The human commensal Haemophilus parainfluenzae is emerging as an opportunistic multidrug-resistant pathogen. The objectives of this work were to characterise a new capsular operon of extensively drug-resistant (XDR) H. parainfluenzae clinical isolates and study their resistance mechanisms using whole-genome sequencing. All strains were resistant to: ß-lactams, via amino acid changes in PBP3 (S385T, I442F, V511A, N526K and V562I); quinolones, by alterations in GyrA (S84F and D88Y) and ParC (S84F and S138T); chloramphenicol, through the presence of catS; macrolides, via the presence of mel and mef(E)-carrying MEGA element; and tetracycline, through the presence of tet(M) and/or tet(B). Phylogenetic analysis revealed high genomic diversity when compared to the H. parainfluenzae genomes available on the NCBI, the isolates from this study being closely related to the Swiss XDR AE-2096513. A full capsular operon showing homology to that of H. influenzae was identified, in accordance with the observation of a capsular structure by TEM. This study describes for the first time a capsular operon in H. parainfluenzae, a major determinant of pathogenicity that may contribute to increased virulence in XDR clinical isolates. Moreover, phylogenetic analysis suggests the possible spread of an XDR-encapsulated strain in Europe.
The members of the genus Haemophilus are pleomorphic and fastidious Gram-negative coccobacilli that require supplementary factors for in vitro growth, particularly V-factor (β-nicotinamide adenine dinucleotide, NAD) and/or X-factor (haem)1,2. These nutritional requirements are essential in dividing this genus into three groups: the haem-dependent H. influenzae group (H. influenzae, H. haemolyticus and H. aegyptius); the haem-independent H. parainfluenzae group (H. parainfluenzae, H. parahaemolyticus, H. paraphrohaemolyticus, H. pittmaniae and H. sputorum); and the group containing H. ducreyi that requires haem, but not NAD for growth1. As a representative of the haem-independent group, H. parainfluenzae is characterised by its ability to synthesise haem, while depending on the presence of NAD in the environment for growth1.
H. parainfluenzae is part of the human oropharyngeal and genitourinary microbiota and is increasingly recognised as an opportunistic pathogen causing invasive, chronic or recurrent diseases, including respiratory tract infections3, meningitis4, endocarditis and pericarditis5, bone and joint infections6, and arthritis7. Recent reports have also linked this pathogen to genitourinary and sexually transmitted infections8,9,10, with one study observing unexpectedly high genital carriage in pregnant women that was frequently associated with antibiotic resistance traits8. In urethral exudates from men with acute Haemophilus spp. urethritis, H. parainfluenzae was observed to be six times more frequent than H. influenzae10. Likewise, urinary tract infections in children have shown differences with gender, with H. influenzae being the main species identified in girls and H. parainfluenzae in boys presenting urinary tract abnormalities, such as malformation, gross reflux or bladder dysfunction11. Moreover, H. parainfluenzae urethritis has also been described in men who have sex with men (MSM), highlighting the potential role of this microorganism in causing sexually transmitted diseases (STD)9.
Virulence factors play a crucial role in the invasion and infection process. Although the capsule has not yet been described in H. parainfluenzae, it is one of the most important virulence factors in H. influenzae and has been used for vaccine development. To date, six different capsular serotypes have been described for H. influenzae (a to f). The genes encoding the capsule are located in the cap locus, which is divided into three different regions. Region I contains four common genes (bexDCBA) that are responsible for the translocation of the capsular polysaccharides. Genes belonging to region II are serotype-specific and are associated with polysaccharide biosynthesis. Finally, region III contains two genes (hcsAB) that are involved in post-polymerisation steps12.
