Helicobacter pylori plays an essential role in the pathogenesis of gastritis, peptic ulcer disease, and gastric cancer. The serine protease HtrA, an important secreted virulence factor, disrupts the gastric epithelium, which enables H. pylori to transmigrate across the epithelium and inject the oncogenic CagA protein into host cells. The function of periplasmic HtrA for the H. pylori cell is unknown, mainly due to unavailability of the htrA mutants. In fact, htrA has been described as an essential gene in this bacterium. We have screened 100 worldwide H. pylori isolates and show that only in the N6 strain it was possible to delete htrA or mutate the htrA gene to produce proteolytically inactive HtrA. We have sequenced the wild-type and mutant chromosomes and we found that inactivation of htrA is associated with mutations in SecA – a component of the Sec translocon apparatus used to translocate proteins from the cytoplasm into the periplasm. The cooperation of SecA and HtrA has been already suggested in Streptococcus pneumonia, in which these two proteins co-localize. Hence, our results pinpointing a potential functional relationship between HtrA and the Sec translocon in H. pylori possibly indicate for the more general mechanism responsible to maintain bacterial periplasmic homeostasis.
HtrA (High Temperature Requirement A) proteins are a family of evolutionarily well preserved serine proteases, identified in the majority of the examined organisms. In addition to their proteolytic activity, several HtrAs exhibit also chaperone-like properties. In prokaryotes these proteins localize to the periplasm, may be attached to membranes or are secreted out of the cell1. Most of HtrAs are involved in the protein quality control and are responsible for the removal of improperly folded proteins from the cellular envelope using their both, proteolytic and chaperone-like, activities2. Aside from their housekeeping functions, certain HtrA homologs play regulatory roles, e.g., regulate the σE-dependent stress response3, others are involved in maturation and secretion of surface proteins, including several virulence factors4. In the Gram-positive bacteria, Streptococcus pyogenes and Streptococcus pneumoniae, HtrA co-localizes to the Sec machinery on the cell surface5,6,7. This fact raises the possibility that HtrA is involved in processing/maturation and/or in quality control of the exported proteins in streptococci. Recently, it was demonstrated that secreted fractions of bacterial HtrAs can directly contribute to the pathogenesis of certain human diseases8. Such diverse tasks are usually performed by several HtrA homologs that function in parallel in a cell. For example, bacteria from the Enterobacteriaceae family encode three members of the HtrA family: HtrA (DegP), DegQ (HhoA) and DegS (HhoB) (UniprotKB, www.expasy.org). However, there are various other bacterial species that carry only one HtrA homolog, including the human pathogen Helicobacter pylori.
H. pylori secretes a certain fraction of HtrA into the extracellular space as an active soluble protease or embedded in outer membrane vesicles (OMVs), promoting bacterial colonization and invasion of host tissues9,10,11,12. Remarkably, secreted HtrA can cleave the extracellular NTF (N-terminal fragment) domain of E-cadherin, the adherens junction protein in polarized gastric epithelial cells11,13. In fact, the ectodomain cleavage of E-cadherin by HtrA results in the disruption of the intercellular adherens junction complex, which supports H. pylori access to deeper tissues11,14. In addition, H. pylori HtrA also targets the tight junction proteins occludin and claudin-8, and the extracellular matrix protein fibronectin11,14,15. Moreover, we demonstrated that HtrA protease activity is required for paracellular transmigration of H. pylori to access basolateral sites, target integrin-α5β1 and inject oncogenic protein CagA via a type IV secretion system encoded by the cag pathogenicity island (PAI)11,14,15. Thus, secreted HtrA exemplifies the first known non-PAI protein contributing considerably to T4SS functionality in H. pylori.
Significant research progress on H. pylori HtrA properties is mainly hindered by the non-existence of htrA knockout mutants, advocating that htrA may be an essential gene in H. pylori16. To by-pass this major draw-back and to investigate the role of HtrA in more detail, in previous studies we overexpressed the enzyme by introducing a second htrA gene copy in the genome and investigated multiple virulence activities by H. pylori17, and established a genetic complementation system of H. pylori HtrA in the close relative Campylobacter jejuni showing its functionality in the bacteria18. Still, an appropriate model to study the HtrA function in H. pylori was missing.
In the present work, we demonstrated that in one strain, H. pylori N6, it was possible to delete the htrA gene from the chromosome or to introduce a 661T > G point mutation into htrA which changes serine 221 into alanine (S221A) and, in consequence, destroys the catalytically active site in HtrA. We also showed that H. pylori lacking HtrA or with inactive HtrA exhibited reduced transmigration activity across MKN28 polarized epithelial cells and reduced translocation of CagA in polarised Caco-2 cells in comparison to the wild-type or htrA-complemented strains. Whole genome sequencing demonstrated that in both mutant strains, the htrA deletion knockout (N6 ΔhtrA) or the protease deficient (N6 htrAS221A), htrA inactivation was accompanied by the spontaneous occurrence of an additional mutation in the secA gene. The function of the SecA protein in H. pylori was not studied thoroughly, but its homologs from other bacterial species are engaged in the transport of newly synthesized polypeptides to be exported by the Sec translocon (type II secretion system). Thus, our work led to construction of a highly valuable new tool for further studies on the role of HtrA in H. pylori physiology and virulence, but also indicated for the possible interdependence between Sec translocon and HtrA in H. pylori in maintaining proper homeostasis in the H. pylori periplasm.
