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BMC Microbiology

Open Access

Comparative genomic analysis of toxin-negative strains of Clostridium difficile from humans and animals with symptoms of gastrointestinal disease

  • Piklu Roy Chowdhury1, 2Email author,
  • Matthew DeMaere1,
  • Toni Chapman2,
  • Paul Worden1,
  • Ian G. Charles1, 3,
  • Aaron E. Darling1 and
  • Steven P. Djordjevic1Email author
BMC MicrobiologyBMC series – open, inclusive and trusted201616:41

https://doi.org/10.1186/s12866-016-0653-3

Received: 29 October 2015

Accepted: 2 March 2016

Published: 12 March 2016

Abstract

Background

Clostridium difficile infections (CDI) are a significant health problem to humans and food animals. Clostridial toxins ToxA and ToxB encoded by genes tcdA and tcdB are located on a pathogenicity locus known as the PaLoc and are the major virulence factors of C. difficile. While toxin-negative strains of C. difficile are often isolated from faeces of animals and patients suffering from CDI, they are not considered to play a role in disease. Toxin-negative strains of C. difficile have been used successfully to treat recurring CDI but their propensity to acquire the PaLoc via lateral gene transfer and express clinically relevant levels of toxins has reinforced the need to characterise them genetically. In addition, further studies that examine the pathogenic potential of toxin-negative strains of C. difficile and the frequency by which toxin-negative strains may acquire the PaLoc are needed.

Results

We undertook a comparative genomic analysis of five Australian toxin-negative isolates of C. difficile that lack tcdA, tcdB and both binary toxin genes cdtA and cdtB that were recovered from humans and farm animals with symptoms of gastrointestinal disease. Our analyses show that the five C. difficile isolates cluster closely with virulent toxigenic strains of C. difficile belonging to the same sequence type (ST) and have virulence gene profiles akin to those in toxigenic strains. Furthermore, phage acquisition appears to have played a key role in the evolution of C. difficile.

Conclusions

Our results are consistent with the C. difficile global population structure comprising six clades each containing both toxin-positive and toxin-negative strains. Our data also suggests that toxin-negative strains of C. difficile encode a repertoire of putative virulence factors that are similar to those found in toxigenic strains of C. difficile, raising the possibility that acquisition of PaLoc by toxin-negative strains poses a threat to human health. Studies in appropriate animal models are needed to examine the pathogenic potential of toxin-negative strains of C. difficile and to determine the frequency by which toxin-negative strains may acquire the PaLoc.

Keywords

Clostridium difficile Toxin-negative isolatesComparative genomicsCDIZoonosis

Background

Clostridium difficile is a Gram-positive pathogen that has emerged to become one of the leading causes of infectious diarrhoea in adult humans, securing its inclusion in the ESCAPE group of pathogens [14]. C. difficile infections range from being asymptomatic to causing mild or severe diarrhoea and occasionally life-threatening conditions such as pseudomembranous colitis and toxic megacolon [1, 5]. However, community-acquired C. difficile infection is being reported with increasing frequency [6] and C. difficile is also emerging as a pathogen in animals particularly cattle, pigs and horses [5, 710]. Molecular epidemiological studies show that infections in humans and animals can share the same ribotype or multilocus sequence type (ST) [11] suggesting that pathogenic C. difficile may traffic between humans and animals, although further studies are needed to confirm these linkages.

C. difficile is a genetically diverse and globally dispersed species [1116] having a clonal structure comprising six major clades (clades 1, 2, 3, 4, 5 and C-I). Clade C-I is the most phylogenetically divergent clade and may represent of a new subspecies of C. difficile [17]. Clade C-I typically comprise toxin-negative strains of C. difficile [17] but toxigenic variants that reside in Clade C-I have recently been described [18]. Representatives from most clades have been associated with CDI in humans and comprise toxigenic strains with A+/B+, A/B+ toxin types [11, 14, 17, 1922]. Non-toxigenic strains of C. difficile are represented in all six clades [11].

Toxin expression is considered mandatory for the development of C. difficile disease [23, 24]. Two large clostridial toxins known as toxins A (308 kDa) and B (260 kDa) encoded by tcdA and tcdB and the genes implicated in regulating their expression (tcdC, tcdE and tcdR) reside on a 19.6-kb pathogenicity locus known as the PaLoc [25, 26]. The PaLoc is replaced by 115/75 base pair non-coding region in toxin negative strains of C. difficile [27]. Approximately 20 % of C. difficile strains express a third toxin, known as the binary toxin (CDT) [28]. Genes encoding binary toxin (cdtA and cdtB) and a regulator gene (cdtR) are usually located on a locus (CdtLoc) that is physically separated from the PaLoc. A recent study described six toxin-negative (A-/B-) isolates of C. difficile that were positive for CDT from patient with symptoms of CDI [28].

Assays that detect toxin genes or the products of their expression dominate laboratory-based tests used to diagnose infections caused by C. difficile [29, 30]. Diagnostic tests that target tcd genes underestimate the frequency of detection of toxin-negative strains (including those that express binary toxin) in C. difficile disease and as such, their role in disease is poorly understood. Phylogenetic studies show that toxin-negative strains of C. difficile cluster tightly with toxin-positive isolates belonging to the same ST [17] suggesting that presence and absence of the PaLoc may be one of the major defining features that differentiate toxin-negative strains from toxin producing strains of C. difficile. Notably, oral bacteriotherapy with toxin-negative strains or their spores has been used successfully to treat patients undergoing long-term antibiotic regimes and prevent colonisation by toxigenic strains of C. difficile [3133]. The utility of this therapeutic strategy is supported by previous studies in hamsters which showed that exposure of the gastrointestinal tract to toxin-negative C. difficile strains prevented colonisation by toxin-positive strains [34, 35]. Interestingly, challenge studies in hamsters have shown that toxin-negative strains can effectively colonise the gut [36, 37] suggesting that toxin production may be of little consequence in determining the success of colonisation of the gastrointestinal tract. Notably, the toxin-negative strain CD1342 (tcdA , tcdB , cdtA and cdtB ) was reported to elicit an innate immune response in the caecum resulting in neutrophil infiltration, damage to epithelial mucosa and localised haemorrhagic congestion [36]. These findings suggest that virulence factors are carried by C. difficile in addition to the known toxins that can induce host pathology.

