Bloodstream infections by Salmonella enterica serovar Typhimurium constitute a major health burden in sub-Saharan Africa (SSA). These invasive non-typhoidal (iNTS) infections are dominated by isolates of the antibiotic resistance-associated sequence type (ST) 313. Here, we report emergence of ST313 sublineage II.1 in the Democratic Republic of the Congo. Sublineage II.1 exhibits extensive drug resistance, involving a combination of multidrug resistance, extended spectrum β-lactamase production and azithromycin resistance. ST313 lineage II.1 isolates harbour an IncHI2 plasmid we name pSTm-ST313-II.1, with one isolate also exhibiting decreased ciprofloxacin susceptibility. Whole genome sequencing reveals that ST313 II.1 isolates have accumulated genetic signatures potentially associated with altered pathogenicity and host adaptation, related to changes observed in biofilm formation and metabolic capacity. Sublineage II.1 emerged at the beginning of the 21st century and is involved in on-going outbreaks. Our data provide evidence of further evolution within the ST313 clade associated with iNTS in SSA.
Salmonella enterica subspecies enterica serovar Typhimurium (S. Typhimurium) and other non-typhoidal Salmonella are common causes of gastrointestinal infections in people living in industrialized countries. However, in sub-Saharan Africa (SSA), invasive non-typhoidal Salmonella (iNTS) bloodstream infections are common1,2 totalling ~3.4 million cases annually, with S. Typhimurium being responsible for approximately two-thirds of these cases. The fatality rate in iNTS can be extremely high3.
In SSA, iNTS patients often do not suffer from diarrhoea but instead display symptoms of fever and septicaemia4. There has been no proven zoonotic source of ST313 infections, and human to human transmission has been postulated5,6. The disease disproportionately affects children under 5-years old and human immunodeficiency virus (HIV) positive adults7.
Whereas the majority of S. Typhimurium associated with gastroenteritis in developed countries belong to sequence types (ST) 19 and 34, S. Typhimurium iNTS in SSA are predominantly of ST3138. The population structure of S. Typhimurium ST313 is dominated by two clonal lineages, named I and II, that sequentially spread across SSA over the past 40 years. The success of these ongoing pandemics has been attributed to resistance to antibiotics and the emergence of HIV9. The majority of iNTS S. Typhimurium isolated in the past 10 years have been of ST313 lineage II10,11,12.
S. Typhimurium ST313 isolates are predominantly multidrug resistant (MDR), implying co-resistance to the three former first line antibiotics ampicillin, trimethoprim/sulfamethoxazole and chloramphenicol13,14. Two recent genomics-based studies reported the acquisition of extended-spectrum β-lactamases (ESBLs) conferring resistance to the third generation cephalosporin ceftriaxone among S. Typhimurium ST313 lineage II isolates from Malawi and Kenya10,11. Ceftriaxone is a recommended antibiotic to treat complicated iNTS, while the fluoroquinolone ciprofloxacin is recommended for uncomplicated iNTS15.
The genomes of S. Typhimurium ST313 show evidence of specialization towards a narrow host range by pseudogenization in a pattern that resembles that found in the host restricted typhoidal Salmonella enterica subspecies enterica serovar Typhi (S. Typhi)4,16,17. The genotypic differences between ST313 and ST19 isolates have been confirmed as phenotypes associated with host virulence and other traits, including biofilm formation which has been postulated to influence both survival in the environment and macrophages9,18,19,20,21,22.
Here, we report the emergence of an extensively drug resistant (XDR) ST313 sublineage we name II.1, which is currently causing bloodstream infections in the Democratic Republic of the Congo (DRC) and represents >10 % of all S. Typhimurium isolated in the Kongo Central Province14. This sublineage is associated with a combination of MDR, ESBL production and resistance to azithromycin (AZI). Additionally, whole-genome sequencing of multiple genomes identifies signatures associated with pathogenicity, metabolism and potentially host adaptation.
