Background
Idiopathic pulmonary fibrosis (IPF) is a well-known life-threatening disease of the lung with median survival of only 3 to 5 years [
1‐
3] Patients with IPF exhibit restrictive ventilatory impairment caused by progressive lung fibrosis, and a decline in forced vital capacity (FVC) is strongly associated with mortality [
4]. Among the various forms of idiopathic interstitial pneumonias, IPF has attracted the most attention because of its poor prognosis and the limited number of therapeutic agents. In addition, acute exacerbation (AE) is the most critical life-threatening event in IPF, especially in Asians, including Japanese [
5‐
7]. Many studies have identified key factors in the development of IPF, and some drugs against fibrosis have been developed, but the direct cause remains unknown [
8,
9].
Until recently, the lung was considered to be a sterile compartment because culture-based techniques are limited in their ability to identify all bacteria that may be present. However, new techniques have been developed that have identified bacterial communities both in healthy humans and those with pulmonary diseases [
10‐
12]. This new characterization of the lung microbiome is likely to provide important pathogenic insights into chronic lung diseases, including cystic fibrosis, chronic obstructive pulmonary disease, and asthma. Recent papers have reported the possible role of microbiome composition in IPF [
13,
14]. Increased bacterial burden and presence of specific bacteria have been associated with disease progression. However, the roles of the microbiome in respiratory functions and as a clinical marker in IPF remain unknown.
In the current study, we performed a retrospective comprehensive analysis of lower respiratory tract bacterial microbiomes in Japanese individuals with IPF. To investigate the clear relationship between microbiome and pathological conditions, we also analyzed microbiome from a mouse model with bleomycin-induced lung fibrosis.
Methods
Patient selection
The subjects who were retrospectively included in this analysis were IPF patients who had visited Sapporo Medical University Hospital. The study was approved by the hospital’s ethics board (approval number, 292–35). Diagnosis of IPF was performed according to the ATS/ERS/JRS/ALAT statement 2011 [
2]. In this study, drug history (discussed in the Results section) is not included in the exclusion criteria. The patient characteristics, results of pulmonary function tests, arterial blood gas analysis, and 6-min walk distance (6MWD) test, as well as general blood test and some biomarkers for IPF in serum at enrollment were investigated. The pulmonary function test (PFT), including determination of the FVC and diffusing capacity of lung carbon monoxide (DLco), was performed by using a CHESTAC-55 V system (CHEST M.I., Inc., Tokyo, Japan). The 6MWD test was performed in accordance with ATS guidelines. The GAP (gender, age, and physiological variables) point score was calculated by determining the subject’s gender, age in years, percent predicted FVC (%FVC), and percent predicted DL
CO (%DL
CO), as described previously [
15]. PFT results at 12 ± 1 months from baseline and the change in FVC were evaluated. Deterioration was defined as a ≥ 10% relative decline in FVC from baseline and severe respiratory status in which PFTs were unable to be performed [
16]. AE was defined according to the Japanese criteria [
16]. These criteria are consistent with the criteria proposed by Collard and coworkers in 2007 [
17].
Sample collection
Bronchoscopy was performed in patients with clinically diagnosed IPF. The bronchoscope was inserted via the mouth and through the vocal cords. After carefully observing the lumen of the bronchus, the bronchoscope was wedged into a targeted lobe using an intubation tube. Bronchoalveolar lavage (BAL) was performed in either the middle lobe or the lingula, irrespective of the imaging abnormality on high-resolution computed tomography (HRCT). BAL was performed with 3 instillations of 50 ml of warmed normal saline for a total of 150 ml with all possible returns collected and pooled. Samples for microbiome analysis were added to a falcon tube and stored at − 80 °C until the time of DNA extraction.
Murine model
C57BL/6 J mice were purchased from Sankyo Labo Service Corporation Inc. (Tokyo, Japan). We ensured that they were equivalent in genetic quality and had stable phenotypes. Although non-littermate mice might have different microbial flora, we did not use littermates in this study to avoid a bias arising from the residing genetic inheritance. In addition to similar housing conditions provided to all animals, including food, water and co-house, the random selection ensured elimination of the bias as much as possible. The mice were maintained under specific pathogen-free conditions and used when they were 8 weeks of age. Thereafter, we divided the mice into two groups: bleomycin and normal saline groups. Bleomycin hydrochloride (Nippon kayaku Co., Tokyo, Japan) was dissolved in normal saline and continuously administrated via micro-osmotic pump (Alzet 1007D; DURECT Corporation, CA). Mice were anesthetized by inhalation of isoflurane, followed by Alzet pump insertion into the mid-back subcutaneous region. Alzet pumps contained either 100 μl of bleomycin hydrochloride (100 mg/kg) or normal saline as a control, and were designed to deliver their contents at 0.5 μL/h over 7 days. At 28 days after Alzet pump insertion, mice were sacrificed with an intraperitoneal injection of pentothal, and blood was immediately collected for obtaining serum samples. Lungs were lavaged with 1 ml of normal saline. For histological examination, lungs were fixed with 10% formalin phosphate and embedded in paraffin. Lung sections were stained with hematoxylin-eosin and Masson trichrome reagent, and examined with a microscope. Total and differential cells in the bronchoalveolar lavage fluid (BALF) were counted using the XT-1800iV (Sysmex, Japan). All experiments using mice were conducted according to the regulations of the Sapporo Medical University Animal Care and Use Committee.
