Helicobacter pylori Infection Aggravates Dysbiosis of Gut Microbiome in Children With Gastritis

Introduction

Helicobacter pylori is a well-known pathogen in chronic gastritis, peptic ulcer, and gastric cancer (Marshall and Warren, 1984), usually acquired in early childhood, mostly before the age of 5 (Weyermann et al., 2009; O'Ryan et al., 2015). This infection causes a persistently chronic and low degree of inflammatory response in gastric and duodenal mucosa, which may persist lifelong without treatment. H. pylori infection is strain dependent and determined by its association with cytotoxic gene A (cag A) (Wang et al., 2016), bacterial characteristics, inflammatory response, host conditions, and environmental factors. China has a high prevalence of H. pylori infection. The infection rate is currently 40–60%, reaching as high as 37.1% before 20 years of infection stage. Early diagnosis and treatment can, therefore, prevent H. pylori-related complications (Sugano et al., 2015; Malfertheiner et al., 2017). The European and North American Societies for Pediatric Gastroenterology, Hepatology and Nutrition recommends the use of triple therapy, including proton pump inhibitors (PPIs) in combination with amoxicillin and either imidazole or clarithromycin, as the first line of treatment for H. pylori eradication in children (Koletzko et al., 2011). However, successful eradication is lower in children owing to poor drug compliance and antibiotic resistance displayed by H. pylori (Oderda et al., 2007; Okuda et al., 2017). Meta-analyses from previous studies have revealed that triple therapy supplemented with probiotics increased the eradication rate while decreasing the adverse reactions of triple therapy in H. pylori infection, especially in children (Szajewska et al., 2010; Li et al., 2014). An understanding of how the gastrointestinal microbiome interacts with H. pylori during infection might provide novel targets for its prevention and treatment in children.

Recent studies focusing on gastric microbiome showed that the interaction between H. pylori and other microbes may play a pivotal role in H. pylori-associated diseases (Bik et al., 2006; Schulz et al., 2015; Alarcon et al., 2017; Brawner et al., 2017; Llorca et al., 2017). Gastric microbiome is mainly represented by four phyla (Proteobacteria, Bacteroidetes, Firmicutes, and Actinobacteria) in the general population, and remarkable changes in gastric microbiome composition were observed between H. pylori-positive and H. pylori-negative individuals (Maldonado-Contreras et al., 2011; Alarcon et al., 2017). Positive H. pylori status was associated with increased abundance of proteobacteria, especially epsilonproteobacteria, mainly because of Helicobacter genus. An increased abundance of Spirochetes and Acidobacteria was also observed, with decreased abundance of Actinobacteria, Bacteroidetes, and Firmicutes (Maldonado-Contreras et al., 2011). Similar results were reported in H. pylori-infected children, presenting a higher relative abundance of Helicobacter genus (66.3%) than in H. pylori-negative children (0.45%) and lower bacterial diversity (Brawner et al., 2017; Llorca et al., 2017). Dysbiosis of gastric microbiota and some specific bacteria were found to be associated with gastric carcinoma or precancerous lesions (Coker et al., 2018; Ferreira et al., 2018). Notably, H. pylori played a crucial role in carcinogenesis. Some studies also suggested that the interaction between Lactobacillus, Streptococcus, and H. pylori enhances gastric inflammation and promotes H. pylori-associated carcinogenesis (Aviles-Jimenez et al., 2014; Rizzato et al., 2019).

For resident microorganisms, the host is a unique entity along the gastrointestinal tract, and any change in these factors would modify homeostasis. As mentioned above, the role of H. pylori infection on the gastric microbiome and the interaction in associated gastric diseases has been highlighted in recent studies. The interaction between H. pylori and gut microbiota has also been analyzed, although the exact underlying mechanism still remains unclear. Hypochlorhydria and hypergastrinemia caused by H. pylori infection were some of the causes in the interaction between H. pylori infection and gut microbiota (Beasley et al., 2015; He et al., 2016). Leptin and ghrelin secretion decreased in H. pylori-positive patients and indirectly also influenced the gastrointestinal microenvironment by modulating gastric acid secretion and immune response (La Cava and Matarese, 2004; Baatar et al., 2011; Francois et al., 2011; Muhsen et al., 2015; He et al., 2016). The plasma ghrelin level also significantly correlated with several kinds of bacteria, including Bifidobacterium and Bacteroides. Additionally, increased immune reaction caused by H. pylori infection is related to the genes in gastric and pulmonary tissues (Kienesberger et al., 2016). Animal studies have indicated that H. pylori results in distinct shifts in gut microbiota in distal, uninflamed parts of the gastrointestinal tract (Heimesaat et al., 2014). Similarly, several researches of human fecal samples on the relationship between H. pylori and intestinal flora also suggested a different composition of gut microbioma (Buhling et al., 2001; Myllyluoma et al., 2007; Chen et al., 2018; Gao et al., 2018; Iino et al., 2018). Some of the literatures we referred to focused on the changes of gut microbiome before and after treatment (Buhling et al., 2001; Myllyluoma et al., 2007; Chen et al., 2018). Myllyluoma et al. concluded that the concentration of clostridia and the total numbers of anaerobes significantly decreased in H. pylori-positive ones, compared with H. pylori-negative ones (Myllyluoma et al., 2007). Chen et al.'s study mainly focused on the impact of H. pylori eradication treatment using triple therapy. They also first compared the two groups on day 0 and observed significant increase in alpha diversity of H. pylori-positive fecal samples compared with H. pylori-negative subjects (Chen et al., 2018). Additionally, a Japanese study of 1,123 adult subjects, using 16S rRNA amplification from fecal samples, also confirmed higher abundance of Lactobacillus in H. pylori-infected subjects with severe atrophic gastritis (Iino et al., 2018). However, there has been only one study related to fecal microbiota and H. pylori infection in children, which included 18 fecal samples from five Japanese families (Osaki et al., 2018). These indicated a similar composition of intestinal microbiota between members of the same family, but the sample size was small. The relationship between H. pylori, gastritis, and gut microbiome variation has scarcely been analyzed (Chen et al., 2018; Gao et al., 2018), especially in children. In this study, fecal microbiome in children with H. pylori-positive gastritis group (HPG), H. pylori-negative gastritis group (HNG), and healthy control group (HCG) were compared before treatment using 16S rRNA gene sequence to confirm the impact of H. pylori infection and gastritis on gut microbiome. The results from this study may be useful in further evaluation of H. pylori infection, prevention, and treatment in children.

Materials and Methods

Study Design and Participants

This prospective pilot study, which was approved by the Institutional Review Boards at Qilu Children's Hospital of Shandong University (IRB# QLCH-ET-2017-06), collected samples from January 2017 to August 2017. Written informed consent and questionnaires were obtained from all subjects (children and legal guardians) visiting the outpatient gastroenterology unit at the Qilu Children's Hospital. They agreed to serve as fecal donors, in compliance with national legislation and the Code of Ethical Principles for Medical Research Involving Human Subjects of the World Medical Association (Declaration of Helsinki). For this study, children with symptoms of dyspepsia, aged 4 to 14 years, were recruited. All children were from the same geographical area. All symptomatic cases underwent ¹³C-urease breath test, abdominal ultrasonography, rapid urease test (RUT), endoscopy, and histopathological examination of gastric biopsy samples. Patients with gastritis indicating positive histopathology and RUT were diagnosed with Helicobacter pylori infection for the first time and were then divided into HPG, whereas those with negative histopathology and RUT results were divided into the HNG (Koletzko et al., 2011; Jones et al., 2017). When one of the histopathology and RUT results is negative, it can be combined with other test results, such as ¹³C-urease breath test. The exclusion criteria screened out patients with duodenal or gastric ulcers; active gastrointestinal bleeding; previous eradiation failure; or history of gastric surgery or drug therapy with antibiotics, probiotics, or gastric acid-suppressing drugs in the preceding 4 weeks. Also, healthy children (volunteers) from the same geographical area with matching age and sex composition as the other groups constituted the control group. They were all healthy with no known family history of digestive disease and medication for gastric disorders. Their ¹³C-urease breath test results were negative (Figure 1). Data were collected by using a standardized questionnaire including basic information, medical history, family history, and examination results.

FIGURE 1

Figure 1. Flowchart of this study. 210 children with dyspeptic symptoms and 64 healthy children were initially screened for the study. Ninety-five individuals refused to donate fecal samples, and another 15 children had oral drug history. They all had been excluded. In the second part of the tests, five patients refused to continue all the tests, and another three patients with the gastrointestinal ulcers and/or bleeding were missed. In the healthy children group, one fecal specimen of the child was missing, and another child with oral drug history was ruled out.