Studies of toxin-negative C. difficile strains have focused on the characterisation of functional binary toxins and their roles in pathogenesis [28, 33, 38]. The binary toxins cdtA and cdtB have adenosine diphosphate ribosyltransferase activity but their capacity to induce symptoms of C. difficile infection remains unclear [3942]. Several adhesins, ECM-binding proteins, proteases, motility proteins, hydrolytic enzymes and other surface-associated proteins have been described in C. difficile and these factors are likely to contribute significantly to the establishment, progression and severity of C. difficile disease [11, 43]. Therefore, further studies are needed to examine the pathogenic potential of toxin-negative strains of C. difficile and to determine the frequency at which toxin-negative strains may acquire the PaLoc and express toxins.

Studies that seek to understand the evolutionary history of the PaLoc highlight the complex nature of the multiple clade-specific acquisitions that have occurred after clonal expansion of each clade in populations of C. difficile [17]. Those studies report homologous and site-specific recombination events as having played an important role in the loss and gain of the PaLoc [17]. The PaLoc is proposed to be a mobile element that can transfer to toxin-negative strains rendering the recipient with the ability to produce clinically relevant concentrations of ToxA and ToxB [44]. Toxin-negative strains are purported to be ancestral to modern C. difficile but lateral genetic events complicate phylogenetic interpretation and alternate hypotheses have been proposed [17]. Genomic studies incorporating a greater diversity of toxin-negative strains of C. difficile are needed to shed light on their potential to cause disease.

Methods

Isolation and culture of Clostridium difficile

All C. difficile isolates analysed in this study (P29, 5.3, 19.3, 22.1, H3) were obtained from watery diarrhoea stool samples from their respective hosts (Additional file 1: Table S1). The porcine and equine C. difficile isolates analysed in this study were sourced in 2008 from different geographical locations in New South Wales, Australia. The porcine isolate P29 was isolated from a stool sample submitted by the veterinarian attending a piglet with severe but non-fatal diarrhoea. The equine isolate H3 was isolated from a live neonatal foal suffering from non-fatal watery diarrhoea. Stool samples were tested with PCR targeting major ETEC virulence genes [45] and common viruses known to cause diarrhoea in neonatal animals and were plated on blood agar plates to select for enteric pathogens. The stool specimens were initially tested for Escherichia coli, Clostridium perfringens and C. difficile using species-specific PCR primers [46]. Briefly, DNA was extracted from 500 μl of stool sample using a FastDNA spin kit (QBiogene, California, USA) and used as a template for PCR using primers specific for C. difficile and C. perfringens 16S rDNA [46], tcdA and tcdB genes (see below) and for E. coli [45]. To enrich for C. difficile 100 μl of each faecal sample was added to 10 ml cooked meat medium (TM0102 Oxoid Australia) and incubated anaerobically at 37 °C for 24 h using the anoxomat system (MART Microbiology B.B., The Netherlands).

Two hundred μl of culture samples that tested positive for C. difficile by PCR were transferred (from cooked meat media enrichment broth) into an Eppendorf tube and centrifuged (10,000 rpm, 5 min). The pellet was resuspended in 1 ml of absolute ethanol (room temperature, 2 h with periodic inversions), harvested by centrifugation (10,000 rpm, 5 min), resuspended in brain heart infusion broth (100 μl) and plated onto C. difficile selective agar (CC-BHIA + Taurocholate, PP2362 Oxoid Australia). Plates were incubated under anaerobic conditions at 37 °C for 24 h. Colonies morphologically representing C. difficile from each plate were selected and sub-cultured onto CC-BHIA + Taurocholate until pure cultures were achieved.

DNA extraction

For routine PCR, template DNA was extracted with Chelex (BIO-RAD) from 2 ml brain heart infusion broth cultures grown under anaerobic conditions at 37 °C for 48 h. Briefly, cell pellets were obtained by centrifuging (10,000 rpm for 5 min) 200 μl aliquots of liquid culture, washed 2 × with 500 μl of sterile water and resuspended in 200 μl of 6 % Chelex solution made in Tris-EDTA buffer (pH 7.5). The samples were incubated at 56 °C for 20 min, vortexed for 10 s and incubated at 100 °C for 8 min. After incubation, the sample was immediately transferred to ice. One aliquot was stored at 4 °C for routine PCR tests while the other aliquots were archived at −20 °C.

Sequencing-quality genomic DNA was prepared from 2 ml brain heart infusion broth culture of isolates grown under anaerobic conditions at 37 °C for 48 h. The overnight culture was harvested by centrifugation (10,000 rpm for 10 min), washed in sterile PBS and resuspended in 180 μl of lysis buffer comprising 20 mM Tris-HCl, pH 8.0, 2 mM EDTA, 1.2 % Triton X-100 and lysozyme (20 mg ml−1) and incubated for 45 min at 37 °C. DNA was isolated using a DNeasy® Blood and Tissue Kit (Qiagen) by adhering to the manufacturer’s instructions for the extraction of DNA from Gram-positive bacteria.

PCR conditions

C. difficile specific 16S rDNA primers, C.diff-F: 5′-TTGAGCGATTTACTTCGGTAAAGA-3′ and C.diff-R: 5′-CCATCCTGTACTGGCTCACCT-3′ were used for identification and confirmation of C. difficile in enrichment as well as pure cultures. The presence of the tpi gene (encoding Triose Phosphate Isomerase), tcdA gene (encoding Toxin A) and tcdB gene (encoding Toxin B) were tested using previously published primer pairs. Conditions for PCR were as described previously [22] with minor modifications. Briefly, PCR was carried out in 25 μl volumes containing 2 μl of Chelex extracted DNA, 2.5 μl of 10 × PCR buffer, 1.5 mM of MgCl2, 1 mM of each dATP, dGTP, dCTP and dDTP (Bioline, Australia), 0.5 μM of each primer and 1 U of BioRad Taq polymerase (Bioline, Australia). PCR cycling conditions consisted of an initial denaturation cycle (2 min, 95 °C) followed by 30 cycles of denaturation (94 °C, 1 min), annealing (55 °C, 1 min) and extension (72 °C, 2 min). The cycling process was completed with a final extension of 72 °C for 5 min.

