- Research article
- Open Access
- Open Peer Review
Characterization of gut microbiota in children with pulmonary tuberculosis
BMC Pediatrics volume 19, Article number: 445 (2019)
Gut microbiota plays a critical role in many important physiological processes and is linked with various pulmonary infectious diseases. The relationship between pulmonary tuberculosis (PTB) and gut microbiota has been poorly studied. The present study aimed to characterize gut microbiota in pediatric patients with PTB.
A case-controlled study was executed for the characterization of gut microbiota in pediatric PTB patients. Fecal samples were collected from the PTB patients and healthy controls upon admission. In addition, a one-month follow-up assessment was performed to investigate alterations in the gut microbiota post anti-tuberculosis treatment. 16SrDNA sequencing analysis of fecal DNA was completed on the Illumina MiSeq platform.
Compared with healthy controls, the gut microbiota of pediatric patients with PTB was characterized by decreased microbial diversity. PTB patients further presented an up-regulation of the pro-inflammatory bacteria Prevotella, the opportunistic pathogen Enterococcus, as well as a reduction of beneficial bacteria including Ruminococcaceae, Bifidobacteriaceae and prausnitzii. One-month after anti-tuberculosis therapy, the richness of gut microbiota in PTB patients was distinctly depleted.
The gut microbiota of pediatric patients with PTB was significantly distinct from healthy controls. Additionally, the richness of gut microbiota in PTB patients decreased after one-month anti-tuberculosis treatment. It is hypothesized that the homeostasis of gut microbiota in PTB patients may affect the pathogenies of PTB by de-regulation of the hosts’ immune status through the gut-lung axis.
Tuberculosis (TB) is one of the most common infectious disease in the world and the leading cause of death from a single infectious agent. TB is caused by Mycobacterium tuberculosis, a bacterium which attacks the lungs predominantly but can affect other organs as well. According to a 2018 WHO report, there were approximately 10.0 million people acquiring TB in 2017. Further, TB caused an estimated 1.3 million deaths in 2017. In addition to the high rate of TB incidence, a growing concern is the prevalence of drug-resistant TB. In 2017, 558,000 new TB patients exhibited resistance to the first-line drug rifampicin, more than 80% of which demonstrated eventual multidrug-resistant TB . Thus, TB remains a significant public health problem requiring effective interventions.
With the development of next-generation high-throughput sequencing, the investigation of the human gut microbiome has become more feasible and has led to insights into gut microbiota. Gut microbiota are a complex and dynamic ecosystem harbouring more than 100 trillion commensal microorganisms, surpassing the number of human cells . A great amount of evidence suggests that the gut microbiota exerts many beneficial effects on humans through the involvement physiological processes including digestion and absorption of nutrition, modulation of the immune system, and protection against pathogenic invasion [3,4,5,6,7]. Increasing lines of evidence have further indicated that the gut microbiota are linked to some systemic infectious diseases [8,9,10] such as HIV infection, chronic hepatitis C and bloodstream infection. In addition, the critical role of gut microbiota in pulmonary infectious disease has also been increasingly recognized and a vital cross-talk mechanism between the gut and lung (termed the “gut-lung axis”) has been previously proposed [11, 12]. The gut-lung axis is bidirectional and its interactions include two aspects: on the one hand, some respiratory diseases including asthma and influenza are strongly linked to a dysbiotic gut microbiota [13, 14]. On the other hand, a protective role of the gut microbiota against invasion of the lung by pathogenic microorganisms may be achieved by modulation of the local and systemic immunity of the host [7, 15, 16].
Although gut microbiota may impact the etiology of pulmonary diseases, there have been few explorations to-date focusing on the characterization of gut microbiota in TB patients, especially in pediatric groups which represent a clinically important population with increased susceptibility to TB . Thus, the present study was developed to explore the gut microbiota of children diagnosed with pulmonary tuberculosis (PTB).
The design of the present study was a case-controlled, two-part study. Fecal samples were collected from PTB pediatric patients and healthy controls on the day of their admission. One-month after anti-tuberculosis treatment, a second analysis was performed to investigate alterations of the gut microbiota.