Sample Collection, DNA Extraction, and Sequencing

Fecal specimens were collected with sterilized 2-ml tubes containing pure ethanol on ice, immediately frozen (within 30 min), and stored at −80°C until analysis. Genomic DNA was extracted using cetyl trimethylammonium bromide (CTAB) method (Wang X. et al., 2018). An equivalent of 1 μl of each sample was used for DNA quantification using NanoDrop 2000 (Thermo Scientific). To analyze the bacterial population and amplification of the variable region, V1–V2 of the 16S rRNA gene was performed. PCR was conducted using bacterial universal primers 27F (5′AGAGTTTGATCMTGGCTCAG3′) 355R (5′GCTGCCTCCCG TAGGAGT 3′). The PCR products were checked using electrophoresis in 1% (w/v) agarose gels in TBE buffer (Tris, boric acid, and EDTA) stained with Genecolour I™ (Gene-bio) and visualized under UV light. Amplicons were first purified using the QIA quick PCR Purification Kit (Qiagen, Barcelona, Spain), quantified using a NanoDrop 2000 (Thermo Scientific), and then pooled in equal concentration. Pooled amplicons (2 nM) were then subjected to sequencing, using Illumina HiSeq 2500, following standard Illumina platform protocols.

Analysis of 16S rRNA Gene Sequence

The 16S rRNA gene sequence paired-end data set was joined and quality filtered using the FLASH method. All sequence analyses were conducted in the Quantitative Insights Into Microbial Ecology (QIIME, version 1.9.1) software suite (Caporaso et al., 2010), as per the QIIME tutorial (http://qiime.org/). Chimeric sequences were removed using usearch61 with de novo models. Sequences were clustered against the 2013 Green genes (13_8 release) ribosomal database, 97% reference data set. Sequences that did not match any entries in this reference were subsequently clustered into de novo operational taxonomic units (OTUs) at 97% similarity with UCLUST. Taxonomy was assigned to all OTUs using the RDP classifier within QIIME and the Greengenes reference data set (Cole et al., 2009).

Statistical Analysis

The questionnaires were analyzed using SPSS version 15.0 (SPSS Inc, Illinois, USA). There was no significant difference in age, sex, and indication for endoscopy between the groups (Table 1). To account for any bias caused by uneven sequencing depth, the least number of sequences present in any given sample was selected randomly from a sample category, prior to calculating community-wide dissimilarity measures (alpha diversity and beta diversity). The OTU table was then rarified to a sequencing depth of 22,000 per sample, for both diversity analyses. All principal coordinate analyses (PCoAs) were based on unweighted and weighted UniFrac distances, using evenly sampled OTU abundances. Linear discriminant effect size (LEfSe) analysis was performed to find features (taxa) differentially represented between patients and healthy controls. LEfSe combines Kruskal–Wallis test or pairwise Wilcoxon rank-sum test with linear discriminant analysis (LDA). It ranks features by effective size, which explains most of the biological differences at the top. LEfSe analysis was performed on the basis of the threshold of logarithmic LDA score for discriminative features, which is equal to 2.0. The effects of each of the two factors, that is, age and gender on the validated biomarkers, were examined within each of the two clinical categories by SPSS, in one-way ANOVA test. The effects were considered significant if P-value was < 0.05. The prediction of the functional composition of a metagenome, using marker gene data and a database of reference genomes, was done with Phylogenetic Investigation of Communities by Reconstruction of Unobserved States (PICRUSt) (Langille et al., 2013). The graphical representation of the results was done with R (McMurdie and Holmes, 2013) and STAMP. The calculation of P-values was done with Kruskal–Wallis H-test and Welch's t-test. Differences were considered significant when P < 0.05.

TABLE 1

Table 1. Demographic and clinical characteristics of the patients.

Results

Demographic and Clinical Characteristics of Subjects

210 children with dyspeptic symptoms and 64 matched healthy children were initially screened for the study. One hundred individuals refused to participate, and 19 children were ruled out, and one fecal specimen was missing. Around 154 individuals were involved (Figure 1 and Table 1), comprising 50 children in HPG (mean age at 8.27 ± 2.8 years, 22 girls and 28 boys). Forty-two children with gastritis, excluding Helicobacter pylori infection, were included in HNG (mean age at 8.64 ± 2.35 years, 12 girls and 30 boys), whereas 62 healthy children (mean age at 8.41 ± 1.17 years, 26 girls and 36 boys) were included in HCG. Fecal specimen and questionnaires were collected from all subjects.

The Diversity of Gut Microbiome in Three Groups of Children

We compared the richness (abundance-based coverage estimator [ACE]) and diversity (Shannon) of bacterial community among HNG, HPG, and HCG (Figure 2). There were no significant differences in Shannon and ACE index in the comparison of three groups, except for ACE index in comparing HNG and HCG (P = 0.0042, Figure 2A).

FIGURE 2

Figure 2. Comparison of alpha diversity (A, Shannon index; and B, ACE index) based on the OTU profile. HPG, HNG, and HCG are colored in red, blue, and green, respectively. The P-value was calculated by the Wilcoxon rank-sum test. HPG, Helicobacter pylori-induced gastritis group; HNG, H. pylori-negative gastritis group; HCG, healthy control group; OUT, operational taxonomic unit.

We also evaluated beta diversity among the three groups using PCoA, on the basis of the unweighted UniFrac distances. The PCoA demonstrated clustering of microbial communities between HNG and HPG (Figure 3A), HCG and HNG (Figure 3B), and HCG and HPG (Figure 3C). We used analysis of similarities (ANOSIM) to test whether two groups are significantly different in PCoA. Results indicated that there was a significant difference in gut microbiome structure between HNG and HPG (P = 0.002, R = 0.055, ANOSIM), HCG and HNG (P = 0.001, R = 0.178, ANOSIM), and HCG and HPG (P = 0.001, R = 0.187, ANOSIM).

FIGURE 3

Figure 3. PCoA of bacterial beta diversity based on the unweighted UniFrac distance. (A) Between HPG and HNG. (B) Between HNG and HCG. (C) Between HPG and HCG. PCoA, principal coordinate analysis; HPG, Helicobacter pylori-induced gastritis group; HNG, H. pylori-negative gastritis group; HCG, healthy control group.

Composition of Gut Microbiome of Children in All Three Groups

In the relative taxon abundance of groups, using 97% as the similarity cutoff, 605 qualified taxa were identified. At the phylum level, the gut microbiome profiles in the three groups of subjects were dominated by Bacteroidetes (HPG 51.37 ± 16.15%, HNG 50.71 ± 18.34%, and HCG 44.07 ± 14.68%), Firmicutes (HPG 35.65 ± 11.92%, HNG 35.16 ± 14%, and HCG 46.54 ± 13.78%), Proteobacteria (HPG 11.53 ± 12.13%, HNG 12.32 ± 9.49%, and HCG 8.09 ± 5.62%) (Figure 4A) (Caporaso et al., 2010; Langille et al., 2013; McMurdie and Holmes, 2013). Phylum level analysis also demonstrated the ratios of Firmicutes/Bacteroidetes (F:B), which had dramatically decreased in HPG (P = 0.012) and HNG (P = 0.0039), as compared with HCG. However, there was no difference between HPG and HNG in F:B ratio, implying that the bacterial community in fecal microbiome may alter in the disease state. At the genus level, Bacteroides (HPG 38.03 ± 17.47%, HNG 37.47 ± 17.81%, and HCG 30.18 ± 15.26%) and Prevotella (HPG 9.41 ± 14.96%, HNG 9.17 ± 15.1%, and HCG 11.45 ± 16.58%) were the major genus. There was also increased abundance of Bacteroides and Parabacteroides, decreased abundance of Roseburia and Faecalibacterium in HPG and HNG, compared with HCG (Figure 4B). Additionally, the Venn diagram shows 104 common OUTs of bacteria among the three groups (Figure 4C). There are four, three, and one unique OTUs for HNG, HPG, and HCG, respectively.

FIGURE 4

Figure 4. Comparison of relative taxa abundance between HPG, HNG, and HCG. (A) Comparison of relative taxa abundance among HPG, HNG, and HCG at the phylum level. (B) Comparison of relative taxa abundance among HPG, HNG, and HCG at the genus level. (C) Venn diagram. HPG, Helicobacter pylori-induced gastritis group; HNG, H. pylori-negative gastritis group; HCG, healthy control group.