Whole genome sequencing, data assembly and phylogenetic analysis

Sequencing was performed at the Next Generation Sequencing facility within the ithree institute at the University of Technology Sydney using a bench top Illumina MiSeq® sequencer and MiSeq V3 chemistry. Genomic DNA stocks shipped to the sequencing facility at concentrations between 1.8 and of 3.7 ng μl−1 were used as template for the preparation of sequencing libraries. The genomes were sequenced and assembled de novo using published protocols [47]. Raw data and assembled genome sequences were submitted in GenBank under the following Bio-project numbers, 5.3: PRJNA232267, 19.3: PRJNA239262, 22.1: PRJNA239264, P29: PRJNA239265 and H3: PRJNA238844.

PhyloSift was used to conduct a phylogenetic analysis of the five C. difficile genomes (P29, 5.3, 19.3, 22.1, H3) with nine closed C. difficile genomes including strains M120, CF5, M68, 2007855, BI1, CD196, R20291, ATCC43255 and CD630 available in the NCBI genome database on the 18th of December 2014 [48]. FigTree version 1.4.0 (http://tree.bio.ed.ac.uk/software/figtree/) was used to draw phylogenetic trees. Genome sequences of C. perfringens (ATCC13124), Clostridium botulinum (ATCC19397) and Clostridium tetani (E88) were included as outgroups in the analysis. To improve visual resolution of the evolutionary distances between test and reference strains of C. difficile the final figure was generated without the out-groups.

For reference-genome based phylogenetic inference, raw Illumina reads from all taxa were mapped to a single reference (strain CD630) using BWA-MEM (ver0.7.9a) (Li unpublished, github commit: 3efc33160c) and consensus sequences generated using the samtools/bcftools (ver0.1.19-96b5f2294a) tool-chain [49]. The complete set of consensus sequences were combined into a multiple sequence alignment. 1,216,986 alignment columns containing unresolved nucleotides (N) were removed using Mothur (ver1.33.3) [50]. A total of 3,073,266 (72 %) polymorphic and non-polymorphic sites were retained for further analysis. The inclusion of invariant sites has been demonstrated to improve accuracy of whole genome phylogeny [51]. Maximum likelihood phylogenetic inference was employed using RAxML (ver8.0.20) [52] with the following options: raxmlHPC-PTHREADS-SSE3 -T 40 -f a -x 2136841 -p 1486312 -N autoMRE -m GTRCAT. Inference was carried out under a general time reversible (GTR) substitution model with an infinite mixture model for substitutional heterogeneity (CAT), following the suggestion of the RAxML user guide for datasets of this size. The CAT approximation has been previously demonstrated to be an accurate and highly efficient alternative to Gamma-distributed rate heterogeneity on data sets with many taxa (73 – 1663) [53, 54]. Confidence in each clade of the Maximum Likelihood tree was estimated using the rapid bootstrap procedure [55] with automatic extended majority-rule criterion (100 bootstraps) and the resulting tree and bootstrap confidence estimates were visualized with FigTree version 1.4.0 (http://tree.bio.ed.ac.uk/software/figtree/).

Multi locus sequence typing and comparative genomic analysis

The online version of C. difficile PubMLST database (http://pubmlst.org/cdifficile/) was used to sequence type the isolates from the assembled genome sequences. The database was also exploited to locate certain genes of interest.

The online version of the RAST annotation server (http://rast.nmpdr.org/) [56] was used to annotate the genomes. The Classic RAST annotation scheme and FigFAM release 70 were used to predict genes (5.3 = RAST-ID 6666666.71923, 19.3 = RAST-ID 6666666.71924, H3 = RAST-ID 6666666.72094, P29 = RAST-ID 1440056.4 and 22.1 = RAST-ID 6666666.72093). Amino acid sequences corresponding to translated peptide products of all open reading frames predicted by RAST [57] from each of the five genomes were used in the ‘all Vs all’ homology search protocol deposited in the github repository as cRBLH (https://github.com/cerebis/crblh/tree/v0.1). The protocol included clustering of predicted peptide sequences using a modified reciprocal best hit method, where simplicity was favoured for the apparent advantage in identifying orthogroups [58]. The all vs. all homology search was carried out with LAST [5961] using runtime parameters (−T 1 -f 0 -e 100). The best hits were used to generate a directed graph with genes as vertices and best hits as edges. Unidirectional links between any two nodes were then pruned. Sets of disconnected subgraphs were then analysed for weak intra-cluster linkages, which likely represented overlap between partially homologous protein clusters. Each subgraph was subjected to modularity optimisation [62] and further decomposed until modularity scores of constituent elements fell below a given threshold (0.2). The nodes of the resulting subgraphs were then written out as protein clusters. Singletons defined as nodes without a single edge to any other were deemed unique/isolated genes.

Whole genome comparisons were performed using Mauve version 2.3.1 [63, 64] and iterative BLASTn analysis (http://blast.ncbi.nlm.nih.gov/Blast.cgi). Inter-isolate regions of interest identified from genome-wide comparisons using Mauve, BLASTp and protein clustering analyses were analysed further using iterative BLASTn and BLASTp searches. Figures of comparative genomic analysis, including comparisons of the PaLoc, were compiled using locally downloaded version of EasyFig version 2.1 [65].

The genome of the epidemic C. difficile CD630 strain was used in whole genome BLASTp analysis (in RAST) with our test C. difficile genomes to identify genes that have been correlated with pathogenicity. All genes deemed as candidate alternative virulence genes or genes for which the products could potentially confer pathogenic traits were individually interrogated using BLASTp and setting amino acid alignment cut off set to 100 % of input query sequence to avoid any data extrapolation.

