficiency can be rescued by inhibiting acid production in the stomach

Given the importance of avoiding the acidic lumen of the stomach environment, we next investigated whether ΔtlpAD H. pylori would be able to colonize the stomachs of mice. We infected C57Bl/6 mice with either wild-type H. pylori strain PMSS1 or the isogenic mutants ΔtlpA, ΔtlpD, or ΔtlpAD. After two weeks of infection, a time point in which wild-type H. pylori has established stable colonization [7, 20], we harvested the stomachs and assessed colonization densities by colony-forming units (CFU) per gram of stomach tissue. We found that the ΔtlpA mutant was not defective in colonization with similar CFU counts as wild-type bacteria. However, the ΔtlpD mutant had a 10-fold defect as had been previously reported [20], and the ΔtlpAD H. pylori mutant was about 100-fold defective in establishing colonization (Fig 6). We hypothesized that without the ability to respond to acid gradients in the stomach, the ΔtlpAD H. pylori is deficient in avoiding the microbicidal HCl. We wondered if pharmacologic inhibition of acid secretion in the stomach would improve ΔtlpAD H. pylori’s survival.

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Fig 6. TlpA and TlpD are important in establishing colonization in acidic conditions in a murine model of gastric infection. Acid suppression rescues ΔtlpAD colonization defect.

Recovered colony forming units (CFU) of H. pylori per gram of stomach tissue after a 2-week infection with wild-type (WT) H. pylori, ΔtlpA H. pylori, ΔtlpD H. pylori, or ΔtlpAD H. pylori (n = 10 mice for WT H. pylori, ΔtlpAD H. pylori, and ΔtlpD H. pylori; n = 7 for ΔtlpA H. pylori). For the experimental groups, omeprazole was administered in the drinking water 3 days prior to infection and throughout the course of the infection (purple), or for 1 week beginning 1 week after infection with H. pylori (blue). Blue dotted line indicates the limit of detection. Bars represent the geometric mean. * P < 0.05, ** P < 0.01, *** P < 0.001, **** P < 0.0001 (Mann Whitney test).

https://doi.org/10.1371/journal.ppat.1006118.g006

We maintained two experimental groups to test this hypothesis. One group of animals was treated with the proton-pump inhibitor omeprazole for three days prior to infection to raise the gastric pH before infection (S13 Fig), and the animals continued to receive omeprazole throughout the course of the 2-week infection. This experimental group allowed us to observe how the gastric pH experienced by the bacteria upon entering the stomach affects the bacteria’s survival in the stomach. The second group of animals was infected with H. pylori for a week before treatment with omeprazole throughout the final week of infection. This group represents the more common clinical scenario in which humans with an established H. pylori infection may take proton-pump inhibitors like omeprazole to treat conditions such as gastroesophageal reflux. We found that treatment of animals with omeprazole prior to or after the establishment of infection partially rescued ΔtlpAD H. pylori’s ability to colonize the stomach (Fig 6), while it did not affect the total number of wild-type bacteria.

We previously reported that in this murine model of infection and in humans the majority of the bacteria reside in the overlying mucus layer. However, a subpopulation of H. pylori can be found deep in the gastric glands adhered to epithelia cells that make up the mid-glandular proliferative zone [7, 11]. We wondered whether acid sensing would affect not only the overall fitness of the bacteria establishing colonization in the stomach, but also their ability to reach and colonize the epithelial surface of the gastric glands. To investigate gastric gland colonization, we used quantitative 3D confocal microscopy to determine the number of bacteria growing as microcolonies within the gastric glands in the antrum and corpus regions of the stomach. One of the main distinguishing features between antrum and corpus is the presence of acid-secreting parietal cell in the corpus glands.