Differential Taxonomic Abundance in Three Groups of Children

We applied LEfSe analysis to further identify the significantly different abundance between HNG and HPG, HCG and HNG, and HCG and HPG. Results revealed 13 taxa, distinguishing the gut microbiome communities with HNG and HPG, using an LDA score of above 2 (Figure 5A). There were 59 taxa each, distinguishing the gut microbiome communities with HCG and HNG (Figure 5C) and HCG and HPG (Figure 5D), respectively. A cladogram (Figures 5B,E,F) was used to represent predominant bacteria and the structure of the microbiota in each group. To assess the impact of H. pylori on the gut microbiome in children, the fecal microbiome in HPG and HNG was analyzed (Figure 5A). There was a higher abundance of Betaproteobacteria and Lactobacillales and lower abundance of Alphaproteobacteria in HPG. At the family and genus levels, higher abundance of Streptococcus and Collinsella and lower abundance of Pseudomonadaceae, Erysipelotrichaceae, and Megasphaera were found in HPG, as compared with HNG. Additionally, the compositions of gut microbiome between HNG and HCG were compared to analyze the altered gut microbiome in gastritis. An abundance of Bacteroidaceae, Enterobacteriaceae, Porphyromonadaceae, Fusobacteriaceae, and Megasphaera was seen in HNG. However, a higher abundance of Ruminococcaceae, Lachnospiraceae, Bifidobacteriaceae, Roseburia, Lactobacillus, Sutterella, and Bifidobacterium were found in the HCG (Figure 5C). The compositions of gut microbiome in children, HPG, and HCG were also compared and analyzed. Significant differences in taxa from phylum to genus level were represented in LDA. At the family and genus levels, Bacteroidaceae, Enterobacteriaceae, Porphyromonadaceae, Bacteroides, Parabacteroides, Streptococcus, and Lactococcus numbers increased significantly in HPG (Figure 5D). Lastly, the compositions of gut microbiome in HNG and HCG, and HPG and HCG were compared at five significant bacterial levels. There was significantly higher abundance of Bacteroidaceae and Enterobacteriaceae and lower abundance of Bifidobacteriaceae, Lactobacillaceae, and Lachnospiraceae in HPG and HNG, compared with HCG (Figures 5G–K). Thus, these results imply that gastric inflammation significantly changes the composition of gut microbiome, especially in children with H. pylori-induced gastritis.

FIGURE 5

Figure 5. Characteristics of microbial community composition in HPG, HNG, and HCG. (A) The most differentially abundant taxa between HPG and HNG (LDA score above 2), which was generated from LEfSe analysis. (B) The enriched taxa of fecal microbiome in HPG and HNG are represented in the cladogram. The central point represents the root of the tree (bacteria), and each ring represents the next lower taxonomic level (phylum to genus: p, phylum; c, class; o, order; f, family; g, genus). (C) The most differentially abundant taxa between HNG and HCG (LDA score above 2), which was generated from LEfSe analysis. (D) The most differentially abundant taxa between HPG and HCG (LDA score above 2), which was generated from LEfSe analysis. (E) Enriched taxa of fecal microbiome in HNG and HCG are represented in cladogram. The central point represents the root of the tree (bacteria), and each ring represents the next lower taxonomic level (phylum to genus: p, phylum; c, class; o, order; f, family; g, genus). (F) The enriched taxa of fecal microbiome in HPG and HCG are represented in cladogram. The central point represents the root of the tree (bacteria), and each ring represents the next lower taxonomic level (phylum to genus: p, phylum; c, class; o, order; f, family; g, genus). (G–K) Relative abundances of five bacteria (Bacteroidaceae, Enterobacteriaceae, Bifidobacteriaceae, Lactobacillaceae, and Lachnospiraceae) among HPG, HNG, and HCG were compared. HPG, Helicobacter pylori-induced gastritis group; HNG, H. pylori-negative gastritis group; HCG, healthy control group; LDA, linear discriminant analysis; LEfSe, linear discriminant effect size.

Predictive Function of Gut Microbiome in Three Groups of Children

We also explored microbiota function on the basis of inferred metagenomes using the PICRUSt algorithm. We compared the differences between HNG and HPG, HCG and HNG, and HCG and HPG in the Kyoto Encyclopedia of Genes and Genomes (KEGG) orthology (KO). Among the 328 affiliated KEGG pathways, 19 had statistically significant and different P < 0.05 in HNG and HPG (Figure 6A). Interestingly, pathways related to genetic information (basal transcription factors) and environmental information processing (calcium signaling pathway) were enriched in HPG. Pathways related to human diseases (toxoplasmosis, small-cell lung cancer, and colorectal cancer), cellular processes (p53 signaling pathway), and metabolism (carbohydrate metabolism) were depleted in HPG. And there were 23 KEGG pathways showing significant differences in HCG and HNG (Figure 6B). Pathways related to metabolism (amino acid, fatty acid, carbohydrate, and drug metabolism—cytochrome P450 and beta-lactam resistance) and human disease (bacterial invasion of epithelial cells) were enriched in HNG. However, cellular processes, signaling (other ion-coupled transporters) and other metabolism (pantothenate and CoA biosynthesis, phenylalanine, tyrosine and tryptophan biosynthesis, and lysine biosynthesis) were depleted in HNG. Seventeen KEGG pathways showed significant differences in HCG and HPG (Figure 6C). Pathways related to metabolism (lipopolysaccharide [LPS] biosynthesis proteins, beta-lactam resistance, LPS biosynthesis, fatty acid metabolism, glycosphingolipid biosynthesis–ganglio series, glycosaminoglycan degradation, metabolism of xenobiotics by cytochrome P450, N-glycan biosynthesis, glycosphingolipid biosynthesis–globo series, and other glycan degradation) and human disease (pertussis, primary immunodeficiency, bladder cancer, Chagas disease, African trypanosomiasis, and bacterial invasion of epithelial cells) were enriched in HPG, but peptidoglycan biosynthesis was found depleted in HPG. These findings show that gut microbiome affected by H. pylori infection and gastritis also causes some changes in the body's basal metabolic function, disease susceptibility, and drug metabolism. It can also be said that gut microbiome influences gastric inflammation. These results thus indicate that in children, H. pylori infection, gastritis, and altered intestinal microbiome interact with each other.

FIGURE 6

Figure 6. Predicted metagenome function based on KEGG pathway analysis. Extended error bar plots show the significantly different abundance of KEGG pathways. (A) Between HPG and HNG. (B) Between HNG and HCG. (C) Between HPG and HCG. The proportion (left side) indicates the possible abundance of microbes possessing each functional feature and the difference between proportions for each feature. Circles (right side) represent the difference between the mean proportion of bacteria (the effect size), adjacent to their respective CI (error bars). KEGG, Kyoto Encyclopedia of Genes and Genomes; HPG, Helicobacter pylori-induced gastritis group; HNG, H. pylori-negative gastritis group; HCG, healthy control group.

Discussions

Microbiome dysbiosis has been linked to gastrointestinal disease including gastritis, in which Helicobacter pylori plays an important role (He et al., 2016; Minalyan et al., 2017; Sgambato et al., 2017; Gorkiewicz and Moschen, 2018). Although there are several studies addressing bacterial biodiversity in upper GI tract, the role of H. pylori infection and gastritis in the gut bacterial community, especially in children, is unknown. A preliminary study evaluated the influence of H. pylori infection and gastritis on fecal microbiome by comparing three pediatric groups, using 16S rRNA gene sequence analysis. This study revealed (i) significant differences in beta diversity analysis in the three groups, especially in HPG, HNG, and HCG; (ii) F:B ratio dramatically decreased in both HPG and HNG, with higher abundance of Bacteroidaceae and Enterobacteriaceae and lower abundance of Lachnospiraceae, Bifidobacteriaceae, and Lactobacillaceae also found in HPG and HNG; and (iii) HPG had higher abundance of Betaproteobacteria, Lactobacillales and Streptococcus, lower abundance of Alphaproteobacteria, Megasphaera, than HNG. The results indicate that H. pylori infection and gastritis could alter gut microbiome.

Unlike adults, H. pylori-infected children were mostly asymptomatic with different microscopic gastric inflammation, and only a small proportion developed clinical manifestations of chronic infection, for example, peptic ulcer and gastric cancer (Jones et al., 2017). With declining prevalence in children, the incidence of early-onset asthma, inflammatory bowel disease (IBD), gastrointestinal and systemic infections, and Barrett's esophagus increased (Arnold et al., 2011; Cohen et al., 2012; Castano-Rodriguez et al., 2017; Minalyan et al., 2017). These were explained by the tolerogenic immune-state induced by H. pylori at an early age, which helps bacteria persist in the human host (Gorkiewicz and Moschen, 2018). Hence, H. pylori has been considered as a late-in-life human pathogen with potential early-life benefits. The decrease in eradication rate and increase in drug resistance are the main problems in children. There is no clear consensus regarding the optimal age for H. pylori eradication therapy (Gotoda et al., 2018). Moreover, the relationship between H. pylori, IBD and colon cancer is currently unclear. Investigating fecal microbiome changes induced by H. pylori infection and gastritis could be beneficial in the assessment of consequences, perpetrated by H. pylori infection in children and also in exploring new treatment strategies.