Results

Toxin-negative C. difficile from animals and humans with clinical disease

The original stool samples and primary enrichment cultures of the stool samples tested negative for C. difficile toxins A and B. PCR assays using DNA from enrichment broths tested negative for enteric (other than C. difficile) and viral pathogens associated with neonatal diarrhoea. The porcine faecal sample was negative for the enterotoxigenic E. coli genes STa, STb and LT and C. perfringens and the disease symptomology did not correlate with viral disease as diagnosed by the attending veterinarian. Similarly, the foal sample was tested for E. coli, Salmonella enterica and rotavirus and none were detected. While gastrointestinal disease was most likely associated with the presence of toxin-negative C. difficile we cannot rule out the possibility that disease was caused by unculturable/unknown pathogens present in the gastrointestinal tract of these animals. Toxin-negative human C. difficile isolates 5.3, 19.3 and 22.1 were collected in the course of routine diagnostic tests for C. difficile-associated diarrhoea in patients presenting typical symptoms of the disease at a gastrointestinal clinic in Sydney, Australia in 2008.

Interrogation of the C. difficile PubMLST database confirmed that none of the toxin-negative isolates in our cohort (P29, H3, 5.3, 19.3, 22.1) had homologs of the known C. difficile PubMLST toxin genes (tcdA, tcdB, cdtA and cdtB) confirming our initial diagnostic PCR data for toxin A and B genes (Additional file 1: Table S1). Isolates 5.3 (ST15), P29 (ST109) and H3 (ST29) were distinct from each other and from ST types of Australian isolates included in a recent phylogenetic study of C. difficile (Additional file 1: Table S1) [17].

Phylogenetic analysis of toxin-negative isolates of C. difficile

A study of the evolution of the C difficile pathogenicity locus (PaLoc) identified an extremely divergent clade C-I that exclusively comprised toxin-negative isolates predominantly of Australian origin [17]. A maximum-likelihood phylogenetic tree using a reference-based, whole genome alignment protocol (see methods section for protocol details) that incorporates both variant and invariant sites of the C. difficile genome sequences was used to verify the ancestry of our toxin-negative isolates. Our approach uses approximately 72 % of the C. difficile genome for the analysis, considerably more than what was used in the original study [17]. All 73 genomes and the reference genome CD630 used in the previous study [17] as well as additional closed genomes of C. difficile (strains 2007855, ATCC43255, BI1, CF5, M68, M120 and R20291 from the GenBank database) were used in our initial phylogenetic analysis. A preliminary phylogenetic tree (Additional file 2: Figure S12) revealed that our genome-based phylogeny was largely congruent with that described in an earlier study [11] and clearly indicated that none of the five genomes that were the subject of our study clustered within the divergent clade C-I.

Strains that resided within clade C-I showed greater than 5 % sequence divergence from the reference genome at homologous sites. Clades that have diverged more than 5 % from the reference genome can be poorly resolved in workflows based on Illumina read mapping to the reference [51]. Given this and the uncertain ancestry of the isolates included in clade C-I in the Dingle et al. [11] study, members of clade C-I were excluded from the subsequent analysis based on a cohort of 86 strains depicted in Fig. 1. The branching order of the five clades in our phylogenetic tree was congruent with that reported earlier [17] with identical clustering of strains in the different sub-clades within each of the five clades. The five toxin-negative isolates from our study clustered with strains in Clades 1 (C. difficile 5.3, and H3) and 4 (C. difficile 19.3, 22.1 and P29) that are known to contain toxin-negative strains [17]. Our toxin-negative isolates (sourced both from animal and human sources) also clustered with strains of the same sequence type that included both toxin-positive and toxin-negative strains isolated from human clinical specimens in an earlier study [17].
Fig. 1

A midpoint rooted phylogenetic tree depicting the five C. difficile clades. Australian toxin-negative strains are identified with blue strain names. Complete, closed genomes available in GenBank that were used as a reference are in green text. Genome names in black text are from a previous study [20]. The tree was constructed from reference-based whole genome alignments. Strains within boxed regions indicate genomes used in the ALL vs ALL BLASTp analysis. Clades highlighted in blue indicate clade 4 and in aqua is clade 1

Our genome sequences were assembled with a de novo assembler using A5 [48]. Prior to conducting a detailed analysis of the toxin-negative C. difficile isolates we identified the closest reference genome for tiling genomic scaffolds. A preliminary phylogeny generated using PhyloSift and FastTree (Additional file 2: Figure S2) indicated that C. difficile strain CF5 (toxin-positive ST86) was the most appropriate reference to order genomic scaffolds of isolates 19.3 (ST39), 22.1 (ST39) and P29 (ST109) while C. difficile strain 630 (toxin-positive, ST54 (PCR ribotype 012) was appropriate to order genomic scaffolds of isolates 5.3 (ST15) and H3 (ST29). Strain CF5 was isolated from a patient in Belgium in 1995 while CD630 is a highly virulent, multiple antibiotic resistant strain of C. difficile that caused pseudomembranous colitis in a human patient and later caused an epidemic of C. difficile infection in a Swiss hospital ward in 1982. All down-stream analyses of the genomes presented in this study were performed on genomic assemblies with scaffolds ordered to match the reference genomes.

Homology based functional similarity in the toxin-negative isolates

Initially a Progressive Mauve alignment performed (Additional file 2: Figure S3) on genome sequences of human ST39 isolates 19.3 and 22.1 revealed a high level of nucleotide identity across the genomes with 324 SNP differences. Most of the SNPs were clustered into 7 groups (see Additional file 3: Table S4) suggesting that lateral gene transfer or homologous recombination-mediated genomic rearrangements may be responsible for the differences and were not considered further. Only 27 SNPs were identified that could generate changes in the amino acid sequence of the predicted proteins in the table Additional file 3: Table S4.