Patients and information
A total of 18 patients with PTB were included in this study from the pediatric department of West China Second University Hospital, Sichuan University in China between June 2016 and June 2017. The diagnosis of PTB was identified according to the tuberculosis diagnosis and treatment guidelines for children in China . Briefly, the diagnostic criteria of PTB was made by a combination of the following: A. pathogenic or pathological evidence including a smear or culture test positive for Mycobacterium tuberculosis in sputum, gastric juice or bronchoalveolar lavage fluid. B. Typical clinical symptoms of PTB including cough and fever lasting for more than 2 weeks and chest X-ray presenting typical signs of PTB; C. A history of contact with active TB patients or D. a positive tuberculin test (reaction diameter of the skin > 5 mm). E. Effective anti-tuberculosis treatment or F. the exclusion of other lung diseases, such as pneumonia, lung cancer, pulmonary cyst and interstitial lung disease were also considered. PTB was confirmed in some patients through a satisfaction of both A and B criteria. Other patients who were satisfied by a combination of B criterion and any two of C, D, E, or F criteria were diagnosed as probable PTB.
The same number of healthy controls were selected from children who completed regular physical check-ups at the hospital during the study period. All of the controls were free of any respiratory diseases, without a history of contact with active TB patients and had received Bacillus Calmette-Guerin vaccine. Finally, all control subjects had tested negative for tuberculin prior to enrollment.
PTB patients and healthy controls were matched for age, weight and sex. None of the enrolled participants had received probiotics, prebiotics or antibiotics one month prior to hospital admission/evaluation. Basic demographic and clinical data were collected at the time of initial hospital evaluation for all subjects. In addition, a follow up was completed for PTB patients after one-month initiation of anti-tuberculosis therapy.
Informed consent was signed by the guardians of each participant prior to sample collection. The protocol of the present study was approved by the Ethical Committee of West China Second University Hospital, Sichuan University.
Sample collection and DNA extraction
Stool samples were obtained from healthy controls on the day of their hospital examination. For PTB patients, fecal samples were collected on the day of their admission and subsequently after a one-month anti-tuberculosis treatment. All samples were immediately frozen after collection and stored at − 80 °C. The genomic DNA was extracted from each sample using the E.Z.N.A.®Stool DNA Kit (D4015, Omega, Inc., USA).
Amplification and sequencing of 16S rRNA encoding gene
The bacterial 16S rRNA gene was amplified with forward primer 338F (5′-ACTCCTACGGGAGGCAGCAG-3′) and reverse primer 806R (5′-GGACTACHVGGGTWTCTAAT-3′). Sequencing was completed on Illumina Miseq platform (Illumina Inc., San Diego, CA, USA) and 300 bp paired-end reads were generated.
QIIME software, version 1.9.1  (http://qiime.org/1.9.1) was used to complete the quality filtering of the readers as well as their taxonomic classification. The quality filtered readers were clustered into operational taxonomic unit (OTU) at 97% similarity threshold and the taxonomic assignment was performed with Greengenes database (Release 13.8, http://greengenes.secondgenome.com). Alpha diversity including the richness and diversity of bacteria in samples was measured by Chao 1 index, ACE index, Shannon index and Simpson index. The Chao 1 index and ACE index which reflect the amount of the OTUs of the microbiota were used to evaluate the richness of the community of gut microbiota. The diversity of microbiota was measured by Shannon index and Simpson index, which calculates the number of species and their relative abundance in the gut. Based on the the biological evolution information of sequences from each sample, the weighted Unifrac metric principal coordinates analysis (PCoA) was used to estimate the Beta diversity of the gut microbiota, which reflects differences of the gut microbiota community between groups.
For the ratio of male to female, the Fisher’s exact test was completed. For age and weight, Chao 1 index, ACE index, Shannon index and Simpson index, comparison were performed by Mann-Whitney U test. The significant difference of Beta diversity was tested with Adonis non-parametric test. The relative abundance of gut microbiota between groups was compared by the T-test. P-values less than 0.05 were considered statistically significant. Fisher’s exact test and the Mann-Whitney U tests were performed by SPSS software, version 22.0 (IBM Corp, New York, NY, USA). The Adonis non-parametric test and T-tests were performed by R software, version 3.4.1 (https://www.r-project.org).