htrA can be deleted in the H. pylori N6 strain
HtrA has been shown to be essential for the viability of every H. pylori strain tested so far16,19. However, it is not very common that HtrA is indispensable for many other bacteria under conventional growth conditions. Thus, we undertook another attempt to inactivate htrA in H. pylori using two strategies. We constructed two vectors, pUZ16 and pUZ17, which were designed to recombine with the H. pylori chromosome at the htrA locus and subsequently delete htrA or substitute T661 for G, respectively (Methods and Supplementary Fig. S1). 661T > G introduces the S221A mutation and, in consequence, inactivates the HtrA catalytic active site. A set of 100 worldwide H. pylori strains from Europe, Asia, Australia, North America and South America (Supplementary Table S1) was transformed with purified pUZ16 and pUZ17 plasmids. Kanamycin resistant colonies were only obtained for the N6 strain. Genomic DNA was extracted from eight pUZ16 and ten pUZ17 transformants and analyzed by PCR using H6-H7 primers (Supplementary Table S4) which amplify the entire htrA gene. The analysis indicated that no htrA gene was present anymore in six H. pylori htrA deletion (N6 ΔhtrA) clones, while htrA was detected in the H. pylori strain with S221A mutation (N6 htrAS221A) (Fig. 1AB and Fig. S2). The PCR products, amplified using H8-H9 primer pair and H. pylori N6 htrAS221A genomic DNA as a template, were PdiI digested and/or sequenced, which confirmed that in eight clones the htrA locus contained the 661T > G substitution introduced into htrA (Fig. 1C and Fig. S2). Finally, using two independent clones of each mutant type, we performed Southern blotting, which confirmed that recombination occurred at the desired locus in both N6 ΔhtrA and N6 htrAS221A strains and that no additional copy of htrA was present in the H. pylori wild-type or mutant strains (Fig. 1D).
Next, we performed western blotting and casein zymography analyses to confirm the presence or absence of HtrA in our H. pylori clones (Fig. 2). No HtrA protein was detected in the N6 ΔhtrA strain by the anti-HtrA antibodies. The corresponding protein lysate of this mutant did not show any proteolytic activity against casein. We also confirmed that the HtrAS221A variant, which was detected by western blotting in the H. pylori htrAS221A strain, showed no caseinolytic activity. Casein zymography also revealed that no detectable additional caseinolytic protease was present in the H. pylori N6 ΔhtrA strain. Thus, to summarize, all performed analyses confirmed that htrA was successfully deleted in H. pylori N6 ΔhtrA, while it was correctly exchanged for the mutated gene in H. pylori N6 htrAS221A.
Deletion or mutation of the htrA gene selects for suppressor mutations in the secA gene
N6 represents the only H. pylori strain, in which htrA was successfully inactivated thus far. These surprising findings raised questions about the uniqueness of this isolate, but also about possible suppressor mutations that might have been selected by inactivation of htrA. Since the full H. pylori N6 sequence is not available in the format allowing for extensive in silico analyses, and taking into account that our laboratory stock of N6 might have accumulated some spontaneous mutations upon passaging, we decided to sequence the entire genomes of the N6 ΔhtrA (clone 2) and N6 htrAS221A (clone 2) mutant strains and the corresponding parental wild-type strain.
Using OrthoVenn20, we compared the N6 wild-type encoded proteome with proteomes of 5 other fully sequenced H. pylori strains: 26695, J99, India7, Shi470, and HPAG1, which represent strains in which no htrA mutant was obtained. The analysis revealed that the N6 wild-type strain contained genes that were found in at least one of the 5 sequenced genomes (Fig. S3). Thus, there were no additional proteins (e.g., proteases) in the N6 wild-type strain that could have taken over the function of HtrA allowing for htrA deletion.
Next, we compared sequences of H. pylori N6 wild-type and mutant strains. We identified genetic variants in the H. pylori N6 htrAS221A and N6 ΔhtrA strains based on short reads mapping result. Surprisingly, in both strains we detected single missense mutations in the secA gene, 2522G > A or 2555G > A, which resulted in the C841Y or C852Y substitutions in the SecA protein, respectively. No other mutations were identified in any of the strains. To further confirm the presence of mutations, secA of H. pylori wild-type, N6 htrAS221A and N6 ΔhtrA were amplified by PCR using H10-H11 primer pair and sequenced by the Sanger method. Sequencing confirmed the presence of distinct mutations detected by NGS sequencing (Fig. 3). Additional Sanger sequencing of another clone of H. pylori N6 ΔhtrA (clone 1) and two other clones of N6 htrAS221A (clones 3 and 4) revealed other types of mutation, 2510G > A, 2529T > A and 2573C > T resulting in the SecA R837K, C843X and P858L mutant protein variants (Fig. 3). All five mutations are located within the C-terminal part of SecA, which in other bacteria is responsible for interaction with the SecB chaperone and Zn2+ binding21 (see Discussion). Finally, the secA gene sequences of the mutant strains were compared with worldwide H. pylori strains deposited in the RefSeq NCBI database. Remarkably, in a total of 645 H. pylori SecA sequences analyzed, similar mutations at the above positions do not occur and are unique to the N6 ΔhtrA and N6 htrAS221A clones (Fig. 3D). Hence, the presence of these mutations must be directly associated with a lack of the functional HtrA protease.
