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  • Research article
  • Open Access
  • Open Peer Review

Gastric bacterial Flora in patients Harbouring Helicobacter pylori with or without chronic dyspepsia: analysis with matrix-assisted laser desorption ionization time-of-flight mass spectroscopy

  • 1,
  • 1Email author,
  • 2 and
  • 3
BMC GastroenterologyBMC series – open, inclusive and trusted201818:20

https://doi.org/10.1186/s12876-018-0744-8

  • Received: 17 October 2017
  • Accepted: 14 January 2018
  • Published:
Open Peer Review reports

Abstract

Background

The gastric microbiota has recently been implicated in the causation of organic/structural gastroduodenal diseases (gastric and duodenal ulcers, gastric cancer) in patients with Helicobacter pylori (H. pylori) infection. We aimed to ascertain, in patients harbouring H. pylori, the role of the gastric microbiota in the causation of symptoms (chronic dyspepsia) in the absence of organic disease.

Methods

Seventy-four gastric biopsy samples obtained at endoscopy from patients with (n = 21) or without (n = 53) chronic dyspepsia, and that tested positive by the bedside rapid urease test for H. pylori infection, were cultured for detection of H. pylori and non-H. pylori organisms. The cultured organisms were identified by matrix-assisted laser desorption ionization time-of-flight mass spectroscopy (MALDI-TOF MS).

Results

A total of 106 non-H. pylori isolates were obtained from 74 patients’ samples. This included 33 isolates (median 2, range 1–2 per patient) from dyspeptic and 73 (median 2, range 1–2 per patient) from non-dyspeptic patients. These were identified from the Bruker Biotyper 2 database as Staphylococcus spp., Streptococcus spp., Lactobacillus spp., Micrococcus spp., Enterococcus spp., Pseudomonas spp., Escherichia spp., Klebsiella spp. and Bacillus spp., Staphylococcus and Lactobacillus were identified significantly more commonly in dyspeptics and Streptococcus, Pseudomonas, Escherichia coli and Klebsiella pneumoniae in non-dyspeptics. All identified organisms belonged to the phyla Firmicutes and Proteobacteria.

Conclusions

There is a qualitative difference in the gastric microbial spectrum between patients harbouring H. pylori with and without chronic dyspepsia. Whether these organisms have an independent role in the development or prevention of dyspepsia or act in concurrence with H. pylori needs study.

Keywords

  • Gastric microbiome
  • Gastric microbiota
  • Helicobacter pylori pathogenicity
  • MALDI-TOF

Background

Traditionally, the human stomach has been viewed as an inhospitable environment for microorganisms mainly because of its acidic lumen [1]. With the discovery of Helicobacter pylori (H. pylori) and other gastric Helicobacters, and subsequent insight into the mechanisms by which these organisms adapt to the gastric environment, the stomach is no longer considered sterile and the adaptative mechanisms of local organisms are becoming clearer [2].

Bacterial counts in the human stomach were traditionally believed to range from 0 to 103 cfu/g [3]; these figures were based on studies with organisms that can be cultured and identified by standard biochemical techniques. More advanced techniques have brought to light one fact: the normal stomach is host to many more organisms than have been identified by standard culture techniques. Studies found colonisation by a complex microbiota belonging mainly to the Proteobacteria, Firmicutes, Actinobacteria and Fusobacterium phyla, which was clearly different from the microbiota described in the mouth and oesophagus [4]. A high prevalence of non-H. pylori bacteria has been found, the majority of which were Streptococcus and Staphylococcus [5, 6].

H. pylori infects up to 50% of the world’s population [3]. It has been implicated in the causation of various gastroduodenal (duodenal ulcers, MALT lymphoma, gastric cancer) as well as extraintestinal (e.g., refractory anaemia, idiopathic thrombocytopenic purpura) diseases [7]. Why only a small fraction of those infected will progress to disease development has been the subject of extensive investigation. Several pathogenic factors have been identified within the organism that enable colonisation and progression to disease [3]. Recent attention has also focused on host factors [68], with increasing interest in the role of the gastric microbiota particularly in the causation of gastric cancer, in the presence of H. pylori infection [914]. The role of the human gut microbiota in health and disease in general has been reviewed in detail recently [15].