To identify genes affected by the SNP changes, a bi-directional BLASTp comparison of 3772 proteins comprising the predicted proteome of strain 19.3 was performed with 3764 predicted protein sequences from strain 22.1 in RAST. The analysis identified 3750 protein sequences that were identical in both the genomes. Nine protein sequences had greater than 99 % sequence identity, six others had greater than 97 % sequence identity and one ORF encoding a hypothetical protein showed 49 % sequence identity (Additional file 3: Table S5). Proteins sharing 97 and 99 % sequence identity predominantly encoded components of the bacterial cell surface including N-acetylmuramoyl-L-alanine amidase, flagellar assembly protein FliH, lipoprotein signal peptidase, putative ABC transporters and permeases. Eight ORFs in isolate 19.3 predominantly encoding hypothetical proteins were missing in isolate 22.1. The genomes of isolates 19.3 and 22.1 comprise 4,181,809 and 4,180,898 bp respectively.

Since isolates 22.1 and 19.3 had high levels of homology, predicted proteins only from isolate 19.3 were included in a pairwise bi-directional BLASTp analysis that seeks to identify conserved genes and major differences among toxin-negative isolates of Australian origin. Isolate P29 had the largest predicted proteome in our collection and was used as the reference. Comparisons of predicted proteomes of human isolates 5.3 & 19.3 and equine isolate H3 with P29 identified major differences in regions harbouring prophage-associated proteins, hypothetical proteins (Additional file 3: Table S5) and putative transposases associated with mobile genetic elements.

Chromosomal context of the PaLoc insertion site

In toxin-negative strains, a 115 bp sequence replaces the PaLoc locus in phylogenetic clades 1 and 4 and the genetic context in which the 115 bp sequence resides varies within the different clades that represent the C. difficile population structure [17]. An analysis of the genetic context of the 115 bp sequence in our toxin-negative isolates compared to GenBank sequence entries representing chromosomal regions adjacent to the PaLoc insertion site in toxin-negative strains belonging to Clades 1 (GenBank Accession no HG002393) and 4 (GenBank Accession no HG002391) is depicted in Fig. 2. We identified several SNPs within the 115 bp-conserved fragment and an 80 nt long insertion in strains 5.3 and H3 downstream of the gene designated CD06642 in the reference genomes (Fig. 2). In addition, we identified a 68 nt tandem repeat of the sequence adjacent to the 80 nt insertion site in strain H3 (see Additional file 2: Figure S7). Within members of clade 4, porcine isolate P29 had a deletion of the hypothetical gene seen in the reference region while human isolates 19.3 and 22.1 had a significant decrease in the nucleotide identity in hypothetical genes in the reference genome. Consistent with observations reported earlier, these differences indicate ongoing micro-evolutionary events within the locus that flanks the PaLoc insertion site [17].
Fig. 2

Genetic context of the PaLoc in Australian toxin-negative strains of C. difficile. a Clade 1 prototype OxI_WB2011 (HG002393). b Clade 4 prototype Oxa464a (HG002391)

Comparative BLASTp analyses of toxin-negative strains to identify functional similarities between groups of isolates

An all versus all BLASTp based protein-clustering analysis was used to identify the putative core proteome of a subset of Clade 1 strains comprising five genomes and Clade 4 strains comprising 10 genomes (see boxed region in Fig. 1). To maintain uniformity in the input data used in the analysis, raw reads representing each of the genomes from an earlier study [17] were reassembled and annotated using the protocols that were used to assemble and annotate the five toxin-negative Australian isolates of C. difficile reported in this study, as described above. The assembly statistics and a comparison of the assembly outputs are presented in Additional file 3: Table S8. On an average, RAST predicted 3700 proteins per genome and these were included in the protein clustering analysis. A bit score cut off of 50 was used to cluster homologous protein sequences. An overview of the data is presented in Table 1.
Table 1

Summary of protein clustering results within the different sub-clades containing the five toxin negative isolates included in this study. Summary of protein clusters within the different sub-clades of C. difficile

Clade 1

Genome names

No of predicted proteins

 Core genome

3323

Total number of unique peptides in:

C. difficile C0000509

45

C. difficile C0000541

38

C. difficile C0000562

176

C. difficile C00005945

212

C. difficile H3

111

Clade 4:

 Core genome

3357

Total number of unique peptides in:

C. difficile 19.3

8

C. difficile 22.1

7

C. difficile C00000089

33

C. difficile C000011286

86

C. difficile C00006473

84

C. difficile C00007671

35

C. difficile C00011267

60

C. difficile CF5

30

C. difficile M68

19

C. difficile P29

299

Ten clade 4 genomes boxed in Fig. 1 shared 3357 proteins (Table 1). Isolate P29 had the highest number (299) of unshared/unique proteins within the clade 4 cohort and most of the 299 proteins were phage-related (Additional file 3: Table S9). Some of the unique proteins clustered together in the same scaffold indicating lateral movement of phage-associated genomic DNA. C. difficile isolates 19.3 and 22.1 carried eight and seven unique proteins respectively. The handful of unshared proteins in 19.3 and 22.1 were attributed to mobile genetic elements or were designated to encode proteins of unknown function. The five C. difficile strains within clade 1 shared 3323 proteins. Equine isolate H3 had 111 unique proteins, most of which were phage related or hypothetical with some clustered in single scaffolds (Additional file 3: Table S9).

We queried the viral and prophage database in GenBank with the genome sequences of all five toxin-negative isolates using PHAST [66]. The database confirmed the presence of several regions contain phage DNA in each of the five genomes in Clade 1 (see Additional file 2: Figure S10 and Additional file 4: Table S11). Table 2 lists a summary of the complete prophage sequences (PHAST scores > 110 and over) identified in the five Australian toxin-negative isolates. Notably, isolates 19.3 and 22.1 returned identical phage profiles (Additional file 2: Figure S10). Both genomes carried an identical and complete 56.8 kb phage that is a close relative of phiC2, a 56.5 kb phage first identified in C. difficile strain CD242 [67]. phiC2 is one of the first completely sequenced temperate phages in C. difficile and regions of phiC2 are present in the majority of C. difficile genomes of clinical origin [68]. We also identified a phage in isolates P29 and H3 that carries sequence identity with phiC2. The prophage in P29 was larger (97.4 kb) than the original phiC2 sequence (Additional file 2: Figure S10). Isolate P29 also carries two other complete prophage sequences. One of these, prophage region 9 has significant sequence identity to the C. difficile temperate bacteriophage phiCD6356 that belongs to the Siphoviridae family [69]. The Siphoviridae family prophage identified in P29 is 52.8 kb (Additional file 4: Table S11) and is considerably larger than the first report of this phage sequence at 37.6 kb [69]. Isolate H3 also carries an identical variant of phage phiCD6356 (Additional file 2: Figure S12) comprising 41.1 kb. Evidence of other complete prophage genomes is listed in Table 2. Comparative BLASTp analysis of the four genomes (19.3, 5.3, H3 and P29) also aligned to the phage search protocol and confirmed the data generated by PHAST analyses, reinforcing the observation that the major differences in our Australian toxin-negative C. difficile isolates have a prophage origin.
Table 2