To better characterize the H. pylori double mutant strains, we analyzed growth of two independent clones of each htrA mutant type (ΔhtrA and htrAS221A), each containing a different secA mutation, and compared it to the growth of the wild-type strain and the complementation mutant ΔhtrA/htrAN6 that was derived from ∆htrAsecAR837K (clone 1), (for strain construction details see Methods, Supplementary Fig. S4 and Table S2). The analysis of growth curves and average generation time calculated for the first 24–27 hours of growth (i.e., characterizing both the lag phase and logarithmic phase of growth) showed that H. pylori ∆htrAsecAR837K and htrAS221AsecAP858Y grew similarly to the wild-type and ΔhtrA/htrAN6 strains, while the ∆htrAsecAC852Y htrAS221AsecAC841Y grew significantly slower (Fig. 4AB and Fig. S5). Since the two clones of each ΔhtrA or htrAS221A mutant type had the same htrA mutation but differed in secA mutation, the differences in growth rate were possibly caused by the type of the secA mutation. R837K and P858L mutations are possibly less harmful to H. pylori than C852Y and C841Y mutations. We also analyzed secA expression in each of the mutated strain. The secA expression level was lower in H. pylori mutants with retarded growth, while in mutants with undisturbed growth secA expression was similar to the wild-type and ΔhtrA/htrAN6 strains. To verify whether lower secA expression was not biased due to delayed growth, we analyzed expression of nifS, a gene encoding cysteine desulfurase - an enzyme unrelated to secretion system. The expression of nifS was similar in the wild-type and all mutant strains. Thus, we conclude that inactivation of htrA by deletion or mutation of its catalytic center is associated with two types of suppressor mutation in secA: 1/ affecting H. pylori growth and secA expression, and 2/ not affecting H. pylori growth and secA expression (both tested under optimal growth conditions). We did not find any mutation in the secA promoter regions in the two sequenced mutants ΔhtrAsecAC852 and htrAS221AsecAC841Y, each of which is characterized by retarded growth and reduced secA expression that could affect secA expression. However, we did not sequence chromosomes of strains, in which growth and secA expression were similar to the wild-type strain, thus we can’t exclude a second type or suppressor mutation. The molecular mechanism of growth retardation and secA expression reduction remains to be discovered. Nonetheless, our comprehensive analyses allowed to select ∆htrAsecAR837K or htrAS221AsecAP858L strains, which can be used for further HtrA studies without secondary effects of secA mutation. In our further phenotypic studies, we used derivatives of H. pylori N6 ∆htrAsecAR837K.
Inactivation of HtrA decreases bacterial transmigration across polarized epithelial cells
To assess the usefulness of the constructed H. pylori htrA mutant strains as novel tools to study the role of HtrA in the pathogenesis of H. pylori infections, we determined the transmigration rates by the H. pylori wild-type and mutated strains (Fig. 5). For this purpose, the polarized MKN28 cells were grown in a transwell filter system for 14 days to reach confluent monolayers. The cells were infected with H. pylori for 24 h in the apical chamber. Transmigrated bacteria were harvested from the bottom chamber, grown on GC agar plates, and the CFUs were determined (Fig. 5). The results show that after 24 hrs the number of transmigrated wild-type H. pylori bacteria were approx. 600 × 104. The number of transmigrated H. pylori N6 ΔhtrAsecAR837K bacteria were about 100 × 104 CFU and decreased by approximately 6-fold compared to the corresponding control H. pylori wild-type strain. As further controls, we analysed transmigration of H. pylori htrA complemented strain (N6 ΔhtrA/htrAN6) or a strain in which the htrA 661T > G mutated gene was introduced into htrA wild-type chromosomal locus (N6 ΔhtrA/htrAS221AN6) (both strains encode SecAR837K variant, see Methods, Supplementary Fig. S4, Fig. S6 and Table S2). The number of transmigrated H. pylori N6 ΔhtrA/htrAN6 bacteria were approx. 300 × 104 (Fig. 5). This indicated that wild-type htrA reintroduced into N6 ΔhtrA strain restored H. pylori transmigration ability to 50% of the corresponding wild-type strain. Transmigration of N6 ΔhtrA/htrAS221AN6 bacteria was similar to transmigration of N6 ΔhtrAsecAR837K, thus HtrAS221A protein variant cannot complement the htrA deletion in this process. The fully active complementation of N6 ΔhtrA was probably not possible due to the presence of a suppressor mutation in secA gene. Nonetheless, we could show that proteolytically active HtrA is important for H. pylori transmigration and that the constructed strains can be used as valuable tools in further studies on H. pylori HtrA.