More common than the development of organic disease is the development of symptoms (chronic dyspepsia) in patients with H. pylori infection even in the absence of organic disease (so-called functional dyspepsia). Although the role of H. pylori infection in functional dyspepsia is still being debated, eradication of the infection with antibacterial therapy has been shown to provide symptom relief more than with placebo [16]. It is not clear whether the relief is due to eradication of this infection or of any concurrent gastric bacterial population [17]. In support of an important role for non-H. pylori bacteria in the causation of disease is the finding in a longitudinal study that treatment for H. pylori decreased the occurrence of gastric cancer even in those in whom the organism could not be eradicated [18].

A qualitative difference in the gastric microbiota in persons infected with H. pylori has been mentioned [8, 9]; which of the two (H. pylori and non-H. pylori bacteria) influenced the other is not clear. Little is known about the gastric microbiota in patients with H. pylori infection with dyspepsia in the absence of organic disease.

Finally, there is information on the gastric microflora in the West [4, 10, 1214], but reports on the gastric microbiota in developing countries are few [8]. The gastric microbiota of Indian subjects has not been studied by advanced techniques. Why is this important? We expect it to be different in developing countries from what has been reported from the more hygienic environs of the West. Besides, in the context of H. pylori infection, it is worth noting that while antibody to this infection is rather widespread in a country like India [19], the incidence of gastric cancer is not as high as would then be expected [20]; the reasons for this are only speculative [21].

Our primary aim was therefore to characterise the culturable gastric microbiota in patients with H. pylori infection with or without chronic dyspepsia in the absence of organic disease. Simultaneously we wished to determine if there is any qualitative difference in the Indian gastric microbiota as compared to that described from the West, in the presence of H. pylori infection. For these purposes, we used matrix-assisted laser desorption ionization time-of-flight mass spectrometry (MALDI-TOF MS) for bacterial identification [22]. A higher accuracy is obtained with this technique compared with the phenotypic methods reported before [23].

Methods

Subjects

During an 11-month period (September 2013 – August 2014), 74 consecutive patients (40 men, 34 women) undergoing upper gastrointestinal endoscopy for indications decided by their treating physician, who had not received any antibiotic for three months prior or acid-suppression therapy for four weeks prior, and who consented to obtaining endoscopic gastric biopsy for the purpose of the study, were enrolled. Patients who had comorbid illness (e.g., renal failure, chronic NSAID use) or obvious organic disease on endoscopy (ulcers, cancer) that can cause dyspepsia were excluded.

With diligent sterile precautions and after flushing the endoscope working channel with sterile normal saline, two sets each of mucosal biopsy samples were taken using single-use forceps, from the gastric antrum and body. One set was placed in a commercial urea-based strip (Halifax Research Laboratory, Kolkata) for the bedside rapid urease test (RUT) for H. pylori infection. The second set was transported in ice packs at 4 °C to the culture laboratory within an hour of collection, using sterile 0.9% saline as transport medium. Samples that yielded positive results on RUT were taken for H. pylori culture and further examinations. Tissue was not taken for histologic examination.

The institution’s Ethics Committee reviewed and approved the study protocol (reference number 760-PA-13 dated August 22, 2013) and informed written consent was obtained from each patient.

The 74 patients were divided into two groups, namely, those with chronic dyspepsia (greater than six months’ duration) as the indication for endoscopy (dyspeptics; n = 21; median age 48, range 21 to 66 years) and those whose indications for endoscopy were other than dyspepsia (non-dyspeptics; n = 53; median age 47, range 22 to 79 years). As mentioned earlier, those with organic disease that can cause dyspepsia were excluded. The dyspeptics group thus had functional dyspepsia, as defined by the Rome III criteria [24]. The non-dyspeptic group included patients with the following indications: dysphagia, anaemia suspected to be due to gastrointestinal blood loss, search for primary cancer, and screening for varices in portal hypertension.

Tissue culture

The selected samples were dispersed using a homogeniser. Each homogenate was inoculated into sterile tryptic soy broth and the samples were plated on non-selective Brucella blood agar and Mueller Hinton agar plates supplemented with 5% human blood, starch and human serum. They were then incubated at 37 °C under microaerophilic, aerobic and anaerobic conditions for 5 to 7 days.

Small translucent colonies were selected for Giemsa’s staining and tested for urease, catalase and oxidase activity. Curved rods resembling Helicobacter that were positive for all the three enzyme activity tests were identified as H. pylori.