During the study period, a total of 36 participants including 18 PTB patients (two confirmed cases of PTB and 16 probable PTB patients) and 18 healthy controls were enrolled. The age, sex and weight of participants in the two groups were matched (Table 1).
Diversity of gut microbiota in PTB patients and healthy controls
A total of 36 fecal samples were obtained from PTB patients and healthy controls on the day of their admission/hospital evaluation. About 1,044,454 sequencing tags were processed from the 18 PTB patients’ fecal samples, corresponding to 592 ± 259 OTU per sample. Another 18 samples from control subjects yielded 1,126,447 sequencing tags, corresponding to 716 ± 235 OTU per sample.
In the present study, the difference of microbiotal richness between the PTB group and healthy participants demonstrated no statistically significant difference. Although the Shannon index indicated no significant difference in gut microbiotal diversity between the two groups, a decreased Simpson index reflected that the diversity of fecal microbiota in PTB patients was significant lower than in healthy children (0.80 ± 0.20 VS 0.93 ± 0.04, p<0.05) (Table 2).
Community of gut microbiota in PTB patients and healthy controls
A weighted UniFrac PCoA was performed to identify the difference in fecal microbiota composition between PTB patients and healthy controls. As shown in Fig. 1, there was no significant differential clustering observed between samples from the two groups (R2 = 0.08, P = 0.08). This demonstrated that the total community of gut microbiota in the two groups exhibited no significant differences.
Although the whole community structure of gut microbiota in the two groups showed no meaningful differences, the relative abundance of fecal microbiota in PTB patients was distinct from healthy controls at the family, genus and species levels. According to the sequencing analysis, the community of gut microbiota in the PTB and healthy control groups consisted of four bacterial phyla: Firmicutes, Bacteroidetes, Proteobacteria, and Actinobacteria. The relative abundance of Firmicutes was 54.54 and 65.08% in the PTB and healthy subjects, respectively. Bacteroidetes, Proteobacteria, and Actinobacteria accounted for 20.72, 21.12 and 2.66% in PTB patients and 18.69, 9.62 and 4.92% of the gut microbiota in healthy controls. While there were no differences in the relative abundance of these four phyla between groups, at the family level (Fig. 2), when compared with healthy controls, PTB patients presented a significant abundance of Enterococcaceae (6.11% VS 0.02%, P<0.01) and Prevotellaceae (8.60% VS 0.29%, P<0.01) over healthy controls. A notable reduction of Rikenellaceae (0.30% VS 1.29%, P<0.05), Bifidobacteriaceae (1.75% VS 4.45%, P<0.05), Lachnospiraceae (11.80% VS 21.05%, P<0.05) and Ruminococcaceae (15.63% VS 30.60%, P<0.05) was also detected in the PTB group.
At the genus level (Fig. 3), Enterococcus (9.61% VS 0.03%, P<0.01) and Prevotella (11.00% VS 0.44%, P<0.01) were found significant enriched in the PTB group when compared with healthy controls. On the other hand, the proportion of Faecalibacterium (9.23% VS 24.25%, P<0.01), Bacteroides (10.54% VS 21.90%, P<0.05), [Ruminococcus] (1.55% VS 4.16%, P<0.05) and Dorea (0.85% VS 2.52%, P<0.05) were significantly decreased in PTB patients versus controls.
At the species level (Fig. 4), results demonstrated that PTB patients tended to be abundant with agilis (1.57% VS 0, P<0.01), barnesiae (1.07% VS 0, P<0.01), stercorea (7.12% VS 0, P<0.01) and copri (14.68% VS 0.67%, P<0.01), while prausnitzii (20.61% VS 51.25%, P<0.01) was underrepresented compared with healthy subjects.
Changes in gut microbiota of PTB patients before and after anti-tuberculosis treatment
Among the 18 PTB patients enrolled in our study, only 6 PTB patients (two confirmed cases of PTB and four probable PTB patients) completed the follow-up and provided fecal samples after receiving one-month of anti-tuberculosis treatment. These 6 patients were treated with a four-drug anti-tuberculosis regimen including isoniazid, rifampicin, pyrazinamide and ethambutol. After one-month of treatment, the clinical symptoms (such as cough, night sweating or fever) of these patients improved. This indicated the effectiveness of the anti-tuberculosis intervention.