Summary of Phage related regions identified by PHAST in the 5 genomes. Phage sequences identified in this study

PHAST region identifier

Length of prophage

PHAST score

No of predicted CDS

Relative position on genome

Predicted Phage

GC content

Location on Genomic scaffolds

C difficile P29 genome

 Region_4

97.4Kb

150

126

1732045-1829500

PHAGE_Clostr_CDMH1_NC_024144

28.7

27.1, 30.1, 40.1, 34.1, 36,1, 5.1, 47.1 and 16.1

 Region_8

113.6Kb

150

101

3773336-3886941

PHAGE_Geobac_virus_E2_NC_009552

40.8

5.1, 19.1 and 22.1

 Region_9

52.8Kb

140

65

4233532-4286418

PHAGE_Clostr_phiCD6356_NC_015262

29.9

8.1, 26.1, 41.1 and 42.1

 Region_10

21.3Kb

100

22

4290994-4312349

PHAGE_Clostr_phiC2_NC_009231

36.4

In over 20 very small scaffolds

C. difficile H3 genome

 Region_2

41.1Kb

150

63

925289-966449

PHAGE_Clostr_phiCD6356_NC_015262

28.5

22.1 and 31.1

 Region_3

50.1Kb

110

66

1114600-1164714

PHAGE_Clostr_phiC2_NC_009231

28.1

18.1 and 5.1

 Region_6

31.5Kb

110

47

4070500-4102080

PHAGE_Clostr_phiC2_NC_009231

29.4

26.1, 27.1, 28.1, 32.1, 33.1

C. difficile 5.3 genome

 Region_3

57.9Kb

140

87

1555612-1613526

PHAGE_Clostr_phiC2_NC_009231

28.6

1.1

 Region_4

45.1Kb

150

49

1741883-1787019

PHAGE_Clostr_phiSM101_NC_008265

27.2

1.1

C.difficle 19.3 genome

 Region_3

56.8Kb

140

74

1700180-1757059

PHAGE_Clostr_phiC2_NC_009231

28.8

1.1

C. difficile 22.1 genome:

 Region_3

56.8Kb

140

74

1703858-1760737

PHAGE_Clostr_phiC2_NC_009231

28.8

3.1

Comparative BLASTp analysis of isolates 19.3, 5.3, H3 and P29 identified a 119.3 kb region on contig 11 in P29 (Additional file 5: Table S6). An all versus all protein clustering analysis also identified a subset of unique proteins on contig 11 of the P29 genome but not in the 10 human C. difficile genomes within clade 4 (Fig. 1). Equine isolate H3 was not included in this analysis as it was on a different clade. BLASTn analysis of the 119.3 kb region against the C. difficile genome database in GenBank identified similarity at the DNA level to parts of C. difficile strain CD630 indicating a phage-mediated lateral movement of parts of the genome of CD630 into the genomes of isolates H3 and P29.

Homology based functional prediction of Putative C. difficile virulence factors implicated in host colonization

A homology-based functional prediction analysis of proteins that have been experimentally verified, or predicted to play a role in the colonization of C. difficile strain CD630 with homologous proteins in the genomes of the toxin-negative isolates in our study is shown in Table 3 [70, 71]. Most of the proteins i had near perfect (98–100 %) protein sequence identity including proteins encoded by spo0A, which serves as a positive regulator for genes required in spore germination and groEL, a chaperone that also functions as an adhesin [72]. Several serine-proteases and other metalloproteases which may contribute to the disease development process [70] were also highly conserved. However, some membrane associated proteins that have been shown to play significant roles in the disease development process had lower alignment scores including SlpA, a surface layer protein that is proposed to facilitate host cell adherence [73] and FliC, an adhesin necessary for the colonization of gut epithelium [74].
Table 3

Proteins derived from C. difficile CD630 that are predicted to play a role in pathogenesis

Selected gene and product

C. difficile 630 locus tag

Experimental Verification

RAST Annotation identifiers

In C. difficile 5.3 (% identity)

In C. difficile 19.3 (% identity)

In C. difficile H3 (% identity)

In Cc difficile P29 (% identity)

Flagellin C gene fliC

CD630_02390

yes, RNAseq

fig|6666666.71923.peg.3142 (86)

fig|6666666.71924.peg.3067 (71)*

fig|6666666.72094.peg.3176 (87)

fig|1440056.4.peg.3191 (97)

Flagellin D gene fliD

CD630_02370

no

fig|6666666.71923.peg.3140 (88)

fig|6666666.71924.peg.3065 (61)

fig|6666666.72094.peg.3174 (88)

fig|1440056.4.peg.3193 (98)

Precursor S-layer protein gene slpA

CD630_27930

yes, proteome

fig|6666666.71923.peg.2081 (43)*

fig|6666666.71924.peg.3725 (59) *

fig|6666666.72094.peg.2466 (58)*

fig|1440056.4.peg.2665 (54)*

Stage 0 Sporulation gene spoA

CD630_12140

yes, proteome

fig|6666666.71923.peg.158 (100)

fig|6666666.71924.peg.1561 (99)

fig|6666666.72094.peg.2932 (99)

fig|1440056.4.peg.240 (99)