The non-H. pylori colonies were subjected to Gram staining and colony characteristics study (size, shape, colour, margins, opacity, elevation), and to MALDI-TOF MS for identification.

Identification by MALDI-TOF MS

The method we used was similar to that used by Hu et al. [23] Approprimately 5–10 mg of colony was scraped and suspended in 300 μL deionized water in an Eppendorf tube and mixed; 900 μL ethanol was added to it and further mixed. The sample was then centrifuged at 12000 rpm for 2 min. The supernatant was decanted and centrifuged again and the ethanol was pipetted off without disturbing the bacterial pellet, which was then dried for 2–3 min. Fifty μL formic acid (70% in water) was added to the dry pellet and mixed, and 50 μL acetonitrile was then added. After centrifugation again at 12000 rpm for 2 min, 1 μL of the supernatant containing the bacterial extract was transferred on to the 96-well steel plate and dried. One μL of matrix solution containing saturated solution of cyano-4-hydroxycinnamic acid in 50% acetonitrile + 2.5% trifluoroacetic acid was added and allowed to air dry at room temperature.

Measurement was done with Microflex LT mass spectrometer (Bruker Daltonics; Germany) equipped with a 200 Hz smartbeam laser. The parameter settings were as follows: delay 320 ns; ion source (i) 20 kV; ion source (ii) 18.5 kV, lens voltage 8.5 kV; and mass range 2–15 kDa. Each run was validated with an Escherichia coli (E. coli) control sample where the presence of 10 specific proteins ensured that the spectrometer was set properly. Raw spectra of the strains were analysed by MALDI Biotyper 2.0 software (Bruker Daltonics; Germany) using the default settings.

A list of peaks up to 100 was generated. The threshold for peak acceptance was a signal-to-noise (S/N) ratio of 3. After alignment, peaks with a mass-to-charge (m/z) ratio difference of less than 200 ppm were considered to be identical. The peak lists generated were used for matches against the reference library, by directly using the integrated pattern-matching algorithm of the software. All parameters were the same regardless of the bacteria analysed [3] and a score was attributed to each identification.

Statistical analysis

Fisher’s exact test was used to compare the frequency of micro-organisms in dyspeptic patients and non-dyspeptic patients.

Results

The ATCC culture of E. coli (positive control) was correctly identified with a score of > 2. The yields on both plates (Brucella blood agar and Mueller Hinton agar) were identical for the types of organisms, as identified on MALDI-TOF.

From the 74 biopsy samples, 106 isolates were obtained. These included 33 isolates (median 2, range 1 to 2 per patient) from dyspeptic and 73 (median 2, range 1–2 per patient) from non-dyspeptic patients; there was no difference in the isolation rates between the two groups.

The 106 isolates included 32 of Staphylococcus spp., 29 of Streptococcus spp., 18 of Lactobacillus spp., 11 of Klebsiella pneumoniae, 8 of Escherichia coli, 5 of Pseudomonas mosselii, and one each of Micrococcus, Enterococcus faecium and Bacillus (Fig. 1). All the organisms identified belonged to the phyla Firmicutes and Proteobacteria. The Staphylococcus species identified included Staph. aureus, Staph. equorum, Staph. haemolyticus, Staph. auricularis, Staph. hominis, Staph. warneri and Staph. xylosus. The Streptococcus species identified included Strep. salivarius, Strep. oralis, Strep. sanguinis, Strep. gordonii and Strep. parasanguinis. The Lactobacillus species included L. brevis and L. paracasei. Micrococcus luteus, Enterococcus faecium, Pseudomonas mosselii, Escherichia coli, Klebsiella pneumonia, and Bacillus spp. were the others identified.
Fig. 1
Fig. 1

Genera isolated in the two groups (dyspeptics and non-dyspeptics) with H. pylori infection

Staphylococcus spp. and Lactobacillus spp. were significantly more commonly identified in dyspeptics; Streptococcus spp., Pseudomonas mosselii, Escherichia coli and Klebsiella pneumoniae were more common in non-dyspeptics (Tables 1 and 2).
Table 1

Genera isolated in the two groups (dyspeptics and non-dyspeptics) with H. pylori infection

Genera

Dyspeptic (n = 21)

Non-dyspeptic (n = 53)

p value

 

No. (%)

No. (%)

 

Staphylococcus

19 (90.5)

13 (24.5)

0.00

Streptococcus

2 (9.5)

27 (50.9)

0.0011

Lactobacillus

10 (47.6)

8 (15)

0.0060

Micrococcus

1 (4.8)

0 (0)

0.2837

Enterococcus

1 (4.8)

0 (0)

0.2837

Pseudomonas

0 (0)

5 (9.4)

0.0625

Escherichia

0 (0)

8 (15)

0.007

Klebsiella

0 (0)

11 (20.8)

0.0009

Bacillus

0 (0)

1 (1.9)

1

Total No.