A comparison of the microbiota obtained from fecal samples of these 6 PTB patients before and after one-month anti-tuberculosis treatment was carried out. The Chao 1 index (387 ± 103 VS 751 ± 299, P<0.05) and ACE index (388 ± 103 VS 739 ± 304, P<0.05) which reflect the richness of gut microbiota demonstrated a significant decrease after one-month of treatment. On the other hand, no significant difference was found though Shannon and Simpson indices which present the diversity of the microbiota (Table 3).
In addition, the results of a weighted UniFrac PCoA demonstrated that the microbiota community as a whole (as represented from fecal samples of the 6 patients) could not be separated significantly (R2 = 0.08, P = 0.50) (Fig. 5). This indicated that the whole community of gut microbiota of PTB patients presented no obvious changes in gut microbiota after one month of treatment. Additionally, the relative abundance of the bacteria in these patients presented no significant changes after one-month of treatment.
The present study is the first to characterize the gut microbiota in pediatric PTB patients through the amplification of next-generation sequencing technology. The results of this study demonstrated that the patterns of gut microbiota in PTB patients were significantly different from healthy controls. The dysbiosis of gut microbiota in PTB patients was specifically characterized by an up-regulation of the pro-inflammatory bacteria Prevotella and the opportunistic pathogen Enterococcus. Further, a reduction of the beneficial bacteria Ruminococcaceae, Bifidobacteriaceae and prausnitzii was observed. This study also revealed that after one-month of effective anti-tuberculosis therapy, the richness of fecal microbiota is similarly decreased.
It is evident that the richness and diversity of gut microbiota plays a critical role in maintaining the health of the human body and that decreases in the richness and diversity of gut microbiota has been linked to diseases including influenza, asthma and HIV infection [13, 20, 21]. The results of this study indicated that the diversity of gut microbiota in PTB patients is generally decreased, which was demonstrated by the descending Simpson index value. This was not surprising given that some animal experiments have revealed similar findings [22, 23]. Winglee et. al. reported that mice infected with aerosolized Mycobacterium tuberculosis presented a rapid decrease in fecal microbiotal diversity . In addition, Namasivayam et. al. found that compared with healthy controls, the diversity of gut microbiota in a murine model of TB presented a slight but significant reduction 12 weeks after infection . In contrast, the results of Luo et. al. demonstrated that both new and recurrent TB patients maintained an increased richness of gut microbiota when compared with healthy subjects, and there were no significant differences in the Shannon and Simpson indices of fecal microbiotal diversity . The discrepancies between that study and the present study may be due to differences in the subjects recruited. In the study by Luo et. al., the participants were adults, some of which had previously received antibiotic treatment (prior to admission). However, the present study was focused specifically on the pediatric population. Additionally, none of the enrolled participants including the PTB group nor healthy controls had received antibiotics of any kind one month prior to hospital admission. We speculate that in either humans or mice, when infected with PTB, the local immunity of the lung is not singularly affected, rather the immune status of the intestine can be modulated due to crosstalk via the gut-lung axis. Thus, the altered immunity of the intestinal mucosa may contribute to a reduction of diversity in gut microbiota.
In the present study, although the total community of gut microbiota in patients with PTB and healthy controls presented no obvious differences, the relative abundance of some special bacteria at the family, genus and species levels were markedly different between the two groups. These results reflected a significant overrepresentation of Prevotella in PTB patients when compared with healthy controls. Previously, the increased abundance of Prevotella at mucosal sites has been reportedly involved with the development of many inflammatory diseases through the stimulation of the local and systemic immune response . Similarly, Mutlu et. al. and Ling et. al. have reported that the relative abundance of Prevotella was predominant in HIV patients’ intestines when compared with healthy controls [26, 27]. Interestingly, a prospective exploration performed by Luo et. al. reported that the levels of Prevotella are positively correlated with the number of peripheral CD 4+ cells in new tuberculosis patients. They hypothesized that Prevotella may regulate the immune status of the host and therefore may be related to the prognosis and outcome of TB patients . However, the exact mechanism of Prevotella’s role in the development of PTB in children remains unclear. Based on the findings of this study, we hypothesize that the increased abundance of Prevotella may activate pulmonary and systematic inflammatory reactions within the host to aggravate TB. This may be achieved through the regulation of the intestinal mucosa immunity and the subsequent increased production of pro-inflammatory cytokines, though this remains to be substantiated in a pediatric population.