Along with virulence factors, antimicrobial resistance is also important during the course of infection and identifying such resistance is required to apply correct antimicrobial treatment. H. parainfluenzae is often resistant to β-lactam antibiotics13 and although resistance to fluoroquinolones and macrolides is still uncommon, isolates presenting reduced susceptibility to these antimicrobial agents are being increasingly reported14. In 2011, a multidrug-resistant (MDR) H. parainfluenzae clinical isolate, presenting resistance to quinolones, tetracycline and co-trimoxazole, was reported in a patient with prostatitis in Spain15. Two years later in Switzerland, a case study of an MSM man co-infected with a pan-susceptible Neisseria gonorrhoeae isolate and an extensively drug-resistant (XDR) H. parainfluenzae strain was described16. XDR microorganisms are defined as resistant to at least one agent in all but two or fewer antimicrobial categories17 and are a significant cause for concern. Our study aimed to describe for the first time a capsule in four XDR H. parainfluenzae strains and fully characterise their molecular antibiotic resistance mechanisms.
Characterisation of antimicrobial resistance
Three isolates were resistant to all the tested β-lactams (ampicillin, cefuroxime, cefotaxime, cefepime, amoxicillin/clavulanic acid and ceftriaxone), except for the carbapenems (imipenem and meropenem). A single isolate remained susceptible to amoxicillin/clavulanic acid and ceftriaxone. All the isolates were also resistant to chloramphenicol, macrolides, quinolones and co-trimoxazole, only remaining susceptible to rifampicin (Table 1).
The mechanisms of antimicrobial resistance were detected in silico (Table 1). Resistance to β-lactams was associated with amino acid substitutions in the penicillin-binding protein (PBP3). Five substitutions were present in all the strains [S385T, I442F, V511A, N526K and V562I], while three additional changes [K276N, A307N and V329I] were only present in HUB12435, HUB12445 and HUB12640. The presence of β-lactamase was not detected in any of the isolates. Fluoroquinolone resistance was attributed to amino acid substitutions in DNA gyrase (GyrA) [S84F and D88Y] and in DNA topoisomerase IV subunit A (ParC) [S84F and S138T] and subunit B (ParE) [D420N and A451S]. Macrolide resistance was conferred by the amino acid substitution A69S in the 50S ribosomal protein L4, encoded by the rplD gene, and by the acquisition of the MEGA element containing mel and mef(E). Tetracycline resistance was attributed to the tet(M) gene located upstream of the MEGA element, as described previously for H. parainfluenzae18. Resistance to chloramphenicol was linked to the presence of an acetyltransferase encoded by the catS (CP015430.1:976644-977267) gene. Moreover, the HUB11505 and HUB12640 strains also acquired the tet(B) gene (NC_015964:1166619-1167824).
Phylogenetic analysis involved the 35 H. parainfluenzae genomes that were available on the NCBI database, including the H. parainfluenzae strain T3T1, which has a fully closed genome and was used as a reference strain for the phylogenetic analysis (Fig. 1). Overall, high intraspecies diversity was found, with an estimated core genome of around 42% and a total of 163,337 single nucleotide variants (SNVs). Despite this genetic diversity, the H. parainfluenzae strains isolated in this study were closely related (80% core genome and 30,955 SNVs) to an XDR strain from Switzerland (AE-2096513)16. Strains HUB12345 and HUB12445, isolated from a single patient, were genetically indistinguishable
New capsular operon related to that of H. influenzae serotype c
A similar capsular operon was detected in all the strains, with a total length of 14,678 bp and 10 predicted ORFs. However, the capsular operon of HUB11505 presented a pcsB gene that was truncated at nucleotide position 5,613 by the insertion of an IS4 family transposase ISVsa5 previously identified in Haemophilus ducreyi (NZ_CP015434.1:125637-126845).
Figure 2 describes the genetic composition of the six H. influenzae and H. parainfluenzae capsular operons. A new name has been designated to each gene from the variable region II in H. parainfluenzae: pcsABCD. Regions I and III from serotypes c and d were not available on the NCBI database and hence, those genes were not included in the analysis. Supplementary Table 1 present the identity between each gene/protein from H. parainfluenzae and from the H. influenzae serotypes available on the NCBI database. Region I was the most conserved among the serotypes, with a high protein identity (>90%). Region III was also conserved, but the protein identity was lower than that of region I. The serotype-specific proteins from region II showed no identity with the new capsular operon, except for the genes fcsA (serotype f), ccsA, ccsC and ccsD (serotype c). Although ccsD and pcsD presented high identity, ccsD from the NCBI database (HQ651151) had a 1-bp deletion at position 34 that resulted in a truncated protein.