33

73

 

Total of 106 species were identified from 74 samples

Table 2

Species isolated in the two groups (dyspeptics and non-dyspeptics) with H. pylori infection

Micro-organisms

Dyspeptic (n = 21)

Non-dyspeptic (n = 53)

Staphylococcus aureus

8 (38.1%)

5 (9.4%)

Staphylococcus equorum

1 (4.8%)

0

Staphylococcus haemolyticus

3 (14.3%)

2 (3.8%)

Staphylococcus auricularis

1 (4.8%)

0

Staphylococcus hominis

2 (9.5%)

3 (5.7%)

Staphylococcus warneri

4 (19.1%)

0

Staphylococcus xylosus

0

3 (5.7%)

Streptococcus salivarius

0

11 (20.8%)

Streptococcus oralis

1 (4.8%)

4 (7.6%)

Streptococcus sanguinis

0

8 (15.1%)

Streptococcus gordonii

1 (4.8%)

0

Streptococcus parasanguinis

0

4 (7.6%)

Lactobacillus brevis

5 (23.8%)

8 (15.1%)

Lactobacillus paracasei

5 (23.8%)

0

Micrococcus luteus

1 (4.8%)

0

Enterococcus faecium

1 (4.8%)

0

Pseudomonas mosselii

0

5 (9.4%)

Escherichia coli

0

8 (15.1%)

Klebsiella pneumoniae

0

11 (20.8%)

Bacillus spp

0

1 (1.9%)

Total No.

33

73

The MALDI-TOF spectra of the four commonest identified species are shown in Fig. 2.
Fig. 2
Fig. 2

MALDI-TOF MS spectra of 4 commonest organisms isolated (a Pseudomonas mosselii; b Staphylococcus aureus; c Escherichia coli; d Lactobacillus brevis)

Discussion

We describe a qualitative difference in the bacterial spectrum in subjects with H. pylori infection who do and do not have chronic dyspepsia. The former excluded patients who had obvious organic gastroduodenal or systemic disease that could cause dyspepsia, and met the Rome III criteria for functional dyspepsia [24]. No subgroup analysis (as epigastric pain syndrome and postprandial distress syndrome) was done. We excluded patients who had recently received antibiotic or acid-suppression therapy; none of our patients was on long-term NSAID use. Subsequent to the initiation of our study, the Rome IV diagnostic criteria for functional dyspepsia were introduced [25]. These differ importantly from the Rome III criteria by defining a severity threshold for identifying symptom as ‘bothersome’ and by providing a cut-off for symptom frequency.

Since it would be unethical to perform endoscopies and obtain biopsies in persons without gastroduodenal indications (truly healthy individuals), our comparator group was a diseased-control group that had patients with the infection but without dyspepsia even if they had other structural disease.

Studies from the West have explored the gastric microbiota in the absence and presence of H. pylori infection [11]; several studies have also explored the role of the gastric microbiota in the development of structural disease, particularly gastric cancer, in the presence of H. pylori infection [1014]. We attempted to address the issue of why some individuals with H. pylori infection develop chronic dyspepsia and others do not, a clinical scenario that is much more common in this infection than the development of structural disease.

We found Staphylococcus spp., Streptococcus spp. and Lactobacillus spp. as the most frequently identified organisms in the samples we studied. The species we isolated on cuture belonged to the phyla Firmicutes and Proteobacteria; Bik et al [4] and others from the West [1214] reported (on 16 s rRNA sequencing) the presence of Proteobacteria, Firmicutes, Actinobacteria, Bacteroidetes and Fusobacteria phyla in the stomach of those with H. pylori infection. Interestingly, the flora in H. pylori-positive patients with chronic dyspepsia in our study was dominated by Staphylococcus and Lactobacillus (in that order of prevalence); those without dyspepsia showed dominance by Streptococcus, Staphylococcus and Klebsiella. There was a significant difference in the organisms in the two groups, with Staphylococcus and Lactobacillus more commonly identified in dyspeptics and Streptococcus, Pseudomonas, Escherichia coli and Klebsiella pneumoniae more common in non-dyspeptics. Lactobacillus is one of the species that has been incriminated in the progression to gastric cancer in H. pylori-positive individuals [26].

A role for H. pylori in the causation of gastroduodenal disease (acid-peptic diseases, low-grade MALT lymphoma, carcinoma) has been established [27, 28]. However, a question that remains is why only some individuals with this infection develop disease while the majority do not. H. pylori virulence factors have been extensively studied in this regard [3]; factors such as the host diet have also been studied, but a clear answer has not been forthcoming. A role for host environment factors (gastric microbiome) has recently received extensive attention [8, 10, 23]. However, we are not aware of studies that attempted to differentiate the gastric microbiota in individuals with H. pylori infection, between those with chronic (functional) dyspepsia and those without dyspepsia.

An earlier study by Hu et al [23] had shown that a higher proportion of patients with non-ulcer (functional) dyspepsia had non-H. pylori flora as compared to those with gastric ulcer [23], suggesting a role for these concurrent organisms in the causation of symptoms. They, however, did not specify any qualitative difference. They observed an overall high prevalence of Streptococcus, Neisseria, Rothia and Staphylococcus in their patients with H. pylori infection; we observed a high prevalence of Staphylococcus spp. and Lactobacillus spp. in chronic dyspeptics and Streptococcus spp., Pseudomonas, Escherichia coli and Klebsiella pneumoniae in non-dyspeptics. Of these, Staphylococcus and Klebsiella are urease-producing organisms.

We suggest a possibility that some or all of these organisms play a role (bacteria-bacteria, bacteria-host, or bacteria-host-bacteria) in the causation of symptoms in H. pylori infection. What the range of interactions among human-associated microbes might be is not clear, nor how this may influence host health or disease [29]. Maldonado-Contreras et al [8] have suggested various mechanisms of interactions between H. pylori and non-H. pylori organisms in the stomach. The interactions of H. pylori with the other bacteria detected in the stomach may be influenced by host response [3, 5, 6, 8, 3032]. It is likely that H. pylori creates special niches that allow the survival and colonisation of bacteria in the stomach [33].

It is well known that colonisation by H. pylori leads to changes in the gastric milieu, including raising the pH to > 4, which facilitates colonisation by other bacteria [34]. Multiple non-H. pylori organisms have been isolated from the stomach in patients with hypochlorhydria [35]. It could be that the spectrum we obtained was influenced by concomitant H. pylori infection. But, if it was, we would expect the influence to be similar in both our study groups, namely, dyspeptics and non-dyspeptics.

On the other hand, Bik et al. [4], who used a metagenomic approach, found no influence of H. pylori on the diversity of gastric microbiota. They also showed that there is no difference in the microbiota isolated from the gastric antrum and corpus, which justifies our decision to pool samples from these two regions. The relationship between H. pylori and the gastric microbiota is thus still controversial [33].

We also describe, probably for the first time, the culturable gastric flora in an Indian population, as identified using MALDI-TOF MS, a technique that identifies organisms more reliably than the standard culture techniques (morphology and biochemical tests) [36]. The organisms we identified in H. pylori-positive individuals may not reflect the spectrum in the general (asymptomatic) Indian population, and so cannot be compared with studies from the healthy population in the West.

Our study had limitations. We used culture (and MALDI-TOF MS) as the identifying technique; this identifies only viable microflora. Metagenomics is a high-end technique that will increase the yield of the microflora by also identifying DNA from dead organisms. Which of these is a more faithful representation of the functional microflora is not clear [26]. Importantly, we did not study the gastric histology in our subjects, and so cannot comment on the presence or absence of inflammation and atrophy, common accompaniments of H. pylori infection. This could be a major confounder: the gastric environment, including the pH and the presence of inflammation, can obviously influence the microbial spectrum. Besides, the presence of inflammation and/or atrophy may be an indicator of the virulence of the H. pylori strains in these patients, a factor we did not study; the latter could contribute to the development of symptoms in addition to possibly influencing the concomitant microflora. We also had no information on the smoker status of our patients. Finally, we did not explore the potential pathogenicity of bacterial types we isolated. Although some of the organisms we isolated are known to be pathogens in other sites and clinical situations, we do not know yet about their pathogenic ability in the gastric environs.