An XDR S. Typhimurium ST313 sublineage II.1 is emerging
Invasive S. Typhimurium have been isolated in various hospital sites across DRC during ongoing microbial surveillance of bacterial bloodstream infections14,23,24. As third-generation cephalosporins and AZI have been used in treatment, we have monitored susceptibility using both phenotypic and genetic approaches. Consequently, to investigate the emerging phenotype of ESBL production and AZI resistance, a selection of 81 S. Typhimurium isolates from the region were subjected to whole-genome sequence analysis. Their year and place of origin, the age of the patient and their phenotypic antimicrobial susceptibility are listed in Supplementary Data 1. Of this panel, 54 S. Typhimurium isolates exhibited AZI resistance and were ESBL positive; all except three were also MDR and are thus classifiable as XDR. The isolates were collected from 2008 to 2016 in western (Kisantu, Kongo Central Province n = 50; Kinshasa n = 2) and north-eastern DRC (Kisangani, Tshopo Province: n = 2) (Fig. 1). Minimum inhibitory concentration (MIC) values for AZI resistance were between 32 and >256 mg L−1. Two of these isolates, 5390_4 (Kisangani, 2016) and 2735 (Kinshasa, 2008), showed decreased susceptibility to the fluoroquinolone ciprofloxacin (decreased ciprofloxacin susceptibility (DCS), MIC values of 0.38 and 0.19 mg L−1against ciprofloxacin, respectively). These isolates also exhibited resistance to the quinolone pefloxacin, and susceptibility (5390_4) or resistance (2735) to the quinolone nalidixic acid. The other 27 S. Typhimurium isolates form a representative local context, originating from bloodstream infections in the same surveillance sites in DRC (see Supplementary Note 1). They were isolated between 2007 and 2016, and showed no ESBL production nor resistance to AZI. The majority of these isolates (22 out of 27) were MDR. One isolate, 16755_3 (Kisantu, 2016), exhibited DCS with a MIC value of 0.19 mg L−1.
Multilocus sequence typing (MLST) confirmed that all belong to ST313. To provide context for the genomic analysis, 153 African9,11,12,25,26 and 42 non-African9 S. Typhimurium genomes were included in the overall analysis. The complete list of 276 analysed S. Typhimurium genomes with the year, place and source of isolation is presented in Supplementary Data 2.
This analysis revealed a sublineage II.1 in DRC defined by the most recent common ancestor of the monophyletic sublineage of 51 XDR isolates (Fig. 2a). One isolate, 5390_4, originating from Kisangani (2016) while being MDR, ESBL producing, AZI resistant and showing DCS, falls outside sublineage II.1, but is part of the clonal lineage II. All 27 control isolates also fall into lineage II, with two older isolates from Kisantu (2009) being most closely related to sublineage II.1 (1577 and 1582).
The S. Typhimurium ST313 lineage I and II in our study accumulated 225 and 216 conserved single nucleotide polymorphisms (SNPs) respectively in their core genomes compared to their most recent common ancestor (Supplementary Fig. 1), which is comparable to previous observations17. In comparison to the lineage II clade, all sublineage II.1 isolates, except 2735, accumulated an additional 38 conserved core SNPs, and show a clonal structure with little substructure (Fig. 2b). Of note, the two isolates showing an AZI MIC value >256 mg L−1 form a monophyletic clade within sublineage II.1 (17399_3 and 17568_3). No SNPs were acquired in known genes involved in macrolide resistance27, but both isolates have a G118V amino acid substitution in the ABC-transporter protein BtuC. This SNP, in addition to the presence of mphA, might be involved in the observed increased AZI resistance28. Cephalosporin resistant ST313 lineage II infections were previously reported from Kenya and Malawi10,11,12. The XDR isolates we describe here form ST313 sublineage II.1.
The putative origin of the ST313 lineage II was previously predicted to be the DRC9. Consequently, we applied a temporal reconstruction using BEAST2 to the S. Typhimurium ST313 lineage II and II.1 isolates. This limited analysis indicates that sublineage II.1 may have emerged in the DRC around 2004 (95% highest probability density (HPD) interval: 2000–2007) (Fig. 3).