Visualisation of capsular polysaccharides
Capsular polysaccharides were visually examined under the TEM, using H. influenzae serotype b and non-encapsulated H. parainfluenzae (bexA-negative) as controls. Cellular visualisation (Fig. 3) revealed that the non-encapsulated H. parainfluenzae was surrounded by a defined bacterial cell membrane, which was significantly thinner than that of the encapsulated H. influenzae serotype b and the H. parainfluenzae strain HUB12445. Strain HUB11505, with a truncated pcsB gene, was also surrounded by a diffuse structure that could be classified as an intermediate between that of the encapsulated H. influenzae serotype b and the non-encapsulated H. parainfluenzae.
H. parainfluenzae is a human commensal responsible for a large range of human infections, including genitourinary infections. The putative role of this pathogen in STDs is a cause for concern. In this paper, we describe for first time the capsular operon of four XDR H. parainfluenzae clinical isolates from three patients with urogenital infections, two males presenting urethritis and a female with vaginal discharge due to intra uterine device implantation.
The accumulation of many resistance mechanisms to several antimicrobial agents (ß-lactams, chloramphenicol, macrolides, quinolones, tetracycline and co-trimoxazole) leaves few available therapeutic options. Although β-lactam resistance is mainly due to the presence of β-lactamases19,20, the resistance in our strains was only associated with amino acid substitutions in the PBP3. These changes have been previously described in an H. parainfluenzae clinical isolate classified as a β-lactamase-negative ampicillin-resistant isolate (gBLNAR) from the III-like group13. Strain HUB11505 was susceptible to amoxicillin/clavulanic acid and ceftriaxone, possible due to the absence of substitutions K276N, A307N and V329I, which have already been reported16, but not conclusively proven to confer resistance to β-lactams. The analysis of the quinolone resistance-determining region (QRDR) of gyrA, parC and parE also revealed mutations that have been previously described21. The substitutions in DNA gyrase (S84F and D88Y) have been reported to be essential in the interaction between DNA and fluoroquinolones in H. influenzae22. Both substitutions, together with S84F in ParC, are the most common changes associated with fluoroquinolone resistance in Gram-negative bacteria. The ParC substitutions S84F and D420N, together with A451S in ParE have also been linked to high-level fluoroquinolone resistance in H. parainfluenzae, but their involvement in resistance has not been demonstrated15. The substitutions S138T and M198L have also been previously described8 outside the QRDR region in ParC, which might be involved with fluoroquinolone resistance14. Although the substitution A69S in the L4 protein has already been found in macrolide-resistant isolates23, a recent report also identified this mutation in susceptible strains, suggesting that it alone might not confer resistance to macrolides14. However, the decrease in susceptibility could also be explained by the presence of the macrolide efflux genetic assembly (MEGA) element, which is present in different bacteria and was found for the first time in an H. parainfluenzae isolate reported in 2013 in Switzerland18. This element contains the mel and mef(E) genes, which encode a dual efflux pump that confers resistance to 14- and 15-membered lactone ring macrolides. Related to co-trimoxazole resistance, the I95L substitution in dihydrofolate reductase (DHFR) has been proposed to be involved in resistance24 and could be a homologue for the I100L substitution found in S. pneumoniae25. However, only two of the strains investigated in this study presented this change, suggesting that additional mechanisms might contribute to this resistance. Finally, all the strains presented catS, an acquired mechanism of resistance to chloramphenicol from H. ducreyi, suggesting the possible horizontal transfer of genetic material between strains from different species.
As observed in Fig. 1, H. parainfluenzae presents high intraspecies diversity with a low percentage of core genome and a high number of SNVs, in accordance with previous epidemiological studies performed by PFGE in our hospital (data not shown). The high genome plasticity in this species facilitates the exchange of genetic material with other microorganisms, enabling this species to act as a genetic reservoir of antimicrobial resistance. The strains isolated in this study shared a high percentage of core genome with the Swiss strain AE-2096513, also presenting very similar antimicrobial resistance profiles that differed mainly in co-trimoxazole resistance. Interestingly, AE-2096513 was most closely related to HUB11505 and HUB12640, suggesting the spread of this resistant clone in Europe possibly via sexual transmission. Further epidemiological studies are needed to verify the spread of these XDR H. parainfluenzae clones.