Information regarding the contribution of the concurrent gastrointestinal microbiome to the development of disease is still in its infancy. Future studies are needed to elucidate whether and to what extent H. pylori infection perturbs the established microbiota, and how the concomitant microbiota influence development of symptoms and disease. Such studies should factor in the limitations in our study, in order to get a clearer understanding. Increasing evidence supports the hypothesis that although H. pylori is the most relevant, it may not be the only local bacterial culprit leading to gastric diseases. There may be a role for non-H. pylori components of the gastric microbiota in both gastric and extragastric diseases. Conversely, some components of the gastric microbiota have been shown to exert antibacterial and probiotic properties, which may be exploited for the prevention and treatment of gastric diseases [37].

Conclusions

The changes that take place in the gastric environment during H. pylori infection are complex and involve several factors. A combination of these would determine not only the composition of the gastric microbiota but also the progress toward different diseases [32]. Our finding of gastric flora dominated by Staphylococcus followed by Lactobacillus in patients with H. pylori-positive chronic dyspepsia and by Streptococcus followed by Staphylococcus and Klebsiella (along with gram-negative bacteria) in those without dyspepsia adds an area of interest in the interaction of bacteria in the causation of symptoms. These findings add to the now-popular belief that individual bacteria identified in individual gut disease may not be lone players but may be influenced in their pathogenicity by the community they live in. Although this is an attractive proposition, it is too early to state whether manipulating the concomitant microflora will offer an alternative approach to preventing or managing these diseases or symptoms.

Declarations

Acknowledgements

We thank the doctors of the Division of Gastroenterology and nurses in the Endoscopy Suite of P D Hinduja Hospital for kindly providing us the biopsy samples. We also thank the staff of the Division of Microbiology for their co-operation and support. We are grateful to the National Education Society for the intramural funding for this project.

Funding

This work was supported by an intramural grant from the National Education Society of P D Hinduja Hospital, Mahim, Mumbai 400016, India. The funding agency had no role in the design of the study and collection, analysis, and interpretation of data and in writing the manuscript.

Availability of data and materials

The datasets used and/or analysed during the current study are available from the corresponding author on reasonable request.

Authors’ contributions

PA conceived and designed the work. VP collected the data. VP, SN and AS analysed the data. VP and PA interpreted the data and drafted the article. All authors critically revised the article and approved the final manuscript.

Ethics approval and consent to participate

The institution’s Ethics Committee reviewed and approved the study protocol (reference number 760-PA-13 dated August 22, 2013) and informed written consent was obtained from each patient.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests

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Authors’ Affiliations

(1)
Division of Gastroenterology, P D Hinduja Hospital, V S Marg, Mahim, Mumbai, 400016, India
(2)
Bruker Daltonics, Bangalore, India
(3)
Division of Microbiology, P D Hinduja Hospital, Mumbai, India