Inactivation of HtrA does not affect bacterial host cell binding, but inhibits translocation and phosphorylation of CagA in polarized Caco-2 cells vs. non-polarized AGS cells
Next, we investigated if inactivation of the htrA gene may affect bacterial binding to host cells and translocation of CagA. For this purpose, non-polarized AGS cells in comparison to polarized Caco-2 cells were infected by the above described H. pylori strains for 6 hours using an MOI of 25 (Fig. 6). The results show that bacterial cell binding was very effective by H. pylori wild-type and was not inhibited by mutation of htrA (Fig. 6AB). Remarkably, translocation and phosphorylation of CagA were very high and similar between the strains in infected AGS cells (Fig. 6C), but deletion of htrA or infection with the protease-inactive ΔhtrA/htrAS221AN6 variant abolished this effect in polarized Caco-2 cells (Fig. 6D). Successful translocation and phosphorylation of CagA was accompanied by the induction of the elongation (hummingbird) phenotype in infected AGS cells (Fig. 6E), while this phenotype was not expressed in polarized Caco-2 cells, irrespectively of whether CagA was phosphorylated or not (Fig. 6F).
In the majority of bacterial species, mutations in the htrA gene are conditionally lethal only8. For example, Escherichia coli strains lacking the functional htrA (degP) gene cannot survive at temperatures exceeding 40 °C22 or under certain conditions of oxidative stress23. C. jejuni ΔhtrA strains are also sensitive to a combination of the oxidative and thermal stresses24,25. In H. pylori, in contrary to other bacterial species, we found that in only one of the 100 examined strains (N6) the htrA gene is dispensable for growth, which confirms the crucial role of htrA in this bacterium16. H. pylori lacking HtrA or with inactive HtrA exhibited reduced transmigration activity across polarized epithelial cells (Fig. 5). H. pylori binding to host cells was similar for the wild-type and mutant strains, while translocation of CagA by ΔhtrAsecAR837K and ΔhtrA/htrAS221AN6 mutants was significantly reduced in polarised Caco-2 cells in comparison to the wild-type or htrA-complemented strains (Fig. 6). Thus, we experimentally proved that HtrA is required for efficient H. pylori virulence connected with disruption of cell junctions. Successful construction of htrA mutant strains thus opens new research possibilities aiming at characterisation of the role of HtrA in H. pylori virulence and physiology (e.g., stress resistance).
However, deletion (N6 ΔhtrA) or mutation of the htrA gene (N6 htrAS221A) selected for suppressor mutations in the secA gene. It was previously shown that the HtrA variants deprived of serine at the active site are proteolytically inactive, but they retain the chaperone activity25,26. Thus, the similar types of suppressor mutations (C852Y, C841Y, C843X, P858L or R837K) detected in N6 ΔhtrA and N6 htrAS221A strains suggests that the proteolytic rather than chaperone activity of HtrA is essential for the H. pylori viability. Differences between H. pylori N6 and other strains, that allow the bacteria to survive without htrA, remain to be uncovered, but it should be noted that H. pylori is known for its high genetic variability between different species27,28. Thus, we suspected that H. pylori N6 may encode an additional protein (e.g. protease), which takes over the HtrA function in the htrA mutants. However, we couldn’t find any additional protease in N6 compared to other fully sequenced H. pylori genomes (Fig. S3). Alternatively, N6 may lack or produce fewer proteins, which may become toxic for H. pylori when accumulated in the periplasm of the ΔhtrA or htrAS221A mutants. The latter hypothesis may be supported by the fact that htrA deletion or inactivation of the HtrA proteolytic activity induced mutations in the secA gene, thus possibly affected periplasmic homeostasis when compared to the wild-type cells.
The SecA protein is a partner of the bacterial SecYEG translocon that exports proteins to extracytoplasmic locations29. The system has been merely studied in H. pylori thus far30,31,32,33, although it is presumably the major protein translocation system in this bacterium34,35. Moreover, the Sec translocon is involved in translocation of vacuolating cytotoxin A (VacA) – one other major H. pylori virulence factor36. Inhibition of SecA synthesis lowers secretion of VacA, thus SecA is indirectly involved in H. pylori pathogenesis30,31,32.
SecA performs a dual role in protein translocation: (1) acts as an ATP-dependent motor to move a given polypeptide across the membrane, (2) participates in recruitment and delivery of suitable substrates to the Sec transmembrane channel. SecA is involved in the post-translational pathway of secretion and its substrates are primarily periplasmic and outer membrane proteins. Substrates can be bound co-translationally directly by SecA or they are delivered by the SecB chaperone to SecA (reviewed in37). SecA is a large protein and it is composed of several domains38. All substitutions found in the secA gene in the ΔhtrA or htrAS221A background mapped to the 5′ region coding for the C-terminal domain, including a zinc-binding motif (Fig. 3). Mutations of cysteine residues, C852Y and C841Y, retarded H. pylori growth; these mutants also exhibited lower secA expression, possibly further reducing SecA activity in H. pylori cells (Fig. 4). Interestingly, in another bacterium, Acinetobacter baumanii, truncation of the C-terminal part of SecA resulted in a reduction of the secA transcript level (to 69% of that detected in the wt parental bacteria)39. Moreover, a model SecA protein from E. coli is known to negatively regulate its own translation by binding to its own RNA and blocking the ribosome binding site40. Therefore, we may expect that also H. pylori SecA controls its own cellular content, possibly at translation step, and certain disturbances in the C-terminal part of this protein may affect this process. However, we also detected secA mutations (R837K and P857L), which neither changed H. pylori growth nor secA expression. Thus, the molecular mechanism of growth retardation and reduction of secA expression remains to be discovered. Nonetheless, the question arises why htrA inactivation selects for specific mutations in C-terminal domain of SecA?