Although the exact mechanism of how gastric inflammation leads to changes in fecal microbiota are not clearly defined, there is increasing evidence that interplay between bacteria and host responses may shape commensal microbiota composition. Changes in the gastric microbiota, luminal pH, and end products of bacterial fermentation play important roles in driving the community structure of gut microbiota (Cremer et al., 2017). However, the relationship between gastritis and gut microbiome has been underreported (Chen et al., 2018; Gao et al., 2018). Juan-Juan Gao et al. analyzed fecal microbiome in patients with different H. pylori-related gastric lesions. They found alterations in dominant phyla of Bacteroidetes, Firmicutes, and Proteobacteria in groups with different H. pylori status (Gao et al., 2018). These had never been observed in related studies in children. The results of the current study first showed that different floras in HNG and HCG before treatment were impacted by simple gastritis. Our data suggested that the abundance of Bacteroidaceae, Enterobacteriaceae, Porphyromonadaceae, Fusobacteriaceae, Bacteroides, and Megasphaera increased in the HNG. Interestingly, most of the significant taxa belonged to Gram-negative bacteria producing LPS. The LPS from intestinal microbiome induces a chronic subclinical inflammatory process (Saad et al., 2016). These results together indicate that variation in fecal microbiome could be an additional risk factor promoting gastrointestinal inflammation in children.

H. pylori infection is the main cause of gastritis and has developed mechanisms to coexist in the harsh gastric microenvironment, where it induces mucosal inflammation, immune activation, hypergastrinemia, and variable effects on gastric acid production. On the basis of our findings, we concluded that HPG had a higher abundance of Lactobacillales and Streptococcus. In our study, the abundance of Lactobacillaceae and Lactobacillus all decreased in HPG and HNG, but in HPG, there was higher abundance of Lactobacillales. Lactobacillales belong to Bacilli class and Firmicutes phylum and have six families. Lactobacillaceae and Lactobacillus did not increase or decrease when HPG and HNG were compared. However, Streptococcus genus, which belongs to the Streptococcaceae family, increased significantly in HPG. Hence, we correlated the rich abundance of Lactobacillales with higher abundance of Streptococcus genus. Streptococcus belongs to commensals like oral microbiome (Nasidze et al., 2009) and healthy esophageal core microbiome (Hunt and Yaghoobi, 2017; Nardone et al., 2017). Khosravi et al. reported that Streptococcus mitis induced the conversion of H. pylori to coccoid cells in coculture studies and inhibited its growth (Khosravi et al., 2014a). Furthermore, a study found that (insulin–gastrin) INS-GAS mice coinfected with H. pylori and Streptococcus salivarius developed more severe gastric inflammation than did H. pylori only at 5 months post-infection (Rizzato et al., 2019). Streptococcus has also been associated with peptic ulcer (Khosravi et al., 2014b) and gastric carcinogenesis (Coker et al., 2018). Hence, Streptococcus genus exists in normal gastrointestinal tract and interacts with gastric diseases. Our study also concluded that a lower abundance of Megasphaera had been found in HPG, compared with HNG. Megasphaera, a genus of Firmicutes bacteria within the class Negativicutes, has been found in the stomach of cattle and sheep and in human fetuses. A type of Megasphaera species, named Megasphaera elsdenii, inhabits the human intestine and has probiotic potential (Kwon et al., 2018). Owing to technological limitations, the real bacterial response in humans still needs to be confirmed in further studies.

In conclusion, fecal microbiome was affected by H. pylori in patients with gastritis. However, comparisons of compositions of gut microbiome in HPG and HCG also confirmed the above alteration in fecal microbiome in gastritis and H. pylori infection. At the same time, it also shows that most changes in intestinal flora are caused by gastric infection. However, factors caused by H. pylori infection can also cause alterations in the quantum of some special bacteria. Streptococcus and Megasphaera were found in abundance in HPG and HNG. This is consistent with symptoms of indigestion observed in patients with H. pylori-induced gastritis and common gastritis (Correa Silva et al., 2016; Jones et al., 2017).

With respect to the altered fecal microbiome composition in gastritis, the F:B ratio dramatically decreased in HPG and HNG. The reduced ratio of F:B in H. pylori-positive subjects before treatment has also been found in another study (Osaki et al., 2018). It is well-known that the ratio of F:B is related to obesity, body mass index (BMI), metabolic syndrome, elderly people, and the eradication of H. pylori infection (Azuma et al., 2002; Claesson et al., 2011; Takeoka et al., 2016). The current study did not measure the BMI of all individuals; further research is needed to verify the interaction between the ratio of F:B and H. pylori infection. Higher abundance of Enterobacteriaceae and Bacteroides was also found in groups. There are many kinds of pathogenic bacteria in Enterobacteriaceae, like Escherichia, Salmonella, and Shigella. Enterotoxigenic Escherichia coli (ETEC) can produce enterotoxin. It is known that ETEC increases the release of diamine oxidase (DAO) and D-lactate in the plasma, which can lead to damage of the intestinal epithelial cell membrane (Liu et al., 2017). The up-regulation of pro-inflammatory cytokines and down-regulation of anti-inflammatory cytokines (Xun et al., 2015) may be a way to influence gastritis. Bacteroides fragilis, which accounts for only 0.5% of the human colonic microbiome, is the most commonly isolated anaerobic pathogen. In addition, a number of Bacteroides spp. have high resistance to antibiotics (Mazmanian et al., 2005; Wexler, 2007). Several studies have reported an increase or decrease in Bacteroidales in mucosal samples of IBD subjects compared with controls (Zitomersky et al., 2013), which indicates that Bacteroidales are connected with IBD. Abundance of two taxa (Enterobacteriaceae and Bacteroides) is connected with intestinal inflammation and IBD.

Generally, two genera of Lactobacillus and Bifidobacterium are considered as probiotics, which are important to human health (Wang Y. et al., 2018). This study revealed that the two genera significantly decreased in the gut microbiome of children in HPG and HNG. They can change the PH of the intestinal environment to inhibit the growth of pathogenic bacteria and stimulate an immune response (Zhu et al., 2018). Some studies also concluded that Lactobacillus spp. in the gastric microbiome also has an inhibitory effect against H. pylori (Zaman et al., 2014; Salas-Jara et al., 2016). In another study, children with H. pylori infection had a decreased relative abundance of Bifidobacterium, which significantly increased after the children ingested probiotics-containing yogurt (Yang and Sheu, 2012). Higher abundance of Lactobacillus and Bifidobacterium in healthy children could protect them from gastrointestinal inflammation. But some other studies also have opposite results from Lactobacillus. A recent study on Lactobacillus and H. pylori coisolates from humans did not reveal any significant influence of lactobacilli on H. pylori strains (Skoog et al., 2011). Iino et al. also found that H. pylori infection initially influenced the composition ratio of each Lactobacillus species in the gut microbiota before atrophic gastritis progression and suggested a higher abundance of Lactobacillus in H. pylori-infected subjects with severe atrophic gastritis (Iino et al., 2018). A German study also reported that H. pylori led to an increased growth of lactobacilli in fecal microbiome (Buhling et al., 2001). These results were considered to take into account long-term acid suppression induced by H. pylori infection and PPI therapy following atrophic gastritis (Takashima et al., 2001; Weck et al., 2009; Jackson et al., 2016). This suggests that lactic acid-producing bacteria may also enhance gastric inflammatory reactions caused by H. pylori. There is still controversy in the species and dosage of Lactobacillus as probiotic with H. pylori infection (Schulz et al., 2015; Iino et al., 2018). Lower abundance of two genera in the gut microbiome of children in HPG may promote the production of inflammatory factors, leading to gastritis. However, before the results of our study are used for the treatment of H. pylori-induced gastritis with Lactobacillus and Bifidobacterium, the two bacterial species need to be confirmed in future studies.

To compare the detailed altered KEGG pathway, significant differences in colorectal cancer occurrence between the two groups have been associated with specific changes in gut microbiome composition. A metagenome-wide association study (MGWAS) was performed, and it was found that certain Bacteroides spp. (e.g., Bacteroides dorei, Bacteroides vulgatus, and Bacteroides massilensis) and E. coli were associated with systemic inflammation and tumor staging (Feng et al., 2015). Since the last two decades, several studies investigated the potential association of H. pylori infection with colorectal neoplasia (Breuer-Katschinski et al., 1999; Mizuno et al., 2005; Inoue et al., 2011; Papastergiou et al., 2016). However, direct activation of colorectal carcinogenesis by the bacterium remains controversial (Papastergiou et al., 2016). Our data suggest that higher abundance of Bacteroidaceae and Enterobacteriaceae was also found in the HNG and HPG, and the KEGG pathway of colorectal cancer increased in HNG, similar to another study (Chen et al., 2018), whereas most studies have reported that colorectal cancer pathways were predicted to be higher in the H. pylori-positive group (Kountouras et al., 2018; Kumar et al., 2018). It is necessary to confirm the true relationship of H. pylori, gastritis, and colorectal cancer by further research on gut microbiome alteration.