References

  1. Von Rosenvinge EC, O’May GA, Macfarlane S, Macfarlane GT, Shirtliff ME. Microbial biofilms and gastrointestinal diseases. Pathog Dis. 2013;67(1):25–38.View ArticlePubMedPubMed CentralGoogle Scholar
  2. Merrell DS, Goodrich ML, Otto G, Lucy S, Falkow S, Tompkins LS. pH-regulated gene expression of the gastric pathogen helicobacter pylori. Infect Immun. 2003;71(6):3529–39.View ArticlePubMedPubMed CentralGoogle Scholar
  3. Sheh A, Fox JG. The role of the gastrointestinal microbiome in helicobacter pylori pathogenesis. Gut Microbes. 2013 Jan 19;4(6):505–31.View ArticlePubMedPubMed CentralGoogle Scholar
  4. Bik EM, Eckburg PB, Gill SR, Nelson KE, Purdom EA, Francois F, et al. Molecular analysis of the bacterial microbiota in the human stomach. Proc Natl Acad Sci U S A. 2006 Jan 17;103(3):732–7.View ArticlePubMedPubMed CentralGoogle Scholar
  5. Yang I, Nell S, Suerbaum S. Survival in hostile territory: the microbiota of the stomach. FEMS Microbiol Rev. 2013;37(5):736–61.View ArticlePubMedGoogle Scholar
  6. Zilberstein B, Quintanilha AG, MAA S, Pajecki D, Moura EG, PRA A, et al. Digestive tract microbiota in healthy volunteers. Clinics (Sao Paulo). 2007 Feb;62(1):47–54.View ArticleGoogle Scholar
  7. Malfertheiner P, Megraud F, O’Morain CA, Gisbert JP, Kuipers EJ, Axon AT, et al. Management of Helicobacter pylori infection – the Maastricht V/Florence consensus report. Gut. 2017 Jan;66(1):6–30.View ArticlePubMedGoogle Scholar
  8. Maldonado-Contreras A, Goldfarb KC, Godoy-Vitorino F, Karaoz U, Contreras M, Blaser MJ, et al. Structure of the human gastric bacterial community in relation to helicobacter pylori status. ISME J. 2011 Apr;5(4):574–9.View ArticlePubMedGoogle Scholar
  9. Coker OO, Dai Z, Nie Y, Zhao G, Cao L, Nakatsu G, et al. Mucosal microbiome dysbiosis in gastric carcinogenesis. Gut 2017 Aug 1; 2017–314281 (Epub ahead of print).Google Scholar
  10. Abreu MT, Peek RM Jr. Gastrointestinal malignancy and the microbiome. Gastroenterology. 2014 May;146(6):1534–46.View ArticlePubMedPubMed CentralGoogle Scholar
  11. Khosravi Y, Dieye Y, Poh B. Culturable bacterial microbiota of the stomach of helicobacter pylori positive and negative gastric disease patients. Sci World. 2014;2014:610421.Google Scholar
  12. Li TH, Qin Y, Sham PC, Lau KS, Chu K-M, Leung WK. Alterations in gastric microbiota after H. Pylori eradication and in different histological stages of gastric carcinogenesis. Sci Rep. 2017;7:44935.View ArticlePubMedPubMed CentralGoogle Scholar
  13. Yu G, Torres J, Hu N, Medrano-Guzman R, Herrera-Goepfert R, Humphrys MS, et al. Molecular characterization of the human stomach microbiota in gastric cancer patients. Front Cell Infect Microbiol. 2017;7:302 (online).Google Scholar
  14. Sohn S-H, Kim N, Jo HJ, Kim J, Park JH, Nam RH, et al. Analysis of gastric body microbiota by pyrosequencing: possible role of bacteria other than Helicobacter pylori in the gastric carcinogenesis. J Cancer Prev. 2017 Jun 30;22(2):115–25.View ArticlePubMedPubMed CentralGoogle Scholar
  15. Wang B, Yao M, Lv L, Ling Z, Li L. The human microbiota in health and disease. Engineering. 2017 Feb 1;3(1):71–82.Google Scholar
  16. Suzuki H, Moayyedi P. Helicobacter pylori infection in functional dyspepsia. Nat Rev Gastroenterol Hepatol. 2013;10:168–74.View ArticlePubMedGoogle Scholar
  17. Holtmann G, Talley NJ. Functional dyspepsia. Curr Opin Gastroenterol. 2015 Nov;31(6):492–8.PubMedGoogle Scholar
  18. Ma JL, Zhang L, Brown LM, Li JY, Shen L, Pan KF, et al. Fifteen-year effects of Helicobacter pylori, garlic, and vitamin treatments on gastric cancer incidence and mortality. J Natl Cancer Inst. 2012;104(6):488–92.View ArticlePubMedPubMed CentralGoogle Scholar
  19. Tewari R, Nijhawan V, Mishra M, Cleary JM, Salopal T, Martínez-Lorenzana G, et al. Prevalence of helicobacter pylori, cytomegalovirus, and chlamydia pneumoniae immunoglobulin seropositivity in coronary artery disease patients and normal individuals in north Indian population. Med J Armed Forces India. 1998;68(1):53–7.View ArticleGoogle Scholar