The exact role of this region in SecA is not fully understood to date. It is known that C-terminus of E. coli SecA, in particular zinc binding domain, is responsible for specific interactions with SecB21,41. However, it is important to note that this domain is well conserved also in bacteria lacking SecB chaperone (e.g., Bacillus subtilis or H. pylori) (Fig. 5C and33,42). Moreover, SecB is not required for viability of E. coli43, while a lack of functional SecA is conditionally lethal in these bacteria. The importance of the very C-terminal 70–75 amino acids in the functionality of the SecA is a subject of controversy. In the work of Breukink et al.44 it was shown that SecA lacking its C-terminal 70 amino acids was not able to suppress the lethality of the temperature sensitive secA mutation (secA51(Ts) or secA amber) at the non-permissive temperature. Na et al.45 demonstrated that the C-terminal 70–75 amino acids can be deleted from SecA without losing complementation activity in E. coli. This domain of E. coli SecA contains a zinc binding motif mentioned above, composed of three cysteines and one histidine residue. In the presence of Zn2+, the fragment adopts a zinc finger-like motif46. The C-terminal part is also implicated in interaction with the inner membrane (acidic phospholipids) and was proposed to play an autoregulatory role. The C-terminally truncated variants showed an increased ATPase activity in vitro44. It has been also suggested that the C-terminal domain could auto-inhibit SecA by competing for interaction with substrate proteins but the significance of this activity is not clear47.
Whatever function is played by the C-terminal part of SecA, its alterations resulted in poor growth and a protein secretion defect in E. coli. These included C-terminal protein truncation45 or cysteine to serine substitutions48. Hence, by analogy, we can hypothesize that the secA suppressor mutations of ΔhtrA or htrAS221A in H. pylori may lead to slowing down general protein translocation and, in consequence, lowering extracytoplasmic folding stress due to the absence or the lack of HtrA proteolytic activity. If this is the case, secA mutations in H. pylori would fall into place with suppression mutations detected in htrA mutants of other bacterial species. For example, in E. coli the majority of the compensatory (suppressor) mutations of the htrA temperature-sensitive phenotype lead to reduction of the envelope stress by either removal/release of HtrA substrates49,50,51,52 or by lowering synthesis of proteins that in the absence of HtrA may exert a proteotoxic effect on a bacterial cell51,53. Further studies are required to reveal the functional relationship between Sec translocon and HtrA in maintaining periplasm homeostasis. Interestingly, the cooperation of SecA and HtrA has been already suggested in S. pneumonia strain D397, in which, during exponential growth and cell division, these two proteins co-localize.
In summary, we constructed the first H. pylori ΔhtrA and htrAS221A mutant strains, which proved to be extremely valuable tools to study the role of HtrA in H. pylori virulence as demonstrated by the transmigration and CagA translocation assays. The suppressor mutations in secA detected in the htrA mutants suggest that lethality of htrA deletion/inactivation is caused by disturbed periplasmic homeostasis. The similar types of suppressor mutations coexisting with the htrA deletion or HtrA proteolytic activity inactivation indicates that the proteolytic rather than chaperone activity is essential for H. pylori survival. Hence, our results pinpointing a potential functional relationship between HtrA and the Sec translocon in H. pylori, together with previously reported cooperating between SecA and HtrA in S. pneumonia, possibly indicate more general mechanism responsible to maintain bacterial periplasmic homeostasis.
Materials, strains and culture conditions
All H. pylori strains tested in htrA gene mutagenesis are listed in the Supplementary Table S1, while H. pylori htrA mutants are listed in the Supplementary Table S2. The plasmids and E. coli bacterial strains used in this work are listed in the Supplementary Table S3. The oligonucleotide sequences are presented in the Supplementary Table S4. E. coli was grown at 37 °C on solid or liquid Luria-Bertani medium, supplemented with 50 µg/ml kanamycin where necessary. E. coli DH5α was used for cloning, while E. coli MC1061 was used for propagation of plasmids used to transform H. pylori. H. pylori was cultivated as described previously54 (for mutagenesis, DNA isolation or lysate preparation) or17 (for transwell migration studies). The liquid cultures were prepared in Brucella broth containing 10% fetal calf serum and antibiotic mix55. The growth of liquid cultures was monitored by measuring the optical density at 600 nm (OD600). Liquid cultures were set up by scraping H. pylori from blood agar plates by a sterile cotton swab and inoculating bacteria into Brucella broth pre-warmed to 37 °C to OD600~0.5 (OD600 = 1 corresponds to 1.4 × 109 CFU/ml). H. pylori cells were grown for approx. 12 hours and then sub-cultured to a fresh medium pre-warmed to 37 °C to OD600 = 0.005. H. pylori culture grown for 40–45 hours, while OD600 of the culture was measured every 3–4 hours in the period of approx. 13–26 hours of growth. Growth rate G was calculated using formula G = t/((log(N/N0))/log2) (t, time of growth; N0, number of bacteria at the beginning of the time interval, N, number of bacteria at the end of the time interval). H. pylori cells were transformed with purified plasmid DNA by natural transformation56. For selection of the H. pylori transformants, kanamycin (15 µg/ml) or chloramphenicol (8 µg/ml) were added to the medium.