Enterococcus is an opportunistic pathogen which usually inhabits the alimentary tract of humans and is associated with many infectious disease including urinary tract infections, surgical wound infections, and bacteraemia . In this study, PTB patients demonstrated a significant abundance of Enterococcaceae and Enterococcus in comparison with the healthy controls. The research performed by Krisna et. al. presented a similar result, in that Enterococcus was more predominant in the TB sputum samples than healthy subjects . Additionally, Sabino et. al. reported that the microbiota of patients with primary sclerosing cholangitis was characterized by an abundance of Enterococcus and that genus was associated with disease severity . On the one hand, the predominance of Enterococcus in PTB patients was hypothesized to be associated with an impaired epithelial barrier and intestinal permeability, resulting in bacterial translocation from the intestinal tract into systemic circulation where an immune inflammatory reaction could be triggered, thus contributing to the development of tuberculosis. On the other hand, it is worth highlighting that some pathogens are species-specific. Thus, accurate identification of specific pathogen species presents a future direction of study.
Interestingly, the structural imbalance of gut microbiota in patients with PTB is not only coupled with significant overrepresentation of pro-inflammatory bacteria and opportunistic pathogens, but also the significant depletion of beneficial bacteria. In the present study, F. ruminococcaceae and F. prausnitzii, belonging to the genus Faecalibacterium, were significant lower in the PTB group than in healthy controls. Previous studies have described that F. ruminococcaceae and F. prausnitzii may exert beneficial effects on human health though their metabolites, short-chain fatty acids (SCFA) [31, 32]. SCFAs are able to affect lipid, glucose, and cholesterol metabolism in many tissues, where a large proportion are used as a source of energy . SCFAs can also regulate the proliferation of colonic epithelial cells and enhance the permeability of the intestinal mucosa . SCFAs, especially butyrate, seem to exert a profound impact on the maintenance of immune homeostasis through broad anti-inflammatory effects, such as the regulation, migration, and adhesion of immune cells, the expression of inflammatory cytokines, and inhibition of histone deacetylases. Cellular proliferation, activation and apoptosis via a host of other signalling pathways have also been implicated in the scope of SCFA’s effects . Besides the significant depletion of butyrate-producing bacteria, another beneficial bacterium, Bifidobacteriaceae, was also found to be reduced in PTB group. As a common bacterium in the human gastrointestinal tract, Bifidobacterium (which belongs to the family Bifidobacteriaceae) exerts a lot of beneficial effects on the host [36, 37]. Some studies have reported that reductions of Bifidobacterium has been associated with many diseases, such as influenza, asthma and cystic fibrosis [13, 14, 38]. We hypothesize that the depletion of these beneficial bacteria promotes the development of the PTB through many pathways, including but not limited to reducing the immune response against the invasion of foreign microbes and inducing the dysbiosis of systematic inflammatory regulation.
The present study also elucidated a significant reduction of the richness of gut microbiota in PTB patients after one-month of anti-tuberculosis treatment. This finding is supported by research performed by Namasivayam et. al , which achieved similar results in mice after anti-tuberculosis treatment, wherein the richness of gut microbiota of the mice was similarly decreased. However, the relative abundance of gut microbiota between the patients upon admission and after one-month of treatment presented no significant difference in our study, which was in contrast to the results of Namasivayam et. al . Namasivayam et. al. reported that the relative abundance of the gut microbiota in TB mice before and after anti-tuberculosis treatment were significantly different. Several factors may account for this discrepancy. One obvious difference would be the species of the subject population. While Namasivayam et. al. utilized an animal model of TB, the present study evaluated human children with TB. Another possibility is that the anti-tuberculosis treatment regimen was different between the two studies. In our study, all patients received a 4-drug regimen including isoniazid, rifampicin, pyrazinamide and ethambutol. But in the study of Namasivayam et, all mice received a 3-drug regimen including isoniazid, rifampin, and pyrazinamide. We speculated that changes in the gut microbiota of PTB patients after treatment may be linked to the following factors. First, the direct effect of the anti-tuberculosis drugs on the gut microbiota. Second, the bidirectionality of gut-lung interactions could be such that when the immunity of the pulmonary condition is improved, the local immunity of intestine (as well as gut microbiota) may be proportionally improved through the influenced of the ‘gut-lung axis’ cross-talk.