We identified and characterised a complete capsular operon for the first time in H. parainfluenzae. Since the capsule is one of the most important virulence factors in H. influenzae, this is a remarkable fact to consider in the surveillance of multidrug-resistant bacterial pathogens. Comparing the predicted genetic structure of the operons, the capsule identified in H. parainfluenzae presented the highest identity with that of H. influenzae serotype c, which is the least common serotype in this species. The high similarity between their capsules suggests that they might have a common ancestor. AE-2096513 was the only strain out of all those available in the NCBI database that presented a completely identical capsular operon to that of our clinical isolates, which was in accordance with the results of the phylogenetic analysis. Capsule visualisation by TEM indicated that the HUB12445 strain had a similar structure to that of encapsulated H. influenzae b, in agreement with previous visualisations of the capsule by TEM26 and proving that the capsular operon was expressed in H. parainfluenzae. HUB11505, whose pcsB gene was interrupted by a transposase, also presented a capsule, but it was morphologically different to the capsule of HUB12445, suggesting that the alternative ORF shown in Fig. 2 encoded a functional protein that modified the polysaccharide composition of the capsule.
In conclusion, this study describes for the first time a capsular operon in H. parainfluenzae. The accumulation of resistance mechanisms leaves few therapeutic options in the treatment of these infections. Furthermore, phylogenetic analysis indicates a possible spread of this XDR clone in Europe that could be through sexual transmission.
Characterisation of the bacterial strains
Four XDR H. parainfluenzae strains were isolated from the urogenital exudates of three patients between January 2016 and January 2017: two males with urethritis and one female with pelvic inflammatory disease linked to an intrauterine device implantation (Table 1).
One of the male patients presented a positive PCR for Chlamydia trachomatis, but was negative for Neisseria gonorrhoeae. For the other male, no appropriate samples for PCR detection were collected, with only H. parainfluenzae being detected by microbiological culture. The female patient had pelvic inflammatory disease, with H. parainfluenzae isolated from both vaginal and endocervical exudates. PCR detection of C. trachomatis and N. gonorrhoeae gave negative results. Gardnerella vaginalis was also isolated from the endocervical exudate.
Clinical isolates were identified as H. parainfluenzae by MALDI-TOF mass spectrometry (Bruker Daltonik GmbH, Bremen, Germany). The strains used in this study were routinely grown in chocolate agar plates (bioMérieux, Marcy l’Etoile, France) or Haemophilus test medium (HTM) broth (Thermo Fisher Scientific, Massachusetts, USA) and incubated at 37 °C with 5%CO2. These strains produced smooth but non-mucoid greyish colonies on chocolate agar plates.
The minimum inhibitory concentration (MIC) was determined by microdilution using commercial panels (STRHAE2; Sensititre, Thermo Fisher Scientific) and interpreted following the guidelines of the European Committee on Antimicrobial Susceptibility Testing (EUCAST)27. β-lactamase activity was tested using the chromogenic cephalosporin method (nitrocefin disks, BD, New Jersey, USA).
Whole-genome sequencing and genome analysis
DNA was extracted using QIAamp DNA Blood Mini Kit (Qiagen, Hilden, Germany) and quantified using the QuantiFluor® dsDNA System (Promega, Wisconsin, USA). Nextera XT was used to prepare the libraries, followed by paired-end sequencing (2 × 150 bp) on an Illumina MiSeq Platform (Illumina Inc., San Diego, CA, USA), following the manufacturer’s instructions. The INNUca v2.6 pipeline (https://github.com/B-UMMI/INNUca) was used for read quality assessment, improvement and genome assembly. Briefly, quality control of the reads was performed using FastQC (http://www.bioinformatics.babraham.ac.uk/projects/fastqc/) and the reads were cleaned and improved with Trimmomatic28. The genome was assembled using SPAdes v3.1029 and subsequently polished. QA/QC statistics, genome depth of coverage and the number of contigs were monitored and reported throughout the analysis. All generated reads were deposited in the European Nucleotide Archive (accession numbers: HUB11505:ERS2616278, HUB12435:ERS2616279, HUB12445:ERS2616280 and HUB12640:ERS2616281).