In vivo H. pylori mutagenesis
N6 ΔhtrA and N6 htrAS221A
The H. pylori 26695 genomic DNA served as a template in PCR reactions performed to prepare plasmids used to construct the mutants with chromosomal deletion of htrA or the mutation of htrA (661T > G) resulting in the synthesis of proteolytically inactive HtrAS221A. The regions flanking htrA were amplified by PCR using two pairs of primers complementary to the upstream (rocE fragment) and downstream (ispDF fragment) regions of htrA: H1-H2 and H3-H4, respectively. The resulting fragments and the non-polar aphA-3 kanamycin resistance gene cassette57, cut out from the pILL2283 plasmid using BamHI-PstI restriction enzymes, were amplified by H1-H4 primer pair, digested by NdeI-EcoRI restriction enzymes and inserted into the NdeI-EcoRI sites of the pUC18 vector giving rise to plasmid pUZ16 (S3 Table). The pUZ16 plasmid was used to delete htrA from its native locus or it was further used as a cloning vector to prepare pUZ17.
To prepare pUZ17, htrA was amplified using H12-H13 primer pair and cloned into pUC19 digested by SmaI, giving pHJS3. The pHJS3 plasmid was used as a template to replace the codon of serine S221 with alanine by site-directed mutagenesis according to the standard protocol of the Quick- Change Mutagenesis Kit (Agilent) using H14- H15 primer pair and giving pUZ1. In parallel, htrA was amplified by PCR using H6-H7 primer pair. The PCR product was digested by NdeI-BamHI and cloned into pUZ16 digested by the same restriction enzymes giving pUZ18. Subsequently, by standard cloning, the SphI - AgeI fragment of htrA was exchanged for homologous htrA fragment containing 661T > G mutation, excised from pUZ1 by the same restriction enzymes, giving the final pUZ17 vector. The presence of 661T > G mutation introduced the PdiI restriction site into htrA, thus PdiI digestion was used to distinguish pUZ18 from pUZ17. H. pylori N6 was transformed with the pUZ16 or pUZ17 and plated on the BA plates supplemented with kanamycin. The colonies resistant to kanamycin were isolated and then analyzed by PCR, Southern blot, DNA sequencing, western blot, and casein zymography to prove that the proper H. pylori htrA deletion mutant (N6 ΔhtrA) or the mutant synthesizing HtrAS221A mutant protein (N6 htrAS221A) were obtained.
N6 ΔhtrA/htrA N6
A three-step strategy was used to generate a complementation strain of the H. pylori htrA deletion mutant strain, that contained the re-introduced wild-type htrA gene in its native position within the genome (Fig. S4). First, the three DNA fragments were amplified using the following primer pairs: H1-H16 for rocE-htrA, H17-H4 for ispDF and H18-H19 for chloramphenicol cassette (cat). The H. pylori N6 wild-type genomic DNA served as a template in PCR for the rocE-htrA and ispDF fragments, while pILL2150 served as a template for the cat cassette. Next, the resulting fragments were amplified by H1-H4 primer pair and the full-length fusion PCR product (approximately 0.8 µg) was used to transform the H. pylori N6 ΔhtrAsecAR837K strain (Table S2). After antibiotic selection, correct integration of the htrA gene was verified by sequencing. Expression of the HtrA protein and its ability to digest casein was checked in the selected H. pylori N6 ΔhtrA/htrAN6 clones using western blotting and zymography, respectively.
A multistep strategy was used to generate a complementation strain of the H. pylori htrA deletion mutant strain, that contained the re-introduced mutated htrA 661T > G gene in its native position within the genome (Fig. S6). First, pUZN10 and pUZN11 were generated to prepare a mutated version of H. pylori N6htrA 661T > G. htrA was amplified using H22-H23 primer pair and H. pylori N6 genomic DNA, cloned into pET26b digested by NcoI-XhoI, giving pUZN10. The pUZN10 plasmid was used as a template to replace the codon of serine S221 with alanine by site-directed mutagenesis according to the standard protocol of the SapphireAmp Fast polymerase (Takara) using H24- H25 primer pair and giving pUZN11. Next, the three DNA fragments were amplified using the following primer pairs: H1-H21 for rocE-htrA, H20-H16 for htrA 661G > T, and H18-H4 for cat-ispDF. The H. pylori N6 wild-type genomic DNA served as a template in PCR for the rocE-htrA, N6 ΔhtrA/htrAN6 for cat-ispDF, while pUZN11 served as a template for the htrA 661T > G. Next, the resulting fragments were amplified by H1-H4 primer pair and the full-length fusion PCR product (approximately 0.8 µg) was used to transform the H. pylori N6 ΔhtrAsecAR837K strain (Table S2). Selection and analysis of H. pylori N6 ΔhtrA/htrAS221AN6 clones were done as described for N6 ΔhtrA/htrAN6.