There were several limitations in the present study. First, owing to the risk of radiation exposure to healthy children, this study did not obtain chest X-ray to exclude PTB in healthy controls. However, tuberculin test, medical history and a physical examination were used to eliminate the possibility of PTB in healthy controls. It has been reported that the sensitivity and specificity of the tuberculin test for screening TB is greater than 80% , thus it can be reliably used to detect TB in subject pools. The present study was limited by the cross-sectional research design, inhibiting the ability to detect causal relationships between the gut microbiota and the development of PTB. Another limitation is the relative small simple size. Because only 18 patients were enrolled in our study, so we didn’t analyze the characterization of gut microbiota in PTB patients in different age groups including infant, childhood and adolescent groups. What’s more, present study only explored changes in the gut microbiota of six PTB patients after one-month of anti-tuberculosis treatment and therefore may not comprehensively reflect the changes in the gut microbiota of pediatric PTB patients after anti-tuberculosis treatment. Finally, a large-scale, multi-center study would be required to validate this initial characterization of the gut microbiota of pediatric TB patients.
The present study provided the first detailed analysis of the characterization of gut microbiota in children with PTB, including changes of the intestinal microbiota after one-month anti-tuberculosis treatment. Our results demonstrated that the gut microbiota in PTB patients was significantly different from healthy controls as characterized by the increase of pro-inflammatory bacteria and opportunistic pathogens and the reduction of beneficial bacteria. In addition, longitudinal profiling revealed a significant decreased richness of gut microbiota in PTB patients who received one-month anti-tuberculosis treatment. It was hypothesized that the above mentioned changes of the gut microbiota could affect the development of PTB through the downstream regulation of the immune status of the host by way of the gut-lung axis.
Availability of data and materials
Operational Taxonomic Unit
Principal Coordinates Analysis
World Health Organization. Global Tuberculosis Report. Geneva: World Health Organization; 2018. https://www.who.int/tb/publications/global_report/en/.
Ley RE, Peterson DA, Gordon JI. Ecological and evolutionary forces shaping microbial diversity in the human intestine. Cell. 2006;124(4):837–48.
Tremaroli V, Backhed F. Functional interactions between the gut microbiota and host metabolism. Nature. 2012;489(7415):242–9.
Hooper LV, Littman DR, Macpherson AJ. Interactions between the microbiota and the immune system. Science. 2012;336(6086):1268–73.
Wu S, Jiang ZY, Sun YF, Yu B, Chen J, Dai CQ, Wu XL, Tang XL, Chen XY. Microbiota regulates the TLR7 signaling pathway against respiratory tract influenza a virus infection. Curr Microbiol. 2013;67(4):414–22.
Gauguet S, D'Ortona S, Ahnger-Pier K, Duan B, Surana NK, Lu R, Cywes-Bentley C, Gadjeva M, Shan Q, Priebe GP, et al. Intestinal microbiota of mice influences resistance to Staphylococcus aureus pneumonia. Infect Immun. 2015;83(10):4003–14.
Chen LW, Chen PH, Hsu CM. Commensal microflora contribute to host defense against Escherichia Coli pneumonia through toll-like receptors. Shock. 2011;36(1):67–75.
Gootenberg DB, Paer JM, Luevano JM, Kwon DS. HIV-associated changes in the enteric microbial community: potential role in loss of homeostasis and development of systemic inflammation. Curr Opin Infect Dis. 2017;30(1):31.
Heidrich B, Vital M, Plumeier I, Döscher N, Kahl S, Kirschner J, Ziegert S, Solbach P, Lenzen H, Potthoff A. Intestinal microbiota in patients with chronic hepatitis C with and without liver cirrhosis compared to healthy controls. Liver Int. 2017.