In control animals with normal acid secretion, the wild-type strain is found mostly colonizing the antral glands and the transition zone between the antrum and corpus [7, 11] (S14A and S14B Fig) rather than the corpus glands (S14C and S14D Fig). We found that in only two out of seven animals infected with ΔtlpAD H. pylori, the mutant was able to colonize the antral glands but at significantly lower densities than wild-type H. pylori (Fig 7A, 7C and 7E). This result suggests that chemotaxis through TlpB and TlpC still allows some bacteria to reach the epithelium and colonize the glands. We know that one such signal is the chemoattractant urea sensed through TlpB [15]. The defect in gland colonization of the mutant, however, may be attributed to low bacterial numbers in both the mucus and the glands as it has a 100-fold defect in overall bacterial load compared to wild-type H. pylori (Fig 6).

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Fig 7. The density of gland-associated H. pylori in the antrum of the stomach is influenced by gastric acidity.

(A-D) 3D confocal immunofluorescence reconstructions of mice infected with wild-type (WT) or ΔtlpAD H. pylori followed by treatment with omeprazole or no treatment. H. pylori are stained in green and actin in red. Scale bar is 100μm for all 4 panels. (E) Quantification of the number of bacteria per gland in the antrum of animals infected with WT or ΔtlpAD treated with omeprazole or untreated. The antral glands of seven animals in each cohort were analyzed for bacterial colonization by 3D volumetric analysis. The number of bacteria in each individual gland is plotted as a scatter point. * P < 0.05, **** P < 0.0001 (Mann Whitney test). The panels on the right show an example of the volumetric measurement of bacteria in gastric glands. 3D confocal reconstructions of glands stained with anti–H pylori (green), phalloidin (red), and DAPI (blue) were generated. Bacterial microcolony signals are identified by fluorescence intensity and size using Volocity software and the identified voxels marked in gray (bottom panels) are measured. The number of bacteria per gland is calculated based on the average voxel volume of 1 bacterium. Scale bar is 10μm for all 4 panels.

https://doi.org/10.1371/journal.ppat.1006118.g007

We performed a similar analysis of gastric gland colonization of ΔtlpAD H. pylori in animals treated with omeprazole after infection, since in these conditions the bacterial load in the stomach was comparable to that of wild-type (Fig 6). When we analyzed the antral glands of infected animals treated with omeprazole one week post-infection, we noted that the bacterial density of both wild-type and ΔtlpAD H. pylori in the antral glands increased significantly compared to those in control animals (Fig 7B, 7D and 7E). Despite the increase in gland colonization, ΔtlpAD H. pylori does not reach the levels of wild-type in the antral glands of omeprazole-treated animals (Fig 7E). These results suggest that omeprazole promotes the colonization of H. pylori in the gastric glands of the antrum, and chemotaxis through TlpA and TlpD is important for proper colonization of the antral glands.

Using quantitative 3D-confocal microscopy, we also found that loss of stomach acidity through omeprazole treatment allowed H. pylori to extend its colonization to the corpus glands (Fig 8). Control animals normally do not have H. pylori in corpus glands (Fig 8A). In our analysis, only one out of the seven control animals had detectable levels of H. pylori in the corpus glands (Fig 8C). In the corpus, the gland-associated bacteria seen after omeprazole treatment were mainly concentrated in the neck region of the glands in the proliferative zone (Fig 8B), and also were seen in close proximity to parietal cells (Fig 8D). This result suggests that the acid in the stomach restricts H. pylori gland-colonization to the antral glands but that an increase in gastric pH allows H. pylori to extend its range to also colonize the epithelium of the corpus glands. We did not find ΔtlpAD H. pylori in the corpus glands of omeprazole-treated animals. These results from the omeprazole treatment experiments suggest that gland colonization is distinct from colonization of the mucus, and sensing through TlpA and TlpD may be necessary for localizing to and/or persisting in the corpus glands.

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Fig 8. Omeprazole treatment expands H. pylori colonization into the corpus glands of stomach.