Our study showed significant increase of activity in metabolic pathways of children with HPG and HNG. This included fatty acid metabolism and beta-lactam resistance to drug due to cytochrome P450. H. pylori depends on unsaturated fatty acid (UFA) biosynthesis for maintaining its membrane structure and function (Bi et al., 2016). The level of microbial UFA is significantly elevated in the blood of patients with H. pylori infection-induced peptic ulceration (Ktsoyan et al., 2010). These results suggest that H. pylori infection is related to higher lipid metabolism. The functional analysis of microbiome revealed that lipid metabolism pathway increased in the group with gastritis, indicating that gut microbiome has similar effects as H. pylori-induced gastritis. H. pylori eradication is affected by antibiotic resistance and genotypes (Chunlertlith et al., 2017). Increased antibiotic resistance, such as beta-lactam and cytochrome P450 CYP2C19 gene expression that could encode a protein degrading PPI decreases the eradication rate of H. pylori (Boyanova et al., 2016). Results showed that beta-lactam resistance and cytochrome P450 pathways increased in children of both HPG and HNG, which is important information for developing alternative or improved treatment strategies. Thus, the body status of the glucose and lipid metabolism, beta-lactam resistance, metabolism of xenobiotics by cytochrome P450 and drugs by cytochrome P450 may be connected to gastritis. Treatment effectiveness of H. pylori-induced gastritis in children can be increased by altering fecal microbiome, especially the eradication rate of H. pylori.

Widespread use of antibiotics in children for H. pylori gastritis decreases efficacy of H. pylori eradication therapy and increases prevalence of antibiotic-resistant strains. This study reports the difference in fecal microbiome observed in infection caused by H. pylori and gastritis. Streptococcus and Megasphaera were found in gut microbiome in HPG and HNG. The altered categories within the KEGG pathway suggest that these different bacteria may play a role in the drug resistance of H. pylori infection or the relationship with colon cancer and IBD. These results suggest that gastritis itself can cause changes in composition of fecal microbiome, which may be exacerbated by H. pylori infection. These changes in gut microbiome may be related to drug resistance and the development of chronic gastrointestinal diseases, affecting the treatment of H. pylori infection and gastritis. Lactobacillus and Bifidobacterium can be used as probiotics to treat gastritis patients. This indeed suggests the close interaction of H. pylori infection, gastritis, and gut microbioma. Hence, the decision to investigate and treat the infection should be assessed by a clear benefit for the individual child. Reasonable and effective treatment should be selected for children to avoid repeated antibiotic use for intestinal flora. The use of probiotics is expected to be used to treat children with mild illness or to alleviate symptoms. But the efficacy, species, and dosage of probiotics, however, need to be further studied.

In conclusion, this study first demonstrated the structural, compositional, and functional dysbiosis of fecal microbiome in gastritis caused by H. pylori. It indicated that the current treatments combined with strategies that modulate the gut microbiome could improve the clinical outcome of H. pylori-induced gastritis. The findings may pave the way for initiating larger-cohort clinical validations and developing guidance for therapeutic strategies with probiotics. However, the study also has some shortcomings; for example, the technology is accurate for only a few species, and the corresponding specimen of gastric mucosa and blood samples of individuals were not collected to compare with the same fecal specimen. In addition, the number of involved children was less. In future, a larger study is required, and detailed clinical data need to be collected to confirm these results.

Data Availability Statement

All sequencing data associated with this study were uploaded to the NCBI SRA database (accession number: PRJNA544571). The webpage of the SRA database is https://www.ncbi.nlm.nih.gov/sra.

Ethics Statement

The studies involving human participants were reviewed and approved by Medical Ethics Committee of Qilu Children's Hospital of Shandong University. Written informed consent to participate in this study was provided by the participants' legal guardian/next of kin.

Author Contributions

LZ and ZG designed the study. LY, JZ, CZ, and JY performed the measurements and data analysis. JX, XW, YL, HL, and YW obtained the samples and clinical details. LY and JZ wrote the manuscript. All authors have read and critically revised the manuscript.

Conflict of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

We thank all the participants of this study, which was supported by the Shandong Provincial Key Research and Development Program under contract no. 2018CXGC1219 (to ZG), the Shandong Provincial Key Research and Development Program under Contract No. 2017G006039 (to YW), and the Weihai Technique Extension Project under Contract No. 2016GNS023, the National Natural Science Foundation of China under Contract No. 31471202 and the Shandong Provincial Key Research and Development Program under Contract No. 2016YYSP009 (to LZ). LZ was also supported by the Taishan Scholars Program of Shandong Province. We were also grateful to Jianfeng Wang and Bin Chen (Beijing Nebula Medical Laboratory Co., Ltd.) for assistance with data analysis and revising manuscripts.

References

Alarcon, T., Llorca, L., and Perez-Perez, G. (2017). Impact of the microbiota and gastric disease development by Helicobacter pylori. Curr. Top. Microbiol. Immunol. 400, 253–275. doi: 10.1007/978-3-319-50520-6_11

PubMed Abstract | CrossRef Full Text | Google Scholar

Arnold, I. C., Dehzad, N., Reuter, S., Martin, H., Becher, B., Taube, C., et al. (2011). Helicobacter pylori infection prevents allergic asthma in mouse models through the induction of regulatory T cells. J. Clin. Invest. 121, 3088–3093. doi: 10.1172/JCI45041

PubMed Abstract | CrossRef Full Text | Google Scholar

Aviles-Jimenez, F., Vazquez-Jimenez, F., Medrano-Guzman, R., Mantilla, A., and Torres, J. (2014). Stomach microbiota composition varies between patients with non-atrophic gastritis and patients with intestinal type of gastric cancer. Sci. Rep. 4:4202. doi: 10.1038/srep04202

PubMed Abstract | CrossRef Full Text | Google Scholar

Azuma, T., Suto, H., Ito, Y., Muramatsu, A., Ohtani, M., Dojo, M., et al. (2002). Eradication of Helicobacter pylori infection induces an increase in body mass index. Aliment. Pharmacol. Ther. 16, 240–244. doi: 10.1046/j.1365-2036.16.s2.31.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Baatar, D., Patel, K., and Taub, D. D. (2011). The effects of ghrelin on inflammation and the immune system. Mol. Cell. Endocrinol. 340, 44–58. doi: 10.1016/j.mce.2011.04.019

PubMed Abstract | CrossRef Full Text | Google Scholar

Beasley, D. E., Koltz, A. M., Lambert, J. E., Fierer, N., and Dunn, R. R. (2015). The evolution of stomach acidity and its relevance to the human microbiome. PLoS ONE 10:e0134116. doi: 10.1371/journal.pone.0134116

PubMed Abstract | CrossRef Full Text | Google Scholar

Bi, H., Zhu, L., Jia, J., Zeng, L., and Cronan, J. E. (2016). Unsaturated fatty acid synthesis in the gastric pathogen helicobacter pylori proceeds via a backtracking mechanism. Cell Chem. Biol. 23, 1480–1489. doi: 10.1016/j.chembiol.2016.10.007

PubMed Abstract | CrossRef Full Text | Google Scholar

Bik, E. M., Eckburg, P. B., Gill, S. R., Nelson, K. E., Purdom, E. A., Francois, F., et al. (2006). Molecular analysis of the bacterial microbiota in the human stomach. Proc. Natl. Acad. Sci. U.S.A. 103, 732–737. doi: 10.1073/pnas.0506655103

PubMed Abstract | CrossRef Full Text | Google Scholar

Boyanova, L., Gergova, G., Evstatiev, I., Spassova, Z., Kandilarov, N., Yaneva, P., et al. (2016). Helicobacter pylori resistance to six antibiotics by two breakpoint systems and resistance evolution in Bulgaria. Infect. Dis. 48, 56–62. doi: 10.3109/23744235.2015.1082035

PubMed Abstract | CrossRef Full Text | Google Scholar

Brawner, K. M., Kumar, R., Serrano, C. A., Ptacek, T., Lefkowitz, E., Morrow, C. D., et al. (2017). Helicobacter pylori infection is associated with an altered gastric microbiota in children. Mucosal Immunol. 10, 1169–1177. doi: 10.1038/mi.2016.131

PubMed Abstract | CrossRef Full Text | Google Scholar

Breuer-Katschinski, B., Nemes, K., Marr, A., Rump, B., Leiendecker, B., Breuer, N., et al. (1999). Helicobacter pylori and the risk of colonic adenomas. Colorect. Adenoma Study Group Digest. 60, 210–215. doi: 10.1159/000007661