An in silico screening of mutations targeting genes involved in antibiotic resistance was performed with Geneious R9 (Biomatters, Auckland, New Zealand), using the closed genome of the H. parainfluenzae strain T3T1 (NC_015964) as reference. A screening of the acquired resistance genes was conducted using the Comprehensive Antibiotic Resistance Database (CARD)30, ARG-ANNOT31 and ResFinder 3.032.
Phylogenetic analysis was performed by constructing an assembly-based core-SNV phylogenetic tree including the 35 H. parainfluenzae genomes available on the NCBI database and using the T3T1 strain as reference. Parsnp from the Harvest suite33 was used with default parameters, with the exception of parameter -C, which was adjusted to 5,000 to maximise the reference coverage. Phylogenetic tree visualisation was achieved with the graphic viewer FigTree (http://tree.bio.ed.ac.uk/software/figtree/).
Capsular operon determination
The capsular operons of H. influenzae serotype a (CP017811:1472186-1485236), serotype b (NC_016809:1190909-1206625), serotype c (HQ651151), serotype d (HM770877), serotype e (FM882247) and serotype f (CP005967:675016-687441) were used for a BLASTn search with Geneious R9 against our four assembled genomes and the open reading frames (ORF) were predicted. The percentage of identity between gene/proteins from H. parainfluenzae and that of the six capsular operons from H. influenzae was calculated as the identical number of bases/residues divided by the length of the longest gene/protein (Supplementary Table 1).
Since the capsular operon of the HUB11505 strain could not be resolved through whole-genome sequencing (WGS) data, we designed the primers 11505_F (5′-GGTTCTACCGACTCGTCTGC-3′) and 11505_R (5′-AGCATCTTCTTGTTTGATATATGCCG-3′) to close the gap by PCR amplification, followed by Sanger sequencing through primer walking, using primers 11505_F and 11505_F2 (5′-GTTCTCGCCTTTGGTTGGCAG-3′). The capsular operon of the H. parainfluenzae strain HUB12445 was deposited in the NCBI database with accession number MH644108.
Transmission electron microscopy for capsule visualisation
Four strains were selected to visualise the presence of the capsule: (a) H. influenzae strain HUB13399 serotype b as a positive control; (b) non-encapsulated H. parainfluenzae strain HUB13327 as a negative control; (c) H. parainfluenzae strains HUB12445 (full ccsB gene); and (d) H. parainfluenzae strain HUB11505 (ccsB gene interrupted by a transposase). Samples were fixed following the lysine-acetate-based formaldehyde-glutaraldehyde ruthenium red-osmium fixation procedure (LRR fixation), as previously described34. Strains were grown overnight in HTM broth and centrifuged for 10 min at 1,800 g. Cells were then fixed, dehydrated, impregnated in resin and finally polymerised, as described for H. influenzae26. Ultra-thin sections were stained with 2% uranyl acetate, counterstained with lead citrate and visualised under JEOL 1010 Transmission Electron Microscope (TEM) operated at 80 kV and equipped with a Orius camera (Gatan, Inc.).
This study has been revised and approved for its publication by the Clinical Research Ethics Committee of the Hospital de Bellvitge (PR324/18). Written informed consent was not required as this is a retrospective and observational study with isolates obtained as part of the normal microbiological routine. Patient confidentiality was always protected; all the data were anonymized and protected according to national normative.
Nørskov-Lauritsen, N. Classification, identification, and clinical significance of Haemophilus and Aggregatibacter species with host specificity for humans. Clin. Microbiol. Rev. 27, 214–240 (2014).
Murray, P. R. & Baron, E. J. American Society for Microbiology. Manual of clinical microbiology. (ASM Press, 2003).