H. pylori mutant deficient in the cagY (virB10) gene of the type IV secretion system was constructed as described58.
Southern blot was performed as described59. Briefly, 10 μg of H. pylori genomic DNA and 10 ng of a control plasmid DNA isolated from E. coli, digested with HindIII, were resolved in 1% agarose gel. DNA was transferred onto a nylon membrane and incubated at 68 °C with digoxigenin-labeled DNA probe (431 bp DNA, amplified with primers H8-H9). Southern blot was developed by a colorimetric reaction using anti-digoxygenin antibody (Anti-Digoxigenin-AP, Fab fragments, Roche).
SDS-PAGE, western blotting and Casein zymography
SDS-PAGE and western blotting were described elsewhere59,60. For western blotting, proteins were transferred onto PVDF membranes (Immobilon-P, Merck Millipore). All steps were carried in TBS-T buffer (140 mM NaCl, 25 mM Tris- HCl, pH 7.4, 0.1% Tween- 20). The membranes were blocked with 5% non-fat milk or 3% BSA (for detection of phosphorylated CagA). Non-phosphorylated and phosphorylated CagA protein species were detected using the rabbit polyclonal α‐CagA antibody (# HPP‐5003‐9, Austral Biologicals, San Ramon/USA) and α-PY‐99 antibody as described61. A monoclonal mouse antibody against GAPDH (# sc‐20357, Santa Cruz) expression was applied as a loading control. HtrA was detected by using polyclonal rabbit anti-HtrA antibodies followed by the secondary goat anti-rabbit polyvalent, horseradish peroxidase-conjugated IgGs (catalogue number #31462, Life Technologies, Darmstadt/Germany). Anti-HtrA antibodies were raised in rabbit against the purified recombinant H. pylori HtrA. Experimental procedures were conducted according to the Interdisciplinary Principles and Guidelines for the Use of Animals in Research, Marketing and Education issued by the New York Academy of Sciences’ Ad Hoc Committee on Animal Research, and Directive 2010/63/UE of the European Parliament and of the Council of 22 September 2010 on the protection of animals used for scientific purposes. All experiments were approved by the First Local Committee for Experiments with the Use of Laboratory Animals, Wroclaw, Poland (permission number 50/2015). Casein zymography was performed as described16.
Human cell culture
The non-polarized human gastric adenocarcinoma cell line AGS (ATCC CRL‐1739™) was cultured in RPMI 1640 medium containing 2 mM L‐glutamine (Invitrogen, Karlsruhe/Germany) and 10% heat‐inactivated fetal calf serum (FCS; Gibco, Paisley/UK). Caco-2 (ATCC HTB‐37) represents a polarized human colon adenocarcinoma cell line and was cultured in Dulbecco’s Modified Eagle Medium (DMEM) supplemented by 110 mg/L sodium pyruvate, 4.5 g/L D‐glucose, 4 mM L‐glutamine and 10% FCS. The human cell line MKN28 was kindly provided by Motomo Kuroki (Fukuoka University/Japan) and is phenotypically different from the MKN28 cell line available from the JCRB cell bank (number 0253) described previously14,62. These cells were cultured in Eagle’s minimum essential medium (Sigma‐Aldrich) with 10% FCS. All cell lines were generally supplemented with 1% antibiotic and antimycotic solution (Sigma‐Aldrich) and grown in incubators with 5% (v/v) CO2 at 37 °C. Subculturing was performed at a ratio of 1:3 to 1:5 at a confluence of 70 to 90% every 2 to 3 days. Every cell line was cultured in 75 cm2 tissue culture flasks and subculturing in 6-well plates (Greiner‐Bio‐One, Germany), and washed with antibiotics-free medium before infection.
Cell binding and elongation assay
Infection of non-polarized AGS cells (80% confluence) and confluent polarized Caco-2 monolayers was performed in triplicates on six‐well plates63. After 6-hour co-incubation with the different indicated H. pylori strains at MOI of 25, infected cells were rigorously washed three times using 1 mL of pre-warmed culture medium (without antibiotics) to remove non-bound H. pylori. For quantification of cell‐bound bacteria as colony forming units (CFU), the cells were incubated with1 mL of buffer (PBS containing 0.1% saponin) for 15 min at 37 °C as described64. The resulting suspensions were diluted in serial steps and incubated on GC agar plates for 5 days, followed by quantification of the number of CFUs. The number of elongated cells after infection was done as described previously65. For western blotting cells were collected as described61.
Transwell infection studies
Transwell infection studies were done as described earlier17. For this purpose, the cells were cultured on 0.33 cm2 cell culture inserts (with 3 μm pore size). The cells were grown to confluent monolayers and then incubated for another 14 days to allow cell polarization. The cells were infected in the apical compartment at MOI of 50 in a time course and the numbers of transmigrated bacteria were quantified in aliquots taken from the basal chambers and counting CFUs on GC agar plates after 5 days of incubation.