Lineage II.1 harbours an IncHI2 resistance plasmid, pSTm-ST313-II.1
A comprehensive resistome, composed of all catalogued genetic determinants for antimicrobial resistance (AMR), was bioinformatically extracted from the sequencing data (Supplementary Data 2). This analysis indicates that the MDR phenotype observed in S. Typhimurium ST313 lineage II and sublineage II.1 isolates is associated with genes predicted to confer resistance to chloramphenicol (catA), ampicillin (blaTEM1) and trimethoprim (dfrA). While lineage II is linked to the presence of dfrA1, this allele is replaced by dfrA14 in sublineage II.1. XDR sublineage II.1 isolates harbour blaSHV-2A and mphA genes, respectively potentially associated with resistance to cephalosporins and azithromycin, respectively. Identical blaSHV-2A and mphA genes are present in the ESBL positive, AZI resistant lineage II isolate from Kisangani (5390_4). One sublineage II.1 isolate, 2735, showed DCS (MIC value ciprofloxacin = 0.19 g L−1) in addition to AZI resistance and ESBL production and harbours a mutation in gyrA (D87N) associated with DCS. DCS combined with ESBL positivity and AZI resistance was also observed in the lineage II isolate 5390_4 (Kisangani, 2016, MIC value ciprofloxacin = 0.38 g L−1), which has acquired a qnrS gene. The lineage II isolate 16755_3 (Kisantu, 2016, MIC value ciprofloxacin = 0.19 g L−1) showed DCS but no ESBL activity nor AZI resistance and harbours a S83Y mutation in gyrA.
All sublineage II.1 isolates as well as the lineage II 5390_4 isolate (ESBL + AZI) from Kisangani harbour an IncHI2 plasmid. IncHI2 plasmids have been reported previously in other S. Typhimurium ST313 isolates from Kenya (pKST313) and Malawi (pSTm-A54650)10,11. We have named the ST313 sublineage II.1 IncHI2 plasmid pSTm-ST313-II.1. The full pSTm-ST313-II.1 plasmid sequence associated with sublineage II.1 was determined using PacBio sequencing of isolate 10433_3 (Kisantu, 2014). pSTm-ST313-II.1 is 274,695 nucleotides (Fig. 4) and is highly conserved among all sublineage II.1 isolates, differing by ~5 single SNPs between isolates. The known AMR determinants of ST313 sublineage II.1 are located on pSTm-ST313-II.1, alongside genes associated with heavy metal resistance against silver and copper. pSTm-ST313-II.1 encodes a potentially active TraB conjugation protein and conjugation operon29.
pSTm-ST313-II.1 exhibits significant similarity to R478 (99% identity over 86% coverage of pSTm-ST313-II.1), a self-transferable IncHI2 plasmid isolated from Serratia marcescens in 1969 in the USA30. Pairwise sequence comparisons of pSTm-ST313-II.1 with the other IncHI2 plasmids (1) pKST313 from Kenya, (2) pSTm-A54650 from Malawi, a (3) draft assembly from the IncHI2 plasmid of 5390_4 from Kisangani, and R478 revealed the significant similarity between the plasmid backbones (Fig. 4 and Supplementary Table 1). The less conserved regions of pSTm-ST313-II.1 include AMR genes, flanked by transposon-associated regions (Fig. 4).
Sublineage II.1 exhibits signatures of host adaptation
ST313 sublineage II.1 harbours multiple chromosomal sequence differences in comparison to ST313 lineage II isolates (Fig. 5). A deletion of 1076 nt was observed in the chromosome of ST313 sublineage II.1, resulting in loss of fljB. The fljB gene codes for the phase 2 flagellin protein which polymerizes to form the bacterial flagella (Supplementary Fig. 2). Loss of fljB (FljB) was confirmed at the DNA and protein levels (Supplementary Fig. 3). Consequently, in contrast to their biphasic ancestors, sublineage II.1 isolates are monophasic as they only harbour the phase 1 flagellin gene, fliC.
We annotated the SNPs that were acquired in ST313 sublineage II.1 relative to lineage II (Supplementary Tables 2–4). Of these SNPs, 19 are present in coding regions and cause predicted non-synonymous mutations in the protein sequence (Supplementary Tables 2–4). Seven of these 19 SNPs are located in conserved Pfam protein domains resulting in deviant bitscores. Consequently, we prioritized these SNPs as the most likely to cause functional defects. The affected genes are geranyltranstransferase ispA, methyl-accepting chemotaxis protein trg_1, precorrin-3B C17-methyltransferase cbiH, propanediol dehydratase reactivation protein, outer membrane assembly protein asmA, putative multidrug export ATP-binding/permease protein SAV1866 and putative diguanylate cyclase yhjK. These genes have been linked to host-adaptation (cbiH)16, virulence-associated processes (asmA)31, and chemotaxis during infection (trg_1)32. Of note, these molecular processes are also linked to pseudogene accumulation in the phylogeny from S. Typhimurium ST19 to ST313 lineage II17.