  20. Ghoshal UC, Chaturvedi R, Correa P. The enigma of helicobacter pylori infection and gastric cancer. Indian J Gastroenterol. 2010;29(3):95–100.View ArticlePubMedPubMed CentralGoogle Scholar
  21. Misra V, Pandey R, Misra SP, Dwivedi M. Helicobacter pylori and gastric cancer: Indian enigma. World J Gastroenterol. 2014;20(6):1503–9.View ArticlePubMedPubMed CentralGoogle Scholar
  22. Clark AE, Kaleta EJ, Arora A, Wolk DM. Matrix-assisted laser desorption ionization - time of flight mass spectrometry: a fundamental shift in the routine practice of clinical microbiology. Clin Microbiol Rev. 2013 Jul 3;26(3):547–603.View ArticlePubMedPubMed CentralGoogle Scholar
  23. Hu Y, He L-H, Xiao D, Liu G-D, Gu Y-X, Tao X-X, et al. Bacterial flora concurrent with helicobacter pylori in the stomach of patients with upper gastrointestinal diseases. World J Gastroenterol. 2012 Mar 21;18(11):1257–61.View ArticlePubMedPubMed CentralGoogle Scholar
  24. Tack J, Talley NJ, Camilleri M, Hollmann G, Hu P, Malagelada JR, et al. Functional gastroduodenal disorders. Gastroenterology. 2006;130:1466–79.View ArticlePubMedGoogle Scholar
  25. Stanghellini V, Chan FKL, Hasler WL, Malagelada JR, Suzuki H, Tack J, Talley NJ. Gastroduodenal disorders. Gastroenterology. 2016;150:1380–92.View ArticlePubMedGoogle Scholar
  26. Noto JM, Peek RM Jr. The gastric microbiome, its interaction with Helicobacter pylori, and its potential role in the progression to stomach cancer. PLoS Pathog. 2017;13(10):e1006573.View ArticlePubMedPubMed CentralGoogle Scholar
  27. Linz B, Balloux F, Moodley Y, Manica A, Liu H, Roumagnac P, et al. An African origin for the intimate association between humans and helicobacter pylori. Nature. 2007 Feb 22;445(7130):915–8.View ArticlePubMedPubMed CentralGoogle Scholar
  28. Kusters JG, van Vliet AHM, Kuipers EJ. Pathogenesis of helicobacter pylori infection. Clin Microbiol Rev. 2006 Jul;19(3):449–90.View ArticlePubMedPubMed CentralGoogle Scholar
  29. Faust K, Sathirapongsasuti JF, Izard J, Segata N, Gevers D, Raes J, Huttenhower C. Microbial co-occurrence relationships in the human microbiome. PLoS Comput Biol. 2012;8(7):e1002606.View ArticlePubMedPubMed CentralGoogle Scholar
  30. Wen Y, Marcus EA, Matrubutham U, Gleeson MA, Scott DR, Sachs G. Acid-adaptive genes of helicobacter pylori. Infect Immun. 2003 Oct;71(10):5921–39.View ArticlePubMedPubMed CentralGoogle Scholar
  31. Moyat M, Velin D. Immune Responses to helicobacter pylori infection. World J Gastroenterol. 2014 May 21;20(19):5583–93.View ArticlePubMedPubMed CentralGoogle Scholar
  32. Yarandi SS, Hebbar G, Sauer CG, Cole CR, Ziegler TR. Diverse roles of leptin in the gastrointestinal tract: modulation of motility, absorption, growth, and inflammation. Nutrition. 2011 Mar;27(3):269–75.View ArticlePubMedGoogle Scholar
  33. Nardone G, Compare D. The human gastric microbiota: is it time to rethink the pathogenesis of stomach diseases? United Eur Gastroenterol J. 2015;3(3):255–60.View ArticleGoogle Scholar
  34. Human CP. Gastric carcinogenesis: a multistep and multifactorial process – first American Cancer Society award lecture on cancer epidemiology and prevention. Cancer Res. 1992 Dec 15;52(24):6735–40.Google Scholar
  35. Williams C, KE MC. Proton pump inhibitors and bacterial overgrowth. Aliment Pharmacol Ther. 2006 Jan 1;23(1):3–10.View ArticlePubMedGoogle Scholar
  36. Calderaro A, Arcangeletti M-C, Rodighiero I, Buttrini M, Gorrini C, Motta F, et al. Matrix-assisted laser desorption/ionization time-of- flight (MALDI-TOF) mass spectrometry applied to virus identification. Sci Rep. 2014 Jan;4:6803.Google Scholar
  37. Ianiro G, Molina-Infante J, Gasbarrini A. Gastric microbiota. Helicobacter. 2015;20:68–71.View ArticlePubMedGoogle Scholar

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