Sanger sequencing of DNA fragments was performed by Genomed SA (Poland) or GATC Biotech (Germany). Next generation sequencing was performed by Biobank Lab, University of Lodz (Poland) and FAU Erlangen (Germany). The genome of H. pylori N6 wt was sequenced on Illumina NexSeq. 500 (Lodz), Illumina MiSeq (Germany) and ONT (Oxford Nanopore Technologies) MinION single molecule sequencing platform (Lodz). The genomes of H. pylori ΔhtrA and htrAS221A strains were sequenced on Illumina NextSeq500 (Lodz) and Illumina MiSeq (Germany). Short reads libraries for all samples were prepared with the Nextera XT kit, in accordance with the manufacturer’s instruction (Illumina, San Diego, USA). Libraries for ONT MinION platform were prepared with ONT Rapid Sequencing Kit (SQK-RAD004, Oxford, UK). Illumina sequencing was performed at a reads length 2 × 150 bp for NextSeq platform and 2 × 300 bp for MiSeq.
RNA was extracted from three independent sets of H. pylori cultures in the logarithmic phase of growth (OD600 ~ 0.4–0.7). RNA was extracted using a Total RNA Extraction Plus kit (A&A Biotechnology) according to the manufacturer’s protocol, and further treated with RNase-free DNAseI (Thermo Scientific). Reverse transcription (RT) reactions were carried out on 0.5 μg of total RNA in 20 μl using Maxima Reverse Transcriptase (Thermo Scientific) and random hexamer primers in the presence of RiboLock RNase Inhibitor (Thermo Scientific), as described by the manufacturer. mRNA levels of the selected H. pylori genes were quantified by qPCR, performed on a CFX96 Touch Real-Time PCR Detection System (BioRad) using SensiFAST SYBR No-ROX (BioLine) and the following parameters: 96 °C for 2 min, followed by 40 three-step amplification cycles consisting of 5 s at 96 °C, 10 s at 60 °C and 10 s at 72 °C. Reaction mixtures (15 µl) contained qPCR mix (7.5 μl), cDNA (1 μl of 50x diluted RT reaction) and primers (0.3 µM each). The following primer pairs were used: secA, H28-H29; nifS, H30-H31 and 16SrRNA, H32-H33. The relative quantity of mRNA for each gene was determined by reference to the mRNA levels of H. pylori 16SrRNA.
In silico analysis
Illumina raw reads were quality and length trimmed with Trim Galore! v. 0.4.5 (https://www.bioinformatics.babraham.ac.uk/projects/trim_galore/). Trimmed data from Illumina and Nanopore sequencing of H. pylori N6 wild-type strain were used to prepare high contiguity reference genome of starting strain. De novo assembly of H. pylori N6wt was prepared with SPAdes 3.1066 hybrid assembly option. Gene annotation was done with Prokka v. 1.1267. Reads mapping and variant calling versus earlier prepared reference genome of H. pylori N6wt was performed with CLC Genomics Workbench v. 8.5.1 and Snippy v. 3.2 (Snippy 9, https://github.com/tseemann/snippy). The massive deletion was identified by visualization mapped reads in IGV v. 2.4.068 and analysis of the obtained image.
Equipment and settings
DNA/protein electrophoresis and chemiluminescent western blot results were documented by the Gel Doc™ XR+ System or ChemiDoc XRS+ and processed by Image Lab software. RT-qPCR was performed using CFX96 Real-Time System and CFX manager software. The images were prepared for publication by CorelDRAW and CorelPHOTO-PAINT software. Digital processing was applied equally across the entire image, including controls.
Statistical data analysis
Each experiment was performed independently for at least three times with similar results. The data were evaluated using the Student’s t‐test with SigmaPlot statistical software (version 13.0) or Excell 2016.
This Whole Genome Shotgun projects (Bioproject PRJNA505142) have been deposited at DDBJ/ENA/GenBank under the accession numbers: SAMN10411099 (N6 wild-type strain), SAMN10411397 (N6 ΔhtrA) and SAMN10411398 (N6 htrAS221A). The version described in this paper is version SAMN01000000.
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D.S. and J.L. was supported by the Polish Ministry of Science and Higher Education grant DIR/WK/2017/01. J.S.G., U.Z. were supported by the National Science Centre grant UMO-2016/21/B/NZ2/01775. A.Z.P. was supported by by research grant SONATA BIS3 from the National Science Centre (DEC-2013/10/E/NZ1/00718). The work of N.T. is supported by the German Science Foundation (DFG project TE776/3-1). We thank Armin Ensser (FAU Erlangen/Germany) for his support with the NGS sequencing.
The authors declare no competing interests.
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Zawilak-Pawlik, A., Zarzecka, U., Żyła-Uklejewicz, D. et al. Establishment of serine protease htrA mutants in Helicobacter pylori is associated with secA mutations. Sci Rep 9, 11794 (2019) doi:10.1038/s41598-019-48030-6
Chaperone activity of serine protease HtrA of Helicobacter pylori as a crucial survival factor under stress conditions
Cell Communication and Signaling (2019)