Standard lysis protocol and DNA isolation
A 1.5 ml aliquot of the BALF sample was centrifuged at 10,000 g for 10 min, and the supernatant was discarded. The pellets were suspended in 180 μl of lysis solution (20 mg/ml egg chicken lysozyme (Sigma-Aldrich), 20 mM Tris-HCl (pH 7.4), 2 mM EDTA, 1.2% Triton X), then incubated for 30 min at 37 °C with occasional vortex mixing. Samples were digested by Proteinase K (final concentration, 1 mg/mL) and incubated for 30 min at 65 °C. DNA purification was performed using a DNeasy Blood and Tissue Kit (Qiagen) per manufacturer instructions.
Real-time polymerase chain reaction (PCR)
The number of tuf gene expression was analyzed to estimate the number of bacteria in the BALF. Real-time PCR was performed on these samples by using a bacterial quantitative PCR kit (Takara, Japan) and a 7900 HT Fast Real-Time PCR System (Applied Biosystems). The cycling conditions were 1 cycle at 95 °C for 30 s, 35 cycles at 95 °C for 5 s, and 60 °C for 30 s.
DNA sequencing and sequence analyses
An Ion 16S Metagenomics Kit, which is designed for rapid analyses of bacterial samples using Ion Torrent sequencing technology, was used for the sequencing analysis of the bacterial 16S rDNA gene. This kit includes 2 primer sets that selectively amplify the corresponding hypervariable regions of the 16S region in bacteria: V2–4-8 and V3–6, 7–9. The primary PCR cycling conditions were 95 °C for 10 min, followed by 27 cycles of standard PCR (95 °C for 30 s, 50 °C for 30 s, and 72 °C for 45 s), and finished with 72 °C for 7 min. Then, sequence analyses were performed by using the Ion Torrent sequencing platform (Ion Torrent PGM™). Raw sequencing data were processed by using the mother software package, as described in the Ion Torrent standard operating procedure. After sequencing, raw signal data were analyzed using Torrent Suite version 5.0. The pipeline included signaling processing, base calling, low quality read removal, and adapter trimming. Sequencing data in BAM format were further processed using Ion Reporter software v5.2. These files, with the taxonomic information for the operational taxonomic units (OTUs), were imported and further analyzed using Explicet v2.10 software (Robertson,
http://www.explicet.org). We restricted the principal components and regression analyses to OTUs that were present at > 1.0% of a given sample’s population and taxonomically identifiable.
Statistical analysis
Continuous variables are shown as the median with interquartile ranges. For comparisons between two groups, continuous variables were examined by using the Mann–Whitney U test on GraphPad Prism v7 software (GraphPad, Inc., San Diego, CA, USA). Alpha-diversity metrics were used to characterize the bacterial diversity within each sample. Alpha-diversity metrics, including the Shannon diversity index and Simpson diversity (1-D) index, were computed by using Explicet v2.10 software. Spearman’s correlation analysis and JMP 13.0 (SAS Institute, Cary, NC, USA) were used to evaluate the coefficients of determination (ρ), residuals, and significance (p) to identify associations between the microbiome and parameters. Principal coordinates analysis (PCoA) of the Bray-Curtis dissimilarity between samples was generated using Past v3.13 software (Hammer O. Past 3.× 2017. Available from:
http://folk.uio.no/ohammer/past/).
Discussion
In this study, we showed that BALF from initially diagnosed IPF contained microbiota and that the loss of diversity of the lung microbiome correlated with the progression of IPF. Regarding the change in lung microbiome diversity, we found that increases in the Firmicutes and Bacteroidetes (Streptococcaceae, Veillonellaceae, and Prevotellaceae families) and a decrease in the phylum Proteobacteria were involved in the reduction of diversity. Moreover, the loss of diversity correlated with IPF indicators, including low FVC, decreased 6MWD, and high serum SP-D and LDH. Unfortunately, there were no healthy controls in this study, but loss of diversity in IPF compare to healthy control was reported in a previous paper [
13]. Also, Molyneaux PL et al. suggested that the bacterial communities of the lower airways act as persistent stimuli for repetitive alveolar injury [
19]. Taken together, loss of diversity might have some impact on the pathogenesis of IPF. There is also a possibility that diversity is related to the mortality rate and FVC decline 1 year after diagnosis, which suggests that lung microbiome diversity may be a prognostic indicator, which is the most crucial finding in this study. Furthermore, racial differences and environmental factors were also considered to be involved in the microbiome and obtaining similar results in Asia compared with Western countries was significant. Additionally, we found that an increase in Streptococcaceae correlated with a reduction in 6MWD (Additional file
1: Figure S4). These results possibly suggest that pulmonary microbiomes and lung fibrosis are closely related and are involved in the pathogenesis of IPF. In contrast, whether microbial changes are a cause or merely a consequence of disease progression remains unclear. Hence, further extensive interventional studies, including antibiotics treatment or vaccines to alter the lung microbiome, are needed to elucidate this phenomenon.
Meanwhile, the examinations of microbiomes using clinical samples are quite complicated, because there are many confounding factors such as smoking history, drugs, etc. So, we decided to verify our results of the clinical samples using the bleomycin-treated mice with a uniform background, which is widely used in IPF studies. Since the living environment of the mice is very different from humans, their detailed bacterial flora was expected to be different [
20]. However, we found that the relative changes in the bacterial communities accompanying fibrosis in the mice were quite similar to that in IPF patients (Fig.
4c). The increase in the relative abundance of Firmicutes and the decrease in that of Proteobacteria, and its accompanying reduction in diversity were observed in BALF from bleomycin-treated mice (Fig.
4b and c). These results partly supported the analysis in the human specimens. Furthermore, PCoA analysis in the mice revealed that the microbial communities under bleomycin-induced fibrosis were different from normal flora (Fig.
4d), which is not detected in human subjects (data not shown). This may be due to the fact that there are many confounding factors among the patients as mentioned above. It is still difficult to identify causative bacteria implicated in the progression of IPF. Nonetheless, our data suggest that fibrotic changes in the lungs are related to the alternations of specific bacteria or the decline of diversity.
The Hokkaido study revealed that the most common (40%) cause of death was an AE, which resulted in rapid disease progression and a mortality rate of 80% [
7]. As the causes of AE, including whether or not bacteria are involved, have not been determined, we believe that it is essential to prove the effect of microbiomes on AEs. Based on our examination at diagnosis, the occurrence of an AE in the future was not related to an increased total bacterial burden and the loss of diversity (Additional File
1: Figure S1). However, because this study highlighted the possibility of the effect of microbiomes on AEs [
21‐
23], we intend to elucidate these findings in our next larger prospective study. Furthermore, we believe that it is imperative to investigate the causative bacteria on fibrosis in a murine model in the future.
An imbalance in the host–microbial relationship is thought to contribute to inflammation and immunity in the IPF lung [
24]. It is well known that the pulmonary collectins, surfactant proteins A and D, have an important role in the alveolar spaces and are useful biomarkers in IPF [
25]. In this study, serum SP-D was strongly associated with microbiome characteristics, including diversity, the relative abundance of Firmicutes, Proteobacteria, and Veillonellaceae. However, serum SP-A correlated poorly with lung microbiomes in contrast to BALF SP-A (Additional file
1: Figure S3). Our previous study reported that serum levels of SP-D could reflect pathological changes of IPF lungs more decisively than those of SP-A [
26]. Because the correlation between BALF SP-A and Veillonellaceae is positive, SP-A production from alveolar type II cells is thought to be increased by inflammatory stimulation accompanying the increase in bacteria. Taken together, it is possible that serum SP-A, in contrast to BALF SP-A, did not correlate with the microbiomes because SP-A remains bound to surfactant lipids in the alveolar space. On the other hand, SP-D reflects changes in the microbiome, such as diversity, because SP-D easily leaks into the bloodstream. As described above, because pulmonary collectins have an important role in pulmonary environments, we plan to clarify the association between the lung microbiome and the collectins in a future study.
This study had some limitations. All participants in this study satisfied the diagnostic criteria of IPF; however, because surgical lung biopsy was not performed at the time of diagnosis, the possibility of including other similar fibrotic diseases cannot be ruled out. In addition, the number of participants (
n = 34) was small to evaluate the association between the microbiome and IPF pathogenesis, because there are many confounding factors among IPF participants. For this reason, the examination using mice was carried out to prove the results of the human specimens by avoiding the influence of the confounders, although the etiology is somewhat different from IPF. Mice study cannot prove or disprove human studies because of their distinctly different nature and environment; it can provide credence to human studies, but cannot prove it. Furthermore, the inclusion of healthy controls would have been ideal, but there were no healthy controls in this study. Future studies using a larger number of subjects with appropriate controls are needed to further investigate the role of the microbiome in IPF. Additionally, the presence or absence of emphysematous change and the degree or location of fibrosis was not considered in this study. It is possible that the microbiomes may change depending on the grade of fibrosis and honeycomb change. Previous studies have shown that patients with some respiratory past history have different microbiomes than those of healthy volunteers [
27]. Furthermore, antibiotics, antacids, inhaled corticosteroids and nutritious food, which can cause microbial changes, should be considered. Because the possible effect of antacids or inhaled corticosteroids on the microbiome cannot be denied in this study. Technically, BAL was carefully performed to prevent contamination from the upper respiratory tract because sampling of the airways by bronchoscopy depends on inserting the bronchoscope into the mouth. It is still possible that contamination from the upper respiratory tract was present; however, a previous report indicated that contamination with oral microbiota from use of typical bronchoscopy techniques was limited [
28].