PubMed Abstract | CrossRef Full Text | Google Scholar

Buhling, A., Radun, D., Muller, W. A., and Malfertheiner, P. (2001). Influence of anti-Helicobacter triple-therapy with metronidazole, omeprazole and clarithromycin on intestinal microflora. Aliment. Pharmacol. Ther. 15, 1445–1452. doi: 10.1046/j.1365-2036.2001.01033.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Caporaso, J. G., Kuczynski, J., Stombaugh, J., Bittinger, K., Bushman, F. D., Costello, E. K., et al. (2010). QIIME allows analysis of high-throughput community sequencing data. Nat. Methods 7, 335–336. doi: 10.1038/nmeth.f.303

PubMed Abstract | CrossRef Full Text | Google Scholar

Castano-Rodriguez, N., Kaakoush, N. O., Lee, W. S., and Mitchell, H. M. (2017). Dual role of Helicobacter and Campylobacter species in IBD: a systematic review and meta-analysis. Gut 66, 235–249. doi: 10.1136/gutjnl-2015-310545

PubMed Abstract | CrossRef Full Text | Google Scholar

Chen, L., Xu, W., Lee, A., He, J., Huang, B., Zheng, W., et al. (2018). The impact of Helicobacter pylori infection, eradication therapy and probiotic supplementation on gut microenvironment homeostasis: an open-label, randomized clinical trial. EBioMedicine 35, 87–96. doi: 10.1016/j.ebiom.2018.08.028

PubMed Abstract | CrossRef Full Text | Google Scholar

Chunlertlith, K., Limpapanasit, U., Mairiang, P., Vannaprasaht, S., Tassaneeyakul, W., Sangchan, A., et al. (2017). Outcomes of a randomized controlled trial comparing modified high dose omeprazole and amoxicillin triple therapy with standard triple therapy for Helicobacter pylori eradication. Asian Pac. J. Cancer Prev. 18, 927–932. doi: 10.22034/APJCP.2017.18.4.927

PubMed Abstract | CrossRef Full Text | Google Scholar

Claesson, M. J., Cusack, S., O'Sullivan, O., Greene-Diniz, R., de Weerd, H., Flannery, E., et al. (2011). Composition, variability, and temporal stability of the intestinal microbiota of the elderly. Proc. Natl. Acad. Sci. U.S.A. 108, 4586–4591. doi: 10.1073/pnas.1000097107

PubMed Abstract | CrossRef Full Text | Google Scholar

Cohen, D., Shoham, O., Orr, N., and Muhsen, K. (2012). An inverse and independent association between Helicobacter pylori infection and the incidence of shigellosis and other diarrheal diseases. Clin. Infect. Dis. 54, e35–e42. doi: 10.1093/cid/cir916

PubMed Abstract | CrossRef Full Text | Google Scholar

Coker, O. O., Dai, Z., Nie, Y., Zhao, G., Cao, L., Nakatsu, G., et al. (2018). Mucosal microbiome dysbiosis in gastric carcinogenesis. Gut 67, 1024–1032. doi: 10.1136/gutjnl-2017-314281

PubMed Abstract | CrossRef Full Text | Google Scholar

Cole, J. R., Wang, Q., Cardenas, E., Fish, J., Chai, B., Farris, R. J., et al. (2009). The ribosomal database project: improved alignments and new tools for rRNA analysis. Nucleic Acids Res. 37, D141–D145. doi: 10.1093/nar/gkn879

PubMed Abstract | CrossRef Full Text | Google Scholar

Correa Silva, R. G., Machado, N. C., Carvalho, M. A., and Rodrigues, M. A. (2016). Helicobacter pylori infection is high in paediatric nonulcer dyspepsia but not associated with specific gastrointestinal symptoms. Acta Paediatr. 105, e228–e231. doi: 10.1111/apa.13347

CrossRef Full Text | Google Scholar

Cremer, J., Arnoldini, M., and Hwa, T. (2017). Effect of water flow and chemical environment on microbiota growth and composition in the human colon. Proc. Natl. Acad. Sci. U.S.A. 114, 6438–6443. doi: 10.1073/pnas.1619598114

PubMed Abstract | CrossRef Full Text | Google Scholar

Feng, Q., Liang, S., Jia, H., Stadlmayr, A., Tang, L., Lan, Z., et al. (2015). Gut microbiome development along the colorectal adenoma-carcinoma sequence. Nat. Commun. 6:6528. doi: 10.1038/ncomms7528

PubMed Abstract | CrossRef Full Text | Google Scholar

Ferreira, R. M., Pereira-Marques, J., Pinto-Ribeiro, I., Costa, J. L., Carneiro, F., Machado, J. C., et al. (2018). Gastric microbial community profiling reveals a dysbiotic cancer-associated microbiota. Gut 67, 226–236. doi: 10.1136/gutjnl-2017-314205

PubMed Abstract | CrossRef Full Text | Google Scholar

Francois, F., Roper, J., Joseph, N., Pei, Z., Chhada, A., Shak, J. R., et al. (2011). The effect of H. pylori eradication on meal-associated changes in plasma ghrelin and leptin. BMC Gastroenterol. 11:37. doi: 10.1186/1471-230X-11-37

PubMed Abstract | CrossRef Full Text | Google Scholar

Gao, J. J., Zhang, Y., Gerhard, M., Mejias-Luque, R., Zhang, L., Vieth, M., et al. (2018). Association between gut microbiota and Helicobacter pylori-related gastric lesions in a high-risk population of gastric cancer. Front. Cell. Infect. Microbiol. 8:202. doi: 10.3389/fcimb.2018.00202

PubMed Abstract | CrossRef Full Text | Google Scholar

Gorkiewicz, G., and Moschen, A. (2018). Gut microbiome: a new player in gastrointestinal disease. Virchows Arch. 472, 159–172. doi: 10.1007/s00428-017-2277-x

PubMed Abstract | CrossRef Full Text | Google Scholar

Gotoda, T., Takano, C., Kusano, C., Suzuki, S., Ikehara, H., Hayakawa, S., et al. (2018). Gut microbiome can be restored without adverse events after Helicobacter pylori eradication therapy in teenagers. Helicobacter 23:e12541. doi: 10.1111/hel.12541

PubMed Abstract | CrossRef Full Text | Google Scholar

He, C., Yang, Z., and Lu, N. (2016). Imbalance of gastrointestinal microbiota in the pathogenesis of Helicobacter pylori-associated diseases. Helicobacter 21, 337–348. doi: 10.1111/hel.12297

PubMed Abstract | CrossRef Full Text | Google Scholar

Heimesaat, M. M., Fischer, A., Plickert, R., Wiedemann, T., Loddenkemper, C., Gobel, U. B., et al. (2014). Helicobacter pylori induced gastric immunopathology is associated with distinct microbiota changes in the large intestines of long-term infected Mongolian gerbils. PLoS ONE 9:e100362. doi: 10.1371/journal.pone.0100362

PubMed Abstract | CrossRef Full Text | Google Scholar

Hunt, R. H., and Yaghoobi, M. (2017). The esophageal and gastric microbiome in health and disease. Gastroenterol. Clin. North Am. 46, 121–141. doi: 10.1016/j.gtc.2016.09.009

PubMed Abstract | CrossRef Full Text | Google Scholar

Iino, C., Shimoyama, T., Chinda, D., Arai, T., Chiba, D., Nakaji, S., et al. (2018). Infection of Helicobacter pylori and atrophic gastritis influence lactobacillus in gut microbiota in a Japanese population. Front. Immunol. 9:712. doi: 10.3389/fimmu.2018.00712

PubMed Abstract | CrossRef Full Text | Google Scholar

Inoue, I., Mukoubayashi, C., Yoshimura, N., Niwa, T., Deguchi, H., Watanabe, M., et al. (2011). Elevated risk of colorectal adenoma with Helicobacter pylori-related chronic gastritis: a population-based case-control study. Int. J. Cancer 129, 2704–2711. doi: 10.1002/ijc.25931

PubMed Abstract | CrossRef Full Text | Google Scholar

Jackson, M. A., Goodrich, J. K., Maxan, M. E., Freedberg, D. E., Abrams, J. A., Poole, A. C., et al. (2016). Proton pump inhibitors alter the composition of the gut microbiota. Gut 65, 749–756. doi: 10.1136/gutjnl-2015-310861

PubMed Abstract | CrossRef Full Text | Google Scholar

Jones, N. L., Koletzko, S., Goodman, K., Bontems, P., Cadranel, S., Casswall, T., et al. (2017). Joint ESPGHAN/NASPGHAN guidelines for the management of Helicobacter pylori in children and adolescents (update 2016). J. Pediatr. Gastroenterol. Nutr. 64, 991–1003. doi: 10.1097/MPG.0000000000001594