(A-B) Representative confocal 3D images of the corpus glands infected with wild-type (WT) H. pylori followed by 1-week treatment or no treatment with omeprazole. H. pylori are stained in green and the cellular actin cytoskeleton is stained with phalloidin in red. Scale bar 100μm for both panels. (C) Quantification of the number of bacteria per gland in the corpus of animals infected with WT H. pylori treated with omeprazole or untreated control. The corpus glands of seven animals in each cohort were analyzed for bacterial colonization by 3D volumetric analysis. Only one out of seven control animals had detectable bacteria in the corpus. **** P < 0.0001 (Mann Whitney test). (D) Higher magnification image of the corpus glands from omeprazole-treated animals infected with wild-type H. pylori. H. pylori are stained in green and actin in red. Gland-associated H. pylori are seen in proximity to parietal cells (P) magnified in the insets. H. pylori are stained with antibodies in green. The glands are visualized with actin staining with phalloidin in red and nuclei are stained with DAPI in blue. Scale bar is 100μm in D and 10μm in the insets in D.

https://doi.org/10.1371/journal.ppat.1006118.g008

Bacterial strains and culture conditions

The previously published wild-type H. pylori strain PMSS1 [40], ΔureAB and single knock-outs chemoreceptor mutants [15] were used for all experiments in this study except those strains noted in S4 Fig. H. pylori strains were either grown on Columbia blood agar plates or in Brucella broth supplemented with 10% fetal bovine serum (BB10) at 37°C, 10% CO₂, as described previously [41]. The ΔtlpAB, ΔtlpAC, ΔtlpAD, ΔtlpBC, ΔtlpBD, and ΔtlpCD PMSS1 isogenic mutants were constructed by natural transformation with genomic DNA from the relevant single knock-out chemoreceptor mutant made in strain PMSS1. The PMSS1 chemoreceptor mutants were verified by immunoblotting using an antibody that recognizes a conserved domain in all four chemoreceptors, courtesy of K. Ottemann [42].

Test solutions for microgradient assay

All solutions were diluted or dissolved in sterile, distilled, and deionized water. Urea and sodium hydroxide solutions were made by dissolving ultra-pure urea or sodium hydroxide tablets into sterile, distilled and deionized water. One molar hydrochloric acid (Sigma Aldrich, Saint Louis, MO) was diluted into sterile, distilled and deionized water to create various concentrations of hydrochloric acid solutions to test. To obtain phosphate buffered solutions with different pHs, 1 M monobasic sodium phosphate (NaH₂PO₄) pH 4.1 and 0.5 M dibasic sodium phosphate (Na₂HPO₄) pH 9.0 were combined in various proportions until desired pH is achieved and confirmed by pH meter. To obtain citrate buffered solutions with different pHs, 1 M citric acid (C₆H₈O_{7 •} H₂O) pH 2.0 and 1 M sodium citrate (C₆H₅O₇Na_{3 •} 2H₂O) pH 8.6 were combined in various proportions until desired pH is achieved and confirmed by pH meter. The buffering capacity and corresponding pH of various concentrations of HCl in BB10 was determined empirically (S6 Fig).

Microgradient assay

H. pylori cultures used for the assay were made by subculturing from a 16-hour overnight Brucella broth + 10% FBS (BB10) culture with a starting OD₆₀₀ of 0.15. The subcultures (also in BB10) were grown for 6 hours until they reach an OD₆₀₀ of 0.3 before using in the microgradient assay. The pH of bacterial cultures prior to the microgradient assay (spent media) was measured at a mean of 6.65 +/- 0.04 SD (S1B Fig). These were not different from the pH of BB10 kept in the incubator without bacteria measured at 6.6, or freshly made BB10 (pH 6.6–6.8). The bacterial culture media for all strains tested, except ΔureAB, contain no detectable urea at the time of the assay due to bacterial urease activity during the subculture (S1A Fig). This was determined by measuring the concentration of urea using the QuantiChrom Urea Assay Kit (BioAssay Systems), a colorimetric assay that quantifies urea directly with a detection level of 13μM. Background was determined by quantifying urea in urease-treated BB10. Twenty five milliliters of fresh BB10 (predicted to contain 2–4 mM urea) were incubated with 300 units of Jack Bean urease for 2 hours at 25°C. This amount of urease is calculated to liberate 0.3 millimole of ammonia in 1 min at 25°C, and therefore is sufficient to hydrolyze all the urea in the media in about one minute. To ensure complete urea degradation, we allowed the reaction to proceed for 2 hours before boiling the urease-treated media for 10 minutes to inactivate urease and filtering the media through a 0.2 μm filter to remove particulates.