Fibrinectin binding proten encoding fbpA gene

CD630_25920

no

fig|6666666.71923.peg.2930 (99)

fig|6666666.71924.peg.2028 (98)

fig|6666666.72094.peg.3740 (99)

fig|1440056.4.peg.41 (98)

GroEL encoding gene groL

CD630_01940

yes, proteome

fig|6666666.71923.peg.3095 (100)

fig|6666666.71924.peg.2995 (99)

fig|6666666.72094.peg.3129 (100)

fig|1440056.4.peg.3232 (99)

Cell surface protein cwp66

CD630_27890

no

fig|6666666.71923.peg.2085 (60)

fig|6666666.71924.peg.3721 (78)

fig|6666666.72094.peg.2462 (77)

fig|1440056.4.peg.2669 (79)

Protease cwp84

CD630_27870

no

fig|6666666.71923.peg.2087 (98)

fig|6666666.71924.peg.3719 (99)

fig|6666666.72094.peg.2460 (99)

fig|1440056.4.peg.2671 (99)

Adhesin (LPXTG)

CD630_28310

no

fig|6666666.71923.peg.2041 (99)

fig|6666666.71924.peg.3767 (94)

fig|6666666.72094.peg.2504 (98)

fig|1440056.4.peg.2625 (94)

Cell wall binding protein encoding cwp2

CD630_27910

yes, proteome

fig|6666666.71923.peg.2083 (98)

fig|6666666.71924.peg.3723 (99)

fig|6666666.72094.peg.2464 (99)

fig|1440056.4.peg.2667 (99)

Cell wall binding protein encoding cwp12

CD630_27940

no

fig|6666666.71923.peg.2080 (65)*

fig|6666666.71924.peg.3726 (98)

fig|6666666.72094.peg.2467 (95)

fig|1440056.4.peg.2664 (94)

Cell wall binding protein encoding cwp11

CD630_27950

yes, proteome

fig|6666666.71923.peg.2079 (98)

fig|6666666.71924.peg.3727 (99)

fig|6666666.72094.peg.2468 (99)

fig|1440056.4.peg.2663 (99)

Cell wall binding protein encoding cwp9

CD630_27980

no

fig|6666666.71923.peg.2076 (99)

fig|6666666.71924.peg.3730 (99)

fig|6666666.72094.peg.2471 (99)

fig|1440056.4.peg.2660 (99)

Cell wall hydrolase (LPXTG)

CD630_01830

no

fig|6666666.71923.peg.3084 (97)*

fig|6666666.71924.peg.2984 (99)

fig|6666666.72094.peg.3118 (100)

fig|1440056.4.peg.3243 (99)

Cell wall binding protein encoding cwp25 gene

CD630_08440

no

fig|6666666.71923.peg.2189 (100)

fig|6666666.71924.peg.3292 (97)

fig|6666666.72094.peg.2128 (99)

fig|1440056.4.peg.522 (97)

N-acetylmuramoyl-L-analini amidase encoding cwp16

CD630_10350

no

fig|6666666.71923.peg.1 (99)

fig|6666666.71924.peg.3716 (65)*

fig|6666666.72094.peg.1495 (99)

fig|1440056.4.peg.1845 (98)

Cell wall hydrolase encoding gene (invasin)

CD630_27680

no

fig|6666666.71923.peg.2107 (99)

fig|6666666.71924.peg.3700 (99)

fig|6666666.72094.peg.2441 (99)

fig|1440056.4.peg.2690 (99)

Polysaccharide de-acetylase

CD630_15220

yes, RNAseq and proteome

fig|6666666.71923.peg.489 (100)

fig|6666666.71924.peg.291 (99)

fig|6666666.72094.peg.3592 (100)

fig|1440056.4.peg.1197 (99)

LmbE-like deacetylase encoding gene

CD630_27900

no

fig|6666666.71923.peg.2084 (93)

fig|6666666.71924.peg.3722 (100)

fig|6666666.72094.peg.2463 (100)

fig|1440056.4.peg.2668 (97)

Invasin/Sh3 domain containing surface protein

CD630_11350

no

fig|6666666.71923.peg.77 (100)

fig|6666666.71924.peg.1641 (98)

fig|6666666.72094.peg.2849 (99)

fig|1440056.4.peg.320 (98)

Cell wall hydrolase/Invasin associated protein

CD630_24020

 

fig|6666666.71923.peg.2730 (100)

fig|6666666.71924.peg.2779 (98)

fig|6666666.72094.peg.2094 (99)

fig|1440056.4.peg.3691 (99)

Autolysin acd gene homolog/mannosyl-glycoprotein endo neta N acetylglucosamine

CD630_13040

no

fig|6666666.71923.peg.256 (100)

fig|6666666.71924.peg.1460 (98)

fig|6666666.72094.peg.3031 (99)

fig|1440056.4.peg.158 (98)

Protease/Serine protease, HrtA family

CD630_32840

no

fig|6666666.71923.peg.1608 (100)

fig|6666666.71924.peg.3459 (99)

fig|6666666.72094.peg.64 (100)

fig|1440056.4.peg.2801 (99)

Intracellular serine protease

CD630_32540

no

fig|6666666.71923.peg.1638 (100)

fig|6666666.71924.peg.3426 (99)

fig|6666666.72094.peg.94 (99)

fig|1440056.4.peg.2834 (99)

Protease/Subtilase family

CD630_07030

no

fig|6666666.71923.peg.2324 (100)

fig|6666666.71924.peg.3155 (97)

fig|6666666.72094.peg.2691 (100)

fig|1440056.4.peg.1169 (97)

Ser-type protease/subtilisin-like serine germination related protease

CD630_22470

yes, Mass spectrometry

fig|6666666.71923.peg.1327 (99)

fig|6666666.71924.peg.2513 (99)

fig|6666666.72094.peg.1937 (99)

fig|1440056.4.peg.1500 (98)

Serine protease precursor/Subtilinase subfamily

CD630_20000

no

fig|6666666.71923.peg.1085 (100)

fig|6666666.71924.peg.2267

fig|6666666.72094.peg.1687 (99)

fig|1440056.4.peg.2329 (99)