Montassier E, Al-Ghalith GA, Ward T, Corvec S, Gastinne T, Potel G, Moreau P, Cochetiere MFDL, Batard E, Dan K. Erratum to: pretreatment gut microbiome predicts chemotherapy-related bloodstream infection. Genome Medicine. 2016;8(1):1–1.
Marsland BJ, Trompette A, Gollwitzer ES: The Gut-Lung Axis in Respiratory Disease. Annals of the American Thoracic Society 2015, 12 Suppl 2:S150.
Yang H, Qu W, Yao F, Dong X, Huang Y, Wang J. Gut-lung axis: the microbial contributions and clinical implications. CRC Crit Rev Microbiol. 2016;43(1):1.
Qin N, Ni S, Shao L, Ye M, Luo R, Jiang B, Guo J, Chen Y, Hu X, Yang F. Influence of H7N9 virus infection and associated treatment on human gut microbiota. Sci Rep. 2015;5(2):14771.
Hevia A, Milani C, López P, Donado CD, Cuervo A, González S, Suárez A, Turroni F, Gueimonde M, Ventura M. Allergic patients with long-term asthma display low levels of Bifidobacterium adolescentis. PLoS One. 2016;11(2):e0147809.
Schuijt TJ, Lankelma JM, Scicluna BP, Melo FDSE, Roelofs JJTH, Boer JDD, Hoogendijk AJ, Beer RD, Vos AD, Belzer C. The gut microbiota plays a protective role in the host defence against pneumococcal pneumonia. Gut. 2016;65(4):575–83.
Mcaleer JP, Kolls JK. Contributions of the intestinal microbiome in lung immunity. European Journal of Immunology. 2017;48(Suppl 1).
Basu Roy R, Whittaker E, Seddon JA, Kampmann B. Tuberculosis susceptibility and protection in children. Lancet Infect Dis. 2019;19(3):e96–e108.
The Subspecialty Group of Respiratory Disease, The Society of Pediatrics, Chinese Medical Association. The clinical diagnosis criteria and therapeutic regimen of pulmonary tuberculosis in children. Chinese Journal of Pediatrics. 2006;44(4):249–51.
Caporaso JG, Kuczynski J, Stombaugh J, Bittinger K, Bushman FD, Costello EK, Fierer N, Pena AG, Goodrich JK, Gordon JI, et al. QIIME allows analysis of high-throughput community sequencing data. Nat Methods. 2010;7(5):335–6.
Abrahamsson TR, Jakobsson HE, Andersson AF, Björkstén B, Engstrand L, Jenmalm MC. Low gut microbiota diversity in early infancy precedes asthma at school age. Clinical & Experimental Allergy Journal of the British Society for Allergy & Clinical Immunology. 2014;44(6):842.
Nowak P, Troseid M, Avershina E, Barqasho B, Neogi U, Holm K, Hov JR, Noyan K, Vesterbacka J, Svärd J. Gut microbiota diversity predicts immune status in HIV-1 infection. Aids. 2015;29(18):2409–18.
Winglee K, Eloefadrosh E, Gupta S, Guo H, Fraser C, Bishai W. Aerosol mycobacterium tuberculosis infection causes rapid loss of diversity in gut microbiota. PLoS One. 2014;9(5):e97048.
Namasivayam S, Maiga M, Yuan W, Thovarai V, Costa DL, Mittereder LR, Wipperman MF, Glickman MS, Dzutsev A, Trinchieri G. Longitudinal profiling reveals a persistent intestinal dysbiosis triggered by conventional anti-tuberculosis therapy. Microbiome. 2017;5(1):71.
Luo M, Liu Y, Wu P, Luo DX, Sun Q, Zheng H, Hu R, Pandol SJ, Li QF, Han YP. Alternation of gut microbiota in patients with pulmonary tuberculosis. Front Physiol. 2017;8.
Larsen JM. The Immune Response to Prevotella Bacteria in Chronic Inflammatory Disease. Immunology. 2017;151:(4).
Mutlu EA, Keshavarzian A, Losurdo J, Swanson G, Siewe B, Forsyth C, French A, Demarais P, Sun Y, Koenig L. A compositional look at the human gastrointestinal microbiome and immune activation parameters in HIV infected subjects. PLoS Pathog. 2014;10(2):e1003829.