Two hundred seventy microliters of the subculture were placed into the center of a glass-bottom 35-mm dish (MatTek) contained by a ring of vacuum grease. The dish was placed above a 32x objective of a Zeiss Axiovert-35 inverted microscope equipped with phase-contrast optics and a heated stage (37°C). A Hammamatsu C2400 video charge-coupled-device (CCD) camera was used to record via an Argus-20 image processor onto Quicktime at 30 frames per second. A Femtotip II microinjection micropipette (Eppendorf) containing 8 μl of the test solution was inserted into or removed from the viewing field using a micromanipulator (Eppendorf 5171) [7]. To create a microscopic gradient (microgradient) in the bacterial culture, a compensation pressure of 30 hPa was applied via the Eppendorf transjector 5246 to maintain a constant flow at 0.372 picoliters/minute from the tip. This pressure was determined empirically and selected because it did not physically affect the bacteria swimming near the micropipette tip while generating a stable gradient within the viewing field.

Quantification of bacterial chemotactic responses to microgradients and display of bacterial traces

H. pylori chemotactic responses were quantified from phase contrast video microscopy movies recorded at 30 frames per second using ImageJ software version 1.46r. Movies were analyzed starting from 4 to 10 seconds before micropipette insertion (pre-injection) to 10–30 seconds after micropipette insertion (post-injection). After background subtraction and contrast adjustment, movies were then subsequently quantified or bacterial traces were obtained for visual depiction of swimming behavior in response to the gradient. For quantification, 0.2 second segments of the movies (6 frames) were combined into Z-projections to generate traces of moving bacteria. Motile bacteria were detected by specifying a size between fifty to three hundred pixels and circularity values between 0.1 to 0.5 (non-motile particles will be more circular than motile bacteria, which will be elliptical traces). These parameters were set in the Analyze Particle function in ImageJ and the output provided the number of motile bacteria per frame. The number of motile bacteria per frame is normalized to the average number of motile bacteria prior to needle entry. Responses are shown as either scatter plots, which display the percent bacteria per field from 4–5 seconds pre-injection to 10–15 seconds post-injection, or bar graphs, which display the percent bacteria per field at 4 second pre-injection and 10 seconds post-injection. Statistical significance between the percent bacteria per field pre-injection versus percent bacteria per field post-injection in the bar graphs or of the overall response in the scatter plots was assessed using a 2-way repeated measures ANOVA. To produce the images that depict the bacterial swimming behavior, longer traces were generated to clearly show the response. The time stated in the pre-injection panel indicates the first frame until 0 seconds used to generate the trace (i.e. -1.5 sec means frames from 1.5 seconds prior to needle entry to 0 second when the needle enters were used to generate a 1.5 trace representing the pre-injection swimming behavior). The range of time stated in the post-injection panels indicates the frames used to generate the trace (i.e. 18.5–20 sec means the frames from 18.5 seconds to 20 seconds post-injection were used to generate a 1.5 trace representing the post-injection swimming behavior).

Immunoblotting

H. pylori cells were harvested from blood plates and lysed with 1x SDS sample buffer. Lysates were boiled for 5 minutes and then separated on a 10% SDS-PAGE gel. After transfer onto nitrocellulose membranes, H. pylori TlpA, TlpB, TlpC, TlpD were detected by blotting with rabbit anti-tlpA22, an antibody that recognizes a conserved domain in all 4 chemoreceptors, courtesy of K. Ottemann [42], followed by a goat anti-rabbit Alexa Fluor 660. UreA, the small subunit of the abundantly expressed urease protein, was used as a loading control and detected with a mouse anti-UreA antibody followed by a goat anti-mouse Alexa Fluor 800. The blot was then scanned with a Licor-Odyssey scanner at 700 and 800 nanometers.