Kosikowska, U., Biernasiuk, A., Rybojad, P., Łoś, R. & Malm, A. Haemophilus parainfluenzae as a marker of the upper respiratory tract microbiota changes under the influence of preoperative prophylaxis with or without postoperative treatment in patients with lung cancer. BMC Microbiol. 16, 1–9 (2016).
Cardines, R. et al. Haemophilus parainfluenzae meningitis in an adult associated with acute otitis media. New Microbiol. 32, 213–215 (2009).
Latyshev, Y., Mathew, A., Jacobson, J. M. & Sturm, E. Purulent pericarditis caused by Haemophilus parainfluenzae. Tex. Heart Inst. J. 40, 608–11 (2013).
O’Neil, C. R., Wilson, E. & Missaghi, B. Bone and Joint Infections due to Haemophilus parainfluenzae: Case Report and Review of the Literature. Can. J. Infect. Dis. Med. Microbiol. 2016, 1–6 (2016).
Hong, M. J., Kim, Y. D. & Ham, H. Do. Acute septic arthritis of the acromioclavicular joint caused by Haemophilus parainfluenzae: a rare causative origin. Clin. Rheumatol. 34, 811–814 (2015).
Cardines, R. et al. Genital carriage of the genus Haemophilus in pregnancy: Species distribution and antibiotic susceptibility. J. Med. Microbiol. 64, 724–730 (2015).
Hsu, M. S., Wu, M. Y., Lin, T. H. & Liao, C. H. Haemophilus parainfluenzae urethritis among homosexual men. J. Microbiol. Immunol. Infect. 48, 450–452 (2015).
Deza, G. et al. Isolation of Haemophilus influenzae and Haemophilus parainfluenzae in urethral exudates from men with acute urethritis: A descriptive study of 52 cases. Sex. Transm. Infect. 92, 29–31 (2016).
Hansson, S., Svedhem, Å., Wennerström, M. & Jodal, U. Urinary tract infection caused by Haemophilus influenzae and Haemophilus parainfluenzae in children. Pediatr. Nephrol. 22, 1321–1325 (2007).
Satola, S. W., Schirmer, P. L. & Farley, M. M. Complete sequence of the cap locus of Haemophilus influenzae serotype b and nonencapsulated b capsule-negative variants. Infect. Immun. 71, 3639–3644 (2003).
García-cobos, S. et al. Novel mechanisms of resistance to β-lactam antibiotics in Haemophilus parainfluenzae: β-lactamase-negative ampicillin resistance and inhibitor-resistant TEM β-lactamases. J. Antimicrob. Chemother. 68, 1054–1059 (2013).
Abotsi, R. E., Govinden, U., Moodley, K. & Essack, S. Fluoroquinolone, Macrolide, and Ketolide Resistance in Haemophilus parainfluenzae from South Africa. Microb. Drug Resist. 23, 667–673 (2017).
Rodríguez-Martínez, J. M., López-Hernández, I. & Pascual, Á. Molecular characterization of high-level fluoroquinolone resistance in a clinical isolate of Haemophilus parainfluenzae. J. Antimicrob. Chemother. 66, 673–675 (2011).
Tinguely, R. et al. Emergence of extensively drug-resistant Haemophilus parainfluenzae in Switzerland. Antimicrob. Agents Chemother. 57, 2867–2869 (2013).
Magiorakos, A. P. et al. Multidrug-resistant, extensively drug-resistant and pandrug-resistant bacteria: An international expert proposal for interim standard definitions for acquired resistance. Clin. Microbiol. Infect. 18, 268–281 (2012).
Endimiani, A., Allemann, A., Wüthrich, D., Lupo, A. & Hilty, M. First report of the macrolide efflux genetic assembly (MEGA) element in Haemophilus parainfluenzae. Int. J. Antimicrob. Agents 49, 265–266 (2017).
Faccone, D. et al. Molecular characterization of a clinical Haemophilus parainfluenzae isolate with cefotaxime resistance and decreased susceptibility to fluoroquinolones. Infect. Genet. Evol. 44, 507–509 (2016).