Membrane-associated zinc metalloprotease/M50 family peptidase

CD630_21290

no

fig|6666666.71923.peg.1209 (100)

fig|6666666.71924.peg.2404 (99)

fig|6666666.72094.peg.1813 (100)

fig|1440056.4.peg.1610 (100)

Zinc Protease/M16 family peptidase

CD630_26610

yes, proteome

fig|6666666.71923.peg.2996 (100)

fig|6666666.71924.peg.626 (99)

fig|6666666.72094.peg.3677 (100)

fig|1440056.4.peg.438 (99)

* indicates gaps in alignment of amino acid sequences with reference, likely suggesting presence of inactive proteins or variants in the test genomes

Discussion

C. difficile colonisation in humans is age dependent. While asymptomatic carriage is common in infants less than three years of age it is rare in adults [75]. As such, infants can be a major reservoir of both pathogenic and toxin-negative strains in a community setting [75]. We isolated five toxin-negative isolates of C. difficile including three from humans (22.1, 19.3, 5.3), one from a pig (P29) and one (H3) from a horse all showing symptoms of gastrointestinal disease. Despite efforts to identify C. difficile toxin genes or toxin gene products in the stool samples during the course of the isolation of these strains, none were detected. Phylogenetic studies showed that human ST39 isolates 19.3 and 22.1 and porcine ST109 isolate P29 grouped with clinical human toxigenic strains of ST39 and ST109 respectively in Clade 4. Furthermore, human ST15 isolate 5.3 and equine ST29 isolate H3 grouped with human clinical toxigenic strains with ST15 and ST29 respectively in Clade 1. Comparative genome analyses showed that our toxin-negative isolates displayed virulence gene profiles akin to those identified in toxigenic strains. The animals from which samples were collected in this study exhibited gastrointestinal disease and we were unable to attribute these symptoms to the presence of toxin-positive strains of C. difficile. Given the mobility of the PaLoc [44] and evidence that the acquisition or loss of the PaLoc via recombination [17] has occurred multiple times during the evolution of the five major clades of C. difficile [11, 17], our data reinforces calls to include toxin-negative strains in genomic epidemiological studies of C. difficile [17, 36] and to better characterise asymptomatic carriage of closely related Clostridia in gut microbiome surveys such as the Human Microbiome Project and MetaHIT, both in humans and close animal contacts.

Our reference-based whole genome alignment and phylogeny analyses support the global population structure of C. difficile as described by Dingle et al. in 2014 [14, 17, 19]. Each clade has been shown previously to have representatives of both toxin-positive and toxin-negative strains [11]. Our toxin-negative isolates (19.3, 22.1, 5.3, P29, H3) belonged to STs that are distinct from those reported in an earlier study [17]. The role of toxins in C. difficile infection has been extensively studied but factors that enable C. difficile to efficiently colonise the human gastrointestinal tract are relatively poorly understood and are not associated with genes encoded on the PaLoc. It is not known why some toxigenic strains evolve into dominant hypervirulent clones. Thus, considering the genetic diversity inherent within the phylogenetic structure of C. difficile [14] a sub-population of toxin-negative strains of C. difficile that are efficient colonisers of the host gastrointestinal tract may readily acquire the PaLoc and evolve to become future hypervirulent strains. Several proteins have been suggested to play crucial roles in the colonization of gastrointestinal epithelium and disease progression [43, 71, 73, 74, 7678]. A recent global proteome study of C. difficile strains CD630 and R20291 has identified numerous extracellular proteins from culture supernatants that may contribute to the virulence attributes of these strains [70].

Our study reinforced the important role played by phage in the evolution of C. difficile. While PHAST analysis was useful for identifying phage sequences, the analysis may not have identified the full extent of lysogenic phage because our draft genomes remain in multiple scaffolds. Although the complete sequence of phage phiC2 was identified in isolates 19.3 and 22.1 the regions that had significant homology with phiC2 in isolates P29 and H3 were located on different scaffolds. We used a scaffold tiling approach against the closed genome of a reference strain to create the input file for PHAST analysis (PHAST converts the scaffolded genomes into a concatenated artificial chromosome prior to predicting the phage content) and as such it remains a possibility that the partial matches are a consequence of the data handling process. Phage phiC2 is present in the majority of human isolates of C. difficile [68]. However, we detected regions of phiC2 in strains P29 and H3 suggesting that further studies are needed to address issues surrounding the association of phiC2 in C. difficile of animal origin. We also identified the C. difficile temperate bacteriophage phiCD6356 from the Siphoviridae family in isolates P29 and H3 but not in our human isolates of C. difficile. Genomes of bacteriophages belonging to the Siphoviridae family range in size from 14 to 50 kb [79, 80] and this broad range may be a reflection of the stringency governing the amount of DNA that can be packaged by phiCD6356. In addition to the acquisition of phage-associated genes, a 119.3-kb region on contig 11 in isolate P29 was also identified in the course of this analysis. This region is unique to the P29 genome and displayed significant DNA sequence identity to portions of the CD630 genome. It remains unknown if the 119.3-kb region exists in C. difficile strains of porcine origin. Further analyses with greater numbers of genomes from both human and animal sources are required to conclusively address these questions.

Conclusions

Our studies reinforce calls to improve our understanding of the physiological conditions that promote lateral transfer of the PaLoc in the gastrointestinal tract [44]. This is important because the conditions that facilitate movement of fragments of DNA carrying the PaLoc and their recombination into the chromosome are also conducive to the movement of conjugative transposons that carry antibiotic resistance genes and putative virulence factors as independent genetic events [44].

Data accessibility

Genome sequences reported in this analysis were submitted to GenBank and are available via the accession numbers provided. The bioinformatics softwares are made available through the GitHub repository links.

Declarations

Acknowledgements

This work is a product of the ausgem partnership. The authors wish to acknowledge Prof Thomas Borody for kindly providing the human isolate included in this analysis.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
The ithree institute, University of Technology Sydney
(2)
NSW Department of Primary Industries, Elizabeth Macarthur Agricultural Institute
(3)
Institute of Food Research, Norwich Research Park

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