Ethics statement

Experiments involving animals were performed in accordance with NIH guidelines, the Animal Welfare Act, and US federal law. All animal experiments were approved by the Stanford University Administrative Panel on Laboratory Animal Care (APLAC) and overseen by the Institutional Animal Care and Use Committee (IACUC) under Protocol ID 9677. Animals were euthanized by CO₂ asphyxiation followed by cervical dislocation.

Animal experiments

6 week-old female C57BL/6J mice were purchased from the Jackson Laboratory (Bar Harbor, ME). Animals were infected intraorally by allowing the animals to drink a 5 microliter suspension containing 10⁸ CFU of H. pylori grown in BB10 from a pipette tip [7]. One cohort of animals was treated with omeprazole at 400 μmol/kg/day via drinking water for seven days after seven days of infection. A second cohort of animals was treated with omeprazole (400 μmol/kg/day) for three days prior to infection and then maintained on omeprazole for the duration of the two-week infection. The control cohort was given untreated water throughout the course of the two week infection. Animals were sacrificed at 2 weeks post-infection by CO₂ asphyxiation. The stomach was harvested with the forestomach removed and discarded, opened via the lesser curvature, and laid flat onto filter paper. Luminal content was removed and the stomach was divided into halves that spanned the corpus to the antrum. One half of the stomach was weighed and mechanically homogenized for 30 seconds in 1 ml Brucella broth. Homogenized stomachs were serially diluted and plated for CFU counts. The data represent the number of CFU/gram of stomach. Bars represent the geometric mean. Statistical significance in the recovered bacterial load between strains was assessed by a Mann Whitney test. The efficacy of the omeprazole treatment was determined via a separate experiment where 5 mice were administered omeprazole in their drinking water for 3 days prior to sacrifice and 5 mice were given water for 3 days prior to sacrifice (S13 Fig). To measure the pH of the stomach, the stomach was cut along the lesser curvature and splayed open. The stomach tissue along with its contents were placed at the bottom of a test tube (with opening wide enough to fit a pH probe) with the stomach lumen facing up. One milliliter of sterile water was added to the stomach in the tube. The pH was then measured using a pH meter.

Immunofluorescence imaging of stomach sections

The other half of the stomach was fixed in a 2% paraformaldehyde and stained for confocal microscopy as previously described [7, 11]. A custom made rabbit anti-H. pylori PMSS1 antibody and chicken anti-rabbit Alexa Fluor 488 antibody was used. DAPI (4 =, 6-diamidino-2-phenylindole) and Alexa Fluor 594-phalloidin (Molecular Probes) were used for visualization of the nuclei and actin cytoskeleton. Samples were imaged with a Zeiss LSM 700 confocal microscope and z-stacks were reconstructed into 3D images using Volocity software (Improvision). Number of bacteria per gland was determined with measurement functions in Volocity.

Statistical analyses

All microgradient assay data comparing percent bacteria per field at 4 seconds pre-injection to percent bacteria per field at 10 seconds post-injection as well as the scatter plots of percent bacteria per field over time were analyzed via a 2-way repeated measures ANOVA test in the GraphPad Prism 7 software program. The p-value for the scatter plots indicates the significance of the time by group interaction via a 2-way repeated measures ANOVA. For animal experiments, statistical significance was assessed via a Mann Whitney test. Center values are geometric means and error bars represent standard deviation (s.d.). n indicates the number of movies per condition or the number of animals used. NS indicates no statistical significance, * P < 0.05, ** P < 0.01, *** P < 0.001, **** P < 0.0001.