Ling Z, Jin C, Xie T, Cheng Y, Li L, Wu N. Alterations in the fecal microbiota of patients with HIV-1 infection: an observational study in a Chinese population. Sci Rep. 2016;6.
Fisher K, Phillips C. The ecology, epidemiology and virulence of Enterococcus. Microbiology. 2009;155(6):1749–57.
Krishna P, Jain A, Bisen PS. Microbiome diversity in the sputum of patients with pulmonary tuberculosis. Eur J Clin Microbiol Infect Dis. 2016;35(7):1205–10.
Sabino J, Vieirasilva S, Machiels K, Joossens M, Falony G, Ballet V, Ferrante M, Assche GV, Merwe SVD, Vermeire S. Primary sclerosing cholangitis is characterised by intestinal dysbiosis independent from IBD. Gut. 2016;65(10):1681–9.
Lopez-Siles M, Duncan SH, Garcia-Gil LJ, Martinez-Medina M. Faecalibacterium prausnitzii: from microbiology to diagnostics and prognostics. Isme J. 2017;11(4):841.
Qu WT, Yuan XJ, Zhao JS, Zhang YX, Hu J, Wang JW, Li JX. Dietary advanced glycation end products modify gut microbial composition and partially increase colon permeability in rats. Mol Nutr Food Res. 2017;61:(10).
Besten GD, Eunen KV, Groen AK, Venema K, Reijngoud DJ, Bakker BM. The role of short-chain fatty acids in the interplay between diet, gut microbiota, and host energy metabolism. J Lipid Res. 2013;54(9):2325–40.
Abruzzo A, Damiano G, Altomare R, Palumbo VD, Tomasello G, Buscemi S, Lo Monte G, Maione C, Buscemi G, Lo Monte AI. The influence of some dietary components on intestinal microbiota. Prog Nutr. 2016;18(3):205–12.
Samuelson DR, Welsh DA, Shellito JE. Regulation of lung immunity and host defense by the intestinal microbiota. Front Microbiol. 2015;6.
Giudice MMD, Indolfi C, Capasso M, Maiello N, Decimo F, Ciprandi G. Bifidobacterium mixture ( B longum BB536 , B infantis M-63 , B breve M-16V) treatment in children with seasonal allergic rhinitis and intermittent asthma. Ital J Pediatr. 2017;43(1):25.
Huda MN, Lewis Z, Kalanetra KM, Rashid M, Ahmad SM, Raqib R, Qadri F, Underwood MA, Mills DA, Stephensen CB. Stool microbiota and vaccine responses of infants. Pediatrics. 2014;134(2):e362.
Hoen AG, Li J, Moulton LA, O'Toole GA, Housman ML, Koestler DC, Guill MF, Moore JH, Hibberd PL, Morrison HG, et al. Associations between gut microbial colonization in early life and respiratory outcomes in cystic fibrosis. J Pediatr-Us. 2015;167(1):138–U520.
Chiappini E, Accetta G, Bonsignori F, Boddi V, Galli L, Biggeri A, De Martino M. Interferon-gamma release assays for the diagnosis of mycobacterium tuberculosis infection in children: a systematic review and meta-analysis. Int J Immunopathol Pharmacol. 2012;25(3):557–64.
This project was supported by a grant from Pediatric Clinical Research Center Foundation of Sichuan Province, China (No.2017-46-4), National Science and Technology Major Project of China (No.2018ZX10103-001) the Fundamental Research Funds for Central Universities (No.2012017yjsy196) and Research development project of Sichuan Provincial Science and Technology Department (No.2018SZ0130). The views expressed are those of the authors and not necessarily those of funders. The funders were not directly involved in the collection, analysis, and interpretation of data or in writing the manuscript. Prior to the grant being awarded, the funding body provided feedback on the study design.
Ethics approval and consent to participate
This study protocol was approved by the Ethical Committee of West China Second University Hospital, Sichuan University. Written informed consent was obtained from guardians of participants prior to study enrollment.
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Li, W., Zhu, Y., Liao, Q. et al. Characterization of gut microbiota in children with pulmonary tuberculosis. BMC Pediatr 19, 445 (2019) doi:10.1186/s12887-019-1782-2
- Pulmonary tuberculosis
- Gut microbiota