PubMed Abstract | CrossRef Full Text | Google Scholar

Khosravi, Y., Dieye, Y., Loke, M. F., Goh, K. L., and Vadivelu, J. (2014a). Streptococcus mitis induces conversion of Helicobacter pylori to coccoid cells during co-culture in vitro. PLoS ONE 9:e112214. doi: 10.1371/journal.pone.0112214

PubMed Abstract | CrossRef Full Text | Google Scholar

Khosravi, Y., Dieye, Y., Poh, B. H., Ng, C. G., Loke, M. F., Goh, K. L., et al. (2014b). Culturable bacterial microbiota of the stomach of Helicobacter pylori positive and negative gastric disease patients. ScientificWorldJournal 2014:610421. doi: 10.1155/2014/610421

PubMed Abstract | CrossRef Full Text | Google Scholar

Kienesberger, S., Cox, L. M., Livanos, A., Zhang, X. S., Chung, J., Perez-Perez, G. I., et al. (2016). Gastric Helicobacter pylori infection affects local and distant microbial populations and host responses. Cell Rep. 14, 1395–1407. doi: 10.1016/j.celrep.2016.01.017

PubMed Abstract | CrossRef Full Text | Google Scholar

Koletzko, S., Jones, N. L., Goodman, K. J., Gold, B., Rowland, M., Cadranel, S., et al. (2011). Evidence-based guidelines from ESPGHAN and NASPGHAN for Helicobacter pylori infection in children. J. Pediatr. Gastroenterol. Nutr. 53, 230–243. doi: 10.1097/MPG.0b013e3182227e90

PubMed Abstract | CrossRef Full Text | Google Scholar

Kountouras, J., Polyzos, S. A., Doulberis, M., Zeglinas, C., Artemaki, F., Vardaka, E., et al. (2018). Potential impact of Helicobacter pylori-related metabolic syndrome on upper and lower gastrointestinal tract oncogenesis. Metabolism 87, 18–24. doi: 10.1016/j.metabol.2018.06.008

PubMed Abstract | CrossRef Full Text | Google Scholar

Ktsoyan, Z. A., Beloborodova, N. V., Sedrakyan, A. M., Osipov, G. A., Khachatryan, Z. A., Kelly, D., et al. (2010). Profiles of microbial fatty acids in the human metabolome are disease-specific. Front. Microbiol. 1:148. doi: 10.3389/fmicb.2010.00148

PubMed Abstract | CrossRef Full Text | Google Scholar

Kumar, A., Kim, M., and Lukin, D. J. (2018). Helicobacter pylori is associated with increased risk of serrated colonic polyps: analysis of serrated polyp risk factors. Indian J. Gastroenterol. 37, 235–242. doi: 10.1007/s12664-018-0855-8

PubMed Abstract | CrossRef Full Text | Google Scholar

Kwon, G., Lee, J., Koh, J. H., and Lim, Y. H. (2018). Lifespan extension of Caenorhabditis elegans by Butyricicoccus pullicaecorum and Megasphaera elsdenii with probiotic potential. Curr. Microbiol. 75, 557–564. doi: 10.1007/s00284-017-1416-6

PubMed Abstract | CrossRef Full Text | Google Scholar

La Cava, A., and Matarese, G. (2004). The weight of leptin in immunity. Nat. Rev. Immunol. 4, 371–379. doi: 10.1038/nri1350

PubMed Abstract | CrossRef Full Text | Google Scholar

Langille, M. G., Zaneveld, J., Caporaso, J. G., McDonald, D., Knights, D., Reyes, J. A., et al. (2013). Predictive functional profiling of microbial communities using 16S rRNA marker gene sequences. Nat. Biotechnol. 31, 814–821. doi: 10.1038/nbt.2676

PubMed Abstract | CrossRef Full Text | Google Scholar

Li, S., Huang, X. L., Sui, J. Z., Chen, S. Y., Xie, Y. T., Deng, Y., et al. (2014). Meta-analysis of randomized controlled trials on the efficacy of probiotics in Helicobacter pylori eradication therapy in children. Eur. J. Pediatr. 173, 153–161. doi: 10.1007/s00431-013-2220-3

PubMed Abstract | CrossRef Full Text | Google Scholar

Liu, Q., Ni, X., Wang, Q., Peng, Z., Niu, L., Wang, H., et al. (2017). Lactobacillus plantarum BSGP201683 isolated from Giant Panda Feces attenuated inflammation and improved gut microflora in mice challenged with enterotoxigenic Escherichia coli. Front. Microbiol. 8:1885. doi: 10.3389/fmicb.2017.01885

PubMed Abstract | CrossRef Full Text | Google Scholar

Llorca, L., Perez-Perez, G., Urruzuno, P., Martinez, M. J., Iizumi, T., Gao, Z., et al. (2017). Characterization of the gastric microbiota in a pediatric population according to Helicobacter pylori status. Pediatr. Infect. Dis. J. 36, 173–178. doi: 10.1097/INF.0000000000001383

PubMed Abstract | CrossRef Full Text | Google Scholar

Maldonado-Contreras, A., Goldfarb, K. C., Godoy-Vitorino, F., Karaoz, U., Contreras, M., Blaser, M. J., et al. (2011). Structure of the human gastric bacterial community in relation to Helicobacter pylori status. ISME J. 5, 574–579. doi: 10.1038/ismej.2010.149

PubMed Abstract | CrossRef Full Text | Google Scholar

Malfertheiner, P., Megraud, F., O'Morain, C. A., Gisbert, J. P., Kuipers, E. J., Axon, A. T., et al. (2017). Management of Helicobacter pylori infection-the Maastricht V/Florence consensus report. Gut 66, 6–30. doi: 10.1136/gutjnl-2016-312288

PubMed Abstract | CrossRef Full Text | Google Scholar

Marshall, B. J., and Warren, J. R. (1984). Unidentified curved bacilli in the stomach of patients with gastritis and peptic ulceration. Lancet 1, 1311–1315. doi: 10.1016/s0140-6736(84)91816-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Mazmanian, S. K., Liu, C. H., Tzianabos, A. O., and Kasper, D. L. (2005). An immunomodulatory molecule of symbiotic bacteria directs maturation of the host immune system. Cell 122, 107–118. doi: 10.1016/j.cell.2005.05.007

PubMed Abstract | CrossRef Full Text | Google Scholar

McMurdie, P. J., and Holmes, S. (2013). phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLoS ONE 8:e61217. doi: 10.1371/journal.pone.0061217

PubMed Abstract | CrossRef Full Text | Google Scholar

Minalyan, A., Gabrielyan, L., Scott, D., Jacobs, J., and Pisegna, J. R. (2017). The gastric and intestinal microbiome: role of proton pump inhibitors. Curr. Gastroenterol. Rep. 19:42. doi: 10.1007/s11894-017-0577-6

PubMed Abstract | CrossRef Full Text | Google Scholar

Mizuno, S., Morita, Y., Inui, T., Asakawa, A., Ueno, N., Ando, T., et al. (2005). Helicobacter pylori infection is associated with colon adenomatous polyps detected by high-resolution colonoscopy. Int. J. Cancer 117, 1058–1059. doi: 10.1002/ijc.21280

PubMed Abstract | CrossRef Full Text | Google Scholar

Muhsen, K., Goren, S., and Cohen, D. (2015). Helicobacter pylori infection in early childhood and growth at school age. Helicobacter 20, 410–417. doi: 10.1111/hel.12227

PubMed Abstract | CrossRef Full Text | Google Scholar

Myllyluoma, E., Ahlroos, T., Veijola, L., Rautelin, H., Tynkkynen, S., and Korpela, R. (2007). Effects of anti-Helicobacter pylori treatment and probiotic supplementation on intestinal microbiota. Int. J. Antimicrob. Agents 29, 66–72. doi: 10.1016/j.ijantimicag.2006.08.034

PubMed Abstract | CrossRef Full Text | Google Scholar

Nardone, G., Compare, D., and Rocco, A. (2017). A microbiota-centric view of diseases of the upper gastrointestinal tract. Lancet Gastroenterol. Hepatol. 2, 298–312. doi: 10.1016/S2468-1253(16)30108-X

PubMed Abstract | CrossRef Full Text | Google Scholar

Nasidze, I., Li, J., Quinque, D., Tang, K., and Stoneking, M. (2009). Global diversity in the human salivary microbiome. Genome Res. 19, 636–643. doi: 10.1101/gr.084616.108

PubMed Abstract | CrossRef Full Text | Google Scholar

Oderda, G., Shcherbakov, P., Bontems, P., Urruzuno, P., Romano, C., Gottrand, F., et al. (2007). Results from the pediatric European register for treatment of Helicobacter pylori (PERTH). Helicobacter 12, 150–156. doi: 10.1111/j.1523-5378.2007.00485.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Okuda, M., Kikuchi, S., Mabe, K., Osaki, T., Kamiya, S., Fukuda, Y., et al. (2017). Nationwide survey of Helicobacter pylori treatment for children and adolescents in Japan. Pediatr. Int. 59, 57–61. doi: 10.1111/ped.13038