As our interpretations are likely biased by the available literature, we applied a data mining approach to obtain a more objective evaluation of the association between the acquired SNPs in sublineage II.1 and invasiveness. Hereto, the Salmonella invasiveness index of each strain was calculated, which is based on the genomic signatures for S. enterica associated with adaptation to an invasive lifestyle33. We observe an increase in invasiveness index from non-ST313 and ST313 lineage I isolates to lineage II, and a significant further increase of the invasiveness index from lineage II to lineage II.1 (Fig. 6a, Supplementary Fig. 3).
In addition to the observed genomic differences, S. Typhimurium ST313 sublineage II.1 isolates exhibited measurably different phenotypes compared to S. Typhimurium ST313 lineage II. A red dry and rough (rdar) biofilm assay was performed that uses agar plates with stains that reveal extracellular matrix production in colonies. In this assay, S. Typhimurium ST313 lineage II isolates lost the rough morphotype compared to ST19, changing from a rdar to a brown and smooth (bas) phenotype. This phenotype was shown previously to be due to defective production of cellulose, one of the two major extracellular components of Salmonella biofilms18,20. Interestingly, S. Typhimurium ST313 lineage II.1 show a further defect in biofilm formation. Sublineage II.1 isolates have a smooth and white (saw) colony morphotype in this assay, whereas sublineage II isolates have a brown and smooth (bas) morphotype (Fig. 6b). This phenotypic defect is consistent across all isolates from sublineage II.1 and resembles the S. Typhi morphotype. The exception was isolate 2735 (Kinshasa, 2008), the phylogenetically oldest representative of sublineage II.1 (Supplementary Fig. 4)19. Among the SNPs that were acquired in sublineage II.1 compared to lineage II, none were located in or near genes responsible for the production of curli, which is another major biofilm compound. Mutagenesis experiments showed that the introduction of a null mutation into the asmA gene of S. Typhimurium ST313 lineage II D23580 partly recreated the sublineage II.1 biofilm phenotype (Fig. 6b), suggesting that the non-synonymous SNP in asmA might contribute to the biofilm defect. asmA encodes an outer membrane protein that was previously described to be involved in the invasion of epithelial cells31. Targeted mutations in wzxC, yhjJ and yhjK in D23580 had no obvious effect on the biofilm phenotype (Supplementary Fig. 5).
While Salmonella causing gastrointestinal infections typically have a relatively large metabolic capacity, strains causing invasive infections generally have a more limited capacity34. We used Biolog Phenotype Microarrays to assess growth on 192 different metabolic compounds between two representative isolates of both lineage II and lineage II.1. Lineage II.1 isolates showed significant lower metabolic capacity for carbon compounds compared to lineage II isolates (Supplementary Data 3). The effect was most pronounced for D-galactonic acid γ-lacton (Supplementary Fig. 6).
We also assessed the phenotypic behaviour of five representative sublineage II.1 isolates in in vitro and in vivo models. Human macrophage infections and intravenous and oral mouse infections did not show significant differences between the lineages, although two sublineage II.1 isolates showed an overall lower infection of THP macrophages and cell counts in mouse deep tissue after intravenous infections (Supplementary Figs. 7–9).
Here, we report the emergence of S. Typhimurium ST313 sublineage II.1 from the DRC showing XDR. The World Health Organization (WHO) has listed Salmonella spp. as one of the pathogens for which new antibiotics are urgently needed35. In addition to the MDR phenotype of lineage II9, sublineage II.1 is associated with ESBL activity, AZI resistance and occasional DCS, thereby giving rise to the first lineage of XDR iNTS. As there is no XDR definition for iNTS yet, we extrapolate the definition from XDR S. Typhi, recently defined as resistant to five antibiotics (observed as MDR combined with resistance against fluoroquinolones and ESