- Open Access
Insights into the respiratory tract microbiota of patients with cystic fibrosis during early Pseudomonas aeruginosa colonization
© Keravec et al. 2015
- Received: 15 April 2015
- Accepted: 3 August 2015
- Published: 9 August 2015
Pseudomonas aeruginosa plays a major role in cystic fibrosis (CF) progression. Therefore, it is important to understand the initial steps of P. aeruginosa infection. The structure and dynamics of CF respiratory tract microbial communities during the early stages of P. aeruginosa colonization were characterized by pyrosequencing and cloning-sequencing. The respiratory microbiota showed high diversity, related to the young age of the CF cohort (mean age 10 years). Wide inter- and intra-individual variations were revealed. A common core microbiota of 5 phyla and 13 predominant genera was found, the majority of which were obligate anaerobes. A few genera were significantly more prevalent in patients never infected by P. aeruginosa. Persistence of an anaerobic core microbiota regardless of P. aeruginosa status suggests a major role of certain anaerobes in the pathophysiology of lung infections in CF. Some genera may be potential biomarkers of pulmonary infection state.
- Cystic fibrosis
- Respiratory tract microbiota
- Pseudomonas aeruginosa
- Early colonization
- Respiratory viruses
Chronic lung infections are the primary cause of morbidity and mortality in cystic fibrosis (CF) (Nixon et al. 2001). The respiratory tract of CF patients is colonized and infected by numerous bacteria from an early age. Among cultivable pathogens, which include Pseudomonas aeruginosa, Staphylococcus aureus, Haemophilus influenzae, Burkholderia cepacia complex and Achromobacter xylosoxidans, P. aeruginosa is the most prevalent pathogen in CF. In children with CF, Kosorok et al. (2001) demonstrated a longitudinal correlation between P. aeruginosa acquisition and gradual deterioration of pulmonary function. Therefore, early detection of P. aeruginosa appears crucial for maximizing the chances of efficiently controlling this pathogen, notably by early institution of anti-Pseudomonas antibiotherapy (Valerius et al. 1991).
Better understanding of the initial steps of P. aeruginosa infection would also help in preventing early colonization in CF airways. According to Klepac-Ceraj et al. (2010), the community composition of the CF pulmonary microbiota is a better indicator of disease progression than the presence of P. aeruginosa alone. The endogenous respiratory microbiota may modulate pathogenesis in a polymicrobial context through microbe–microbe and polymicrobe–host interactions (Sibley and Surette 2011). Several studies reported important differences in the structure of the respiratory microbiota between healthy subjects and patients with chronic lung diseases (Huang et al. 2010). The lung infections of CF patients are also considered as polymicrobial (Sibley and Surette 2011; Sibley et al. 2006). Recently, van der Gast et al. (2011) identified a core group dominated by P. aeruginosa and a satellite group composed of multiple microbial species, including species not routinely identified by culture and not recognized as CF pathogens. The inability of conventional infection models to detect a pathogenic response to certain microorganisms known as commensals should not mean that their potential to contribute to polymicrobial infection can be disregarded (Sibley et al. 2008). The CF lung infection model has thus moved from a classical to an ecological paradigm.
In the light of these new findings, the present study investigated whether early P. aeruginosa colonization in CF patients was accompanied by significant changes in respiratory microbiota in terms of community structure and relative abundance, with the challenge of identifying potential biomarkers or predictive factors of P. aeruginosa implantation.
Population and sampling
Five CF patients with an age range of 5–19 years were followed up during a median of 22 months [16–39 months]. Sputum samples were processed using the standard operating procedure (SOP) of the French guidelines (Anonyme 2010). Twenty spontaneous sputum samples (4 per patient) were collected and homogenized with an equal volume of dithiothreitol (Digest-EUR® Eurobio, Courtabœuf, France) for 30 min at 37 °C. Clinical, therapeutic and biological data were compiled such as CFTR mutation, clinical state, antibiotic treatment and P. aeruginosa status. Sputum sample quality was verified by cytological examination of fresh smears and classified according to the number of epithelial cells and leukocytes. Sputum samples were classified in three quality classes: poor quality when the number of epithelial cells (cells/field) was ≥25 and the number of leukocytes (cells/field) was ≤10; appropriate quality when the number of epithelial cells was ≤25 and the number of leukocytes (cells/field) was ≥10. The other combinations between epithelial cells and leukocytes were considered of moderate quality. All samples were stored at −80 °C prior to DNA extraction. According to the Lee’s definition of P. aeruginosa infection status (Lee et al. 2003), three patients were categorized as ‘free’ (no culture of P. aeruginosa for at least the previous year), and two patients as ‘never’ (P. aeruginosa had never been detected from sputum or cough swabs culture). All patients became P. aeruginosa positive in culture during the follow-up.
DNA extraction and quantitative PCR
Presence of P. aeruginosa was also investigated by quantitative PCR (qPCR) as previously described (Le Gall et al. 2013) (Additional file 1: Table S1). Bacterial DNA was extracted using the QIAamp DNA Mini Kit (QIAGEN, Courtabœuf, France) according to the manufacturer’s instructions; a sonication step of 5 min was applied prior to proteinase K digestion, which was performed for 3 h at 56 °C. The total bacterial load was established by qPCR with universal primers targeting the 16S rRNA gene as previously described (Zemanick et al. 2013).
Barcoded pyrosequencing and bioinformatic analyses
The V3 and V4 hypervariable regions of the 16S rRNA gene were amplified using primers 347F (5′-GGAGGCAGCAGTRRGGAAT-3′) and 803R (5′-CTACCRGGGTATCTAATCC-3′) (Nossa et al. 2010). The 50 µl PCR mixture contained 10 pmol of each primer, 1× of polymerase buffer, 0.4 mM of each dNTP, 1.25 U of GoTaq® Flexi DNA polymerase (Promega, France), 3 mM of MgCl2 and 50 ng of DNA template. Reactions were heated at 94 °C for 5 min followed by 30 cycles of 94 °C for 1 min, 58 °C for 40 s and 72 °C for 40 s, and with a final extension step of 5 min at 72 °C. Two independent PCR amplifications were carried out for each sputum sample and the resulting PCR products were pooled. Prior to pyrosequencing, the size and quantity of pooled amplicon libraries were determined by an Agilent 2100 Bioanalyzer (Agilent Technologies, Germany) and PCR products were sequenced on a Genome Sequencer FLX™ Titanium (454 Life Sciences Corp., Bradford, CT, USA) by GATC Biotech (Konstanz, Germany). Quality control and sequence processing were performed using the UPARSE pipeline (Edgar 2013).
Data set was processed and analyzed using the UPARSE pipeline with scripts available on drive5 (http://drive5.com). The following quality filtering parameters were applied: truncation length of 250 bp, truncation to the first nucleotide with a quality score under 20, maximal expected error of 0.25. After removal of singletons, sequences were clustered into OTUs based on a sequence similarity level of 0.97 using the UPARSE-OTU algorithm followed by filtration of chimeras against the ‘Gold’ database using UCHIME (Edgar 2013; Edgar et al. 2011).
Sequence data and the OTU table obtained using the UPARSE pipeline were then processed and analyzed using Quantitative Insights Into Microbial Ecology (QIIME) (Caporaso et al. 2010). The representative sequence of each OTU was classified in QIIME against the Greengenes database (http://greengenes.lbl.gov/, version released on May 2013) using the Ribosomal Database Project (RDP) classifier with a confidence threshold of 80 %. OTUs of interest were also further classified to the species level using the RDP SeqMatch tool. Prior to alpha and beta diversity analyses, the OTU table was rarefied to the smallest number of reads obtained in a sample. Alpha diversity was determined using the Shannon index, Chao-1 estimator and equitability (evenness) index. Beta diversity was assessed using the Adonis test and the Bray–Curtis distance and visualized by principal coordinate analysis (PCoA). Diversity was also evaluated using the Simpson’s diversity index (SDI) transformed with the arcsine square root. A non-parametric (Kruskal–Wallis test) statistical test was applied in QIIME to test whether genera abundance was significantly associated with their associated metadata. A hierarchical ascendant classification (HAC) by Euclidean distance and an abundance heatmap were also obtained using XLstat software package (http://www.xlstat.com). The core microbiota was defined as OTUs present in at least 50 % of samples at a minimum relative abundance of 0.1 % of the total bacterial community. Sequences of the selected OTUs were aligned to the Greengenes core-set-aligned using PyNast with default parameters. The concordance between detection of P. aeruginosa using 454 pyrosequencing and culture based-method was assessed. The alignment was then filtered to remove gaps and hypervariable regions using a lane mask and a tree was generated using FastTree (Price et al. 2009). A circular phylogenetic tree was then constructed using the Interactive Tree Of Life (iTOL) (Letunic and Bork 2007). The sequence data were deposited at the NCBI Short Read Archive (BioProject no. PRJNA258440).
Respiratory viruses screening
One sample (A1) was not included in this screening as having not enough DNA. From the remaining 19 samples, viral RNA and DNA were extracted using the automated NUCLISENS® easyMAG™ (bioMérieux, Marcy l’Etoile, France) after a treatment with 25 µl of proteinase K (10 mg/ml) during 2 h at 56 °C. The nucleic acids were eluted in 50 µl and conserved at −80 °C. The RespiFinder® SMART 22 FAST (PathoFinder, Maastricht, The Netherlands) was used according to the manufacturer’s instructions and then, qPCR was performed in a GeneAmp® PCR System 9700 (Applied Biosystems, Courtabœuf, France). The kit simultaneously detects 18 respiratory viruses (Influenza A, Influenza B, Influenza A H1N1v, Respiratory Syncytial Virus A, Respiratory Syncytial Virus B, Parainfluenza 1, Parainfluenza 2, Parainfluenza 3, Parainfluenza 4, Coronavirus OC43, Coronavirus 229E, Coronavirus NL63, Coronavirus HKU1, Rhinovirus/enterovirus, Adenovirus, human Metapneumovirus, Bocavirus Type 1) and four bacteria (Chlamydophila pneumoniae, Mycoplasma pneumoniae, Legionella pneumophila, Bordetella pertussis).
For the cloning and sequencing analysis, the near-full-length 16S rRNA gene was amplified using universal primers pA (5′-AGAGTTTGATCCTGGCTCAG-3′) and pH (5′-AAGGAGGTGATCCAGCCGCA-3′) (Turner et al. 1999). PCR amplification was performed in a total volume of 25 µl containing 2.5 pmol of each primer, 1× polymerase buffer, 0.2 mM of each dNTP, 0.625 U GoTaq polymerase and 2 mM MgCl2 and 50 mg DNA template. Reaction was heated at 94 °C for 5 min followed by 30 cycles of 94 °C for 60 s, 57 °C for 40 s and 72 °C for 60 s followed by a final extension at 72 °C for 10 min. After PCR, the amplification products approx. 1,500 bp in size were checked on 1 % agarose gel (Promega, France). The PCR products obtained were ligated in pCR4-TOPO vector (Invitrogen, Carlsbad, CA, USA). The recombinant plasmids were used to transform Escherichia coli strain TOP 10 One Shot chemically competent cells according to the manufacturer’s instructions. Restriction fragment length polymorphism (RFLP) was used for dereplication of clone libraries as described previously (Mounier et al. 2009) using HaeIII restriction enzyme. Clone representatives of each clone library showing distinct restriction profiles were then sequenced at the Biogenouest sequencing platform in the Station Biologique de Roscoff center (http://www.sb-roscoff.fr). The sequences were assembled into contigs using DNA Baser software (http://www.dnabaser.com) and compared with the NCBI database (http://www.ncbi.nlm.nih.gov/BLAST), Greengenes (http://greengenes.lbl.gov/, version released on May 2013) and RDP SeqMatch tool program to obtain S_ab values with database sequences. Clone sequences and sequences with the highest S_ab score retrieved from GenBank were then aligned using ClustalW. The coverage percentage of clone library coverage using the Good’s formula and alpha diversity were calculated.
Diversity of the respiratory microbiota
Out of 625,263 reads generated using pyrosequencing, 287,306 high-quality reads were retained, with a mean 14,365 reads per sample (7,954–29,458) (Additional file 2: Table S2). After normalization to the sample with the lowest number of reads (7,954), 159,060 reads (mean length approx. 420 bp) were analyzed; 124 OTUs were identified (32–85 per sample). Three samples (C2, D3 and D4) were not included in clone libraries because small numbers of clones were obtained for these samples. From the remaining 17 samples, 1,327 clones were analyzed, representing 35 OTUs. According to Good’s formula, the coverage of clone libraries ranged from 77 to 99 %, indicating that the most abundant taxa were represented in the libraries.
Bacterial diversity was high, with a mean Shannon index of 3.58 (1.20–4.50) which was in accordance with others studies (Boutin et al. 2015; Bernarde et al. 2015) (Additional file 2: Table S2). The majority of bacteria were represented (Good’s coverage of 0.999). Moreover, the Chao1 richness index was only slightly higher than the number of observed OTUs in each sample, indicating that true bacterial richness was not underestimated. An Adonis test was performed and no significant impact of the cytological score was observed (p > 0.1, R2 = 0.19). The Bray Curtis dissimilarity was evaluated between successive samples (Additional file 3: Table S3) and showed some degree of fluctuations. The SDI values were calculated to assess bacterial diversity and showed increasing trends across time (y = 0.0496x + 0.8775, R2 = 0.7314). The high diversity found in the present study can be explained by the young age of these patients (mean age 10 years) because microbial diversity is maximal in this age range (Cox et al. 2010). However, such age correlation is still an open question and further studies are needed to confirm these findings.
Core CF pulmonary microbiota in children is characterized by ‘oral’ anaerobic bacteria
The 13 predominant genera identified in the present study are commonly found in CF respiratory tract microbiota (Willner et al. 2012; Venkataraman et al. 2015; Tunney et al. 2008; Carmody et al. 2013). Nine of them have been described to be the most abundant genera in healthy lungs (Wat et al. 2008). In agreement with previous studies, there was a large abundance of obligate anaerobes such as Veillonella and Prevotella (Tunney et al. 2008; Cheung et al. 2013), and facultative anaerobes such as Gemella, which is thought to be a biomarker for the exacerbation in CF lung (Carmody et al. 2013). OTUs corresponding to uncultivable bacteria affiliated to the TM6, TM7 and WPS-2 phyla also reported to be components of the oral microbiota (Adler et al. 2013), were present at low abundances in the sputum samples. While TM7 has already been detected in CF sputum samples (Blainey et al. 2012), this is the first time, to our knowledge, that TM6 and WPS-2 are reported in CF. The large abundance of so-called ‘oral bacteria’ in the respiratory microbiota of CF children corroborates the viewpoint that the oral cavity is a potential source of pathogens and other bacteria such as anaerobes that reach and colonize the lower airways of CF patients (Boutin et al. 2015; Rivas Caldas and Boisramé 2015). In fact, undoubtedly, upper and lower airways are interconnected and it would be interesting to determine the origin of pathogens to better understand their colonization process in CF.
High viral prevalence in CF sputum samples
In 52.6 % of samples (n = 10), at least one respiratory virus was detected while ≥2 viruses were found in 15.8 % of samples (n = 3). The most frequent viruses detected were human picornaviruses (rhinovirus or enterovirus) with a prevalence of 36.8 % (n = 7) in 4 of the 5 CF patients (Additional file 1: Table S1). We also detected in low proportion (n = 1) bocavirus type 1, parainfluenzae type 1 and type 2, coronavirus NL63, and influenzae A/H1N1v. There was no link between virus prevalence and P. aeruginosa abundance (Kruskal–Wallis test, FDR corrected >0.5). Rhinoviruses are commonly detected in CF children and are frequently associated with pulmonary exacerbations with worse severity in young CF patients (Asner et al. 2012). In accordance with the findings of Asner et al. (2012), peak prevalence of rhinovirus occurs in spring and fall months. It has been hypothesized that respiratory viruses could improve the acquisition of bacterial pathogens (Wat et al. 2008). In further study, it would be interesting to determine the influence of respiratory viruses on CF pulmonary microbiota.
CF respiratory tract microbiota dynamics throughout P. aeruginosa early colonization
Stability of the microbial structure in the early stages of P. aeruginosa colonization
Persistence of anaerobes
A specific microbiota composition relative to Lee’s status?
A way to evaluate whether P. aeruginosa had impacted the airway microbiota was to compare ‘never’ and ‘free’ patients’ microbiota. The difference in bacterial density and in the number of reads of P. aeruginosa between ‘never’ and ‘free’ patients was not statistically significant (p > 0.05) (Additional file 1: Table S1). Thus, bacterial density did not appear to be a potential marker of P. aeruginosa implantation. Similarly, Shannon’s index and equitability were not significantly different between ‘free’ and ‘never’ CF patients. Conversely, richness was significantly greater (p < 0.05) in ‘never’ [Chao-1: 79.8 (72.03–87.61); observed species: 71.6 (63.85–79.43)] than in ‘free’ patients [Chao-1: 62.7 (52–73.5); observed species: 55.9 (45.24–66.71)] (Additional file 2: Table S2). Moreover, as depicted in Fig. 2b, the structure of the microbiota was affected by the Lee’s status (see also Additional file 6: Fig. S3). Indeed, a significant clustering by Lee’s status was observed (Adonis test p = 0.0199, R2 = 0.105). The present results may suggest that the richness of the CF respiratory microbiota is directly negatively impacted by first acquisition of P. aeruginosa; this very preliminary data has to be reinforced with a larger sample dataset.
The present study allowed identifying bacterial species, including anaerobic bacteria, the role of which may be underestimated and which may be indirectly implicated in P. aeruginosa lung infection pathogenesis. In addition, this study demonstrated the impact of P. aeruginosa status on the composition of the CF lung microbiota. It was confirmed that core OTUs including anaerobes, were a common denominator in CF patients.
Further studies are needed to confirm these results and thereby improve our knowledge of the early stages of P. aeruginosa colonization. This pilot study underlines the importance of characterizing microbial communities associated with pulmonary clinical profiles, as longitudinal follow-up of CF patients could improve our overall view of the pathophysiology of lung infection in CF patients. Furthermore, the application of strategies such as respiratory microbiota transplantation or probiotics could delay pathogen implantation in CF patients. Henceforth, is it clearly demonstrated the crucial importance to follow the evolution of the pulmonary microbiota of CF patients allowing to monitor the efficiency of treatments and determine valuable predictive biomarkers.
SR performed DNA extraction. MK performed qPCR and pyrosequencing. MK, EP, JKJ and JM performed pyrosequencing data analysis. SG, MK and SV performed the respiratory virus multiplex PCR. MK, JM and GBu performed statistical analysis. GHA and GR contributed to data collection. GHA conceived and designed the study. JM, GR, SV, EC and GBa contributed to design. MK, GHA and JM wrote the manuscript. All authors read and approved the final manuscript.
This work was supported by a Grant to GHA from the French Cystic Fibrosis Association: ‘Vaincre la Mucoviscidose’ (contract no. RC20120600696) and the French Ministry of Higher Education and Research (Ministère de l’Enseignement Supérieur et de la Recherche: MESR, France). The Association had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript. Written informed consent was obtained from the CF patients or their relatives for publication of this manuscript and accompanying images. The authors are very grateful to the patients involved in this study.
Compliance with ethical guidelines
Competing interests The authors declare that they have no competing interests.
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