PubMed Abstract | CrossRef Full Text | Google Scholar

O'Ryan, M. L., Lucero, Y., Rabello, M., Mamani, N., Salinas, A. M., Pena, A., et al. (2015). Persistent and transient Helicobacter pylori infections in early childhood. Clin. Infect. Dis. 61, 211–218. doi: 10.1093/cid/civ256

PubMed Abstract | CrossRef Full Text | Google Scholar

Osaki, T., Zaman, C., Yonezawa, H., Lin, Y., Okuda, M., Nozaki, E., et al. (2018). Influence of intestinal indigenous microbiota on intrafamilial infection by Helicobacter pylori in Japan. Front. Immunol. 9:287. doi: 10.3389/fimmu.2018.00287

PubMed Abstract | CrossRef Full Text | Google Scholar

Papastergiou, V., Karatapanis, S., and Georgopoulos, S. D. (2016). Helicobacter pylori and colorectal neoplasia: is there a causal link? World J. Gastroenterol. 22, 649–658. doi: 10.3748/wjg.v22.i2.649

PubMed Abstract | CrossRef Full Text | Google Scholar

Rizzato, C., Torres, J., Kasamatsu, E., Camorlinga-Ponce, M., Bravo, M. M., Canzian, F., et al. (2019). Potential role of biofilm formation in the development of digestive tract cancer with special reference to Helicobacter pylori infection. Front. Microbiol. 10:846. doi: 10.3389/fmicb.2019.00846

PubMed Abstract | CrossRef Full Text | Google Scholar

Saad, M. J., Santos, A., and Prada, P. O. (2016). Linking gut microbiota and inflammation to obesity and insulin resistance. Physiology 31, 283–293. doi: 10.1152/physiol.00041.2015

PubMed Abstract | CrossRef Full Text | Google Scholar

Salas-Jara, M. J., Sanhueza, E. A., Retamal-Diaz, A., Gonzalez, C., Urrutia, H., and Garcia, A. (2016). Probiotic Lactobacillus fermentum UCO-979C biofilm formation on AGS and Caco-2 cells and Helicobacter pylori inhibition. Biofouling 32, 1245–1257. doi: 10.1080/08927014.2016.1249367

PubMed Abstract | CrossRef Full Text | Google Scholar

Schulz, C., Koch, N., Schutte, K., Pieper, D. H., and Malfertheiner, P. H. (2015). Pylori and its modulation of gastrointestinal microbiota. J. Dig. Dis. 16, 109–117. doi: 10.1111/1751-2980.12233

PubMed Abstract | CrossRef Full Text | Google Scholar

Sgambato, D., Miranda, A., Romano, L., and Romano, M. (2017). Gut microbiota and gastric disease. Minerva Gastroenterol. Dietol. 63, 345–354. doi: 10.23736/S1121-421X.17.02380-7

PubMed Abstract | CrossRef Full Text | Google Scholar

Skoog, E. C., Lindberg, M., and Linden, S. K. (2011). Strain-dependent proliferation in response to human gastric mucin and adhesion properties of Helicobacter pylori are not affected by co-isolated Lactobacillus sp. Helicobacter 16, 9–19. doi: 10.1111/j.1523-5378.2010.00810.x

CrossRef Full Text | Google Scholar

Sugano, K., Tack, J., Kuipers, E. J., Graham, D. Y., El-Omar, E. M., Miura, S., et al. (2015). Kyoto global consensus report on Helicobacter pylori gastritis. Gut 64, 1353–1367. doi: 10.1136/gutjnl-2015-309252

PubMed Abstract | CrossRef Full Text | Google Scholar

Szajewska, H., Horvath, A., and Piwowarczyk, A. (2010). Meta-analysis: the effects of Saccharomyces boulardii supplementation on Helicobacter pylori eradication rates and side effects during treatment. Aliment. Pharmacol. Ther. 32, 1069–1079. doi: 10.1111/j.1365-2036.2010.04457.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Takashima, M., Furuta, T., Hanai, H., Sugimura, H., and Kaneko, E. (2001). Effects of Helicobacter pylori infection on gastric acid secretion and serum gastrin levels in Mongolian gerbils. Gut 48, 765–773. doi: 10.1136/gut.48.6.765

PubMed Abstract | CrossRef Full Text | Google Scholar

Takeoka, A., Tayama, J., Yamasaki, H., Kobayashi, M., Ogawa, S., Saigo, T., et al. (2016). Impact of Helicobacter pylori immunoglobulin G levels and atrophic gastritis status on risk of metabolic syndrome. PLoS ONE 11:e0166588. doi: 10.1371/journal.pone.0166588

PubMed Abstract | CrossRef Full Text | Google Scholar

Wang, G., Romero-Gallo, J., Benoit, S. L., Piazuelo, M. B., Dominguez, R. L., Morgan, D. R., et al. (2016). Hydrogen metabolism in Helicobacter pylori plays a role in gastric carcinogenesis through facilitating CagA translocation. mBio 7:e1022-16. doi: 10.1128/mBio.01022-16

PubMed Abstract | CrossRef Full Text | Google Scholar

Wang, X., Zhang, L., Wang, Y., Liu, X., Zhang, H., Liu, Y., et al. (2018). Gut microbiota dysbiosis is associated with Henoch-Schonlein Purpura in children. Int. Immunopharmacol. 58, 1–8. doi: 10.1016/j.intimp.2018.03.003

PubMed Abstract | CrossRef Full Text | Google Scholar

Wang, Y., Guo, Y., Chen, H., Wei, H., and Wan, C. (2018). Potential of Lactobacillus plantarum ZDY2013 and Bifidobacterium bifidum WBIN03 in relieving colitis by gut microbiota, immune, and anti-oxidative stress. Can. J. Microbiol. 64, 327–337. doi: 10.1139/cjm-2017-0716

PubMed Abstract | CrossRef Full Text | Google Scholar

Weck, M. N., Gao, L., and Brenner, H. (2009). Helicobacter pylori infection and chronic atrophic gastritis: associations according to severity of disease. Epidemiology 20, 569–574. doi: 10.1097/EDE.0b013e3181a3d5f4

PubMed Abstract | CrossRef Full Text | Google Scholar

Wexler, H. M. (2007). Bacteroides: the good, the bad, and the nitty-gritty. Clin. Microbiol. Rev. 20, 593–621. doi: 10.1128/CMR.00008-07

PubMed Abstract | CrossRef Full Text | Google Scholar

Weyermann, M., Rothenbacher, D., and Brenner, H. (2009). Acquisition of Helicobacter pylori infection in early childhood: independent contributions of infected mothers, fathers, and siblings. Am. J. Gastroenterol. 104, 182–189. doi: 10.1038/ajg.2008.61

PubMed Abstract | CrossRef Full Text | Google Scholar

Xun, W., Shi, L., Zhou, H., Hou, G., Cao, T., and Zhao, C. (2015). Effects of curcumin on growth performance, jejunal mucosal membrane integrity, morphology and immune status in weaned piglets challenged with enterotoxigenic Escherichia coli. Int. Immunopharmacol. 27, 46–52. doi: 10.1016/j.intimp.2015.04.038

PubMed Abstract | CrossRef Full Text | Google Scholar

Yang, Y. J., and Sheu, B. S. (2012). Probiotics-containing yogurts suppress Helicobacter pylori load and modify immune response and intestinal microbiota in the Helicobacter pylori-infected children. Helicobacter 17, 297–304. doi: 10.1111/j.1523-5378.2012.00941.x

PubMed Abstract | CrossRef Full Text | Google Scholar

Zaman, C., Osaki, T., Hanawa, T., Yonezawa, H., Kurata, S., and Kamiya, S. (2014). Analysis of the microbial ecology between Helicobacter pylori and the gastric microbiota of Mongolian gerbils. J. Med. Microbiol. 63, 129–137. doi: 10.1099/jmm.0.061135-0

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhu, W., Lin, K., Li, K., Deng, X., and Li, C. (2018). Reshaped fecal gut microbiota composition by the intake of high molecular weight persimmon tannin in normal and high-cholesterol diet-fed rats. Food Funct. 9, 541–551. doi: 10.1039/c7fo00995j

PubMed Abstract | CrossRef Full Text | Google Scholar

Zitomersky, N. L., Atkinson, B. J., Franklin, S. W., Mitchell, P. D., Snapper, S. B., Comstock, L. E., et al. (2013). Characterization of adherent bacteroidales from intestinal biopsies of children and young adults with inflammatory bowel disease. PLoS ONE 8:e63686. doi: 10.1371/journal.pone.0063686

PubMed Abstract | CrossRef Full Text | Google Scholar