Tristram, S. G. et al. Characterization of extended-spectrum β-lactamase-producing isolates of Haemophilus parainfluenzae. J. Antimicrob. Chemother. 61, 509–514 (2008).
Law, D. K. S., Shuel, M., Bekal, S., Bryce, E. & Tsang, R. S. W. Genetic detection of quinolone resistance in Haemophilus parainfluenzae: Mutations in the quinolone resistance-determining regions of gyrA and parC. Can. J. Infect. Dis. Med. Microbiol. 21, 20–22 (2010).
Georgiou, M. et al. Ciprofloxacin-resistant Haemophilus influenzae strains possess mutations in analogous positions of GyrA and ParC. Antimicrob. Agents Chemother. 40, 1741–1744 (1996).
Peric, M., Bozdogan, B., Jacobs, M. R. & Appelbaum, P. C. Effects of an efflux mechanism and ribosomal mutations on macrolide susceptibility of Haemophilus influenzae clinical isolates. Antimicrob. Agents Chemother. 47, 1017–1022 (2003).
de Groot, R. et al. Genetic characterization of trimethoprim resistance in Haemophilus influenzae. Antimicrob. Agents Chemother. 40, 2131–6 (1996).
Varaldo, P. E., Montanari, M. P. & Giovanetti, E. Genetic elements responsible for erythromycin resistance in streptococci. Antimicrob. Agents Chemother. 53, 343–353 (2009).
Schouls, L. et al. Two variants among Haemophilus influenzae serotype b strains with distinct bcs4, hcsA and hcsB genes display differences in expression of the polysaccharide capsule. BMC Microbiol. 8, 1–11 (2008).
The European Committee on Antimicrobial Susceptibility Testing. Clinical breakpoints. European Society of Clinical Microbiology and Infectious Diseases (EUCAST) Basel, Switzerland. Available at, http://www.eucast.org/clinical_breakpoints/ (2018).
Bolger, A. M., Lohse, M. & Usadel, B. Trimmomatic: A flexible trimmer for Illumina sequence data. Bioinformatics 30, 2114–2120 (2014).
Bankevich, A. et al. SPAdes: A New Genome Assembly Algorithm and Its Applications to Single-Cell Sequencing. J. Comput. Biol. 19, 455–477 (2012).
Jia, B. et al. CARD 2017: Expansion and model-centric curation of the comprehensive antibiotic resistance database. Nucleic Acids Res. 45, D566–D573 (2017).
Gupta, S. K. et al. ARG-annot, a new bioinformatic tool to discover antibiotic resistance genes in bacterial genomes. Antimicrob. Agents Chemother. 58, 212–220 (2014).
Zankari, E. et al. Identification of acquired antimicrobial resistance genes. J. Antimicrob. Chemother. 67, 2640–2644 (2012).
Treangen, T. J., Ondov, B. D., Koren, S. & Phillippy, A. M. The harvest suite for rapid core-genome alignment and visualization of thousands of intraspecific microbial genomes. Genome Biol. 15, 1–15 (2014).
Hammerschmidt, S. et al. Illustration of Pneumococcal Polysaccharide Capsule during Adherence and Invasion of Epithelial Cells. Infect. Immun. 73, 4653–4667 (2005).
We wish to thank the staff of the Microbiology Laboratory of Bellvitge University Hospital who contributed to this project on a daily basis, and to Centres Científics i Tecnològics (Campus Hospital Clinic, Universitat de Barcelona, Spain) for their technical assistance in Transmission Electron Microscopy. This study has been funded by Instituto de Salud Carlos III through the Projects from the Fondo de Investigaciones Sanitarias “PI16/00977” and CIBER de Enfermedades Respiratorias (CIBERES - CB06/06/0037), and Co-funded by the European Regional Development Fund/European Social Fund (ERDF/ESF, “Investing in your future”).
The authors declare no competing interests.
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
González-Díaz, A., Tubau, F., Pinto, M. et al. Identification of polysaccharide capsules among extensively drug-resistant genitourinary Haemophilus parainfluenzae isolates. Sci Rep 9, 4481 (2019). https://doi.org/10.1038/s41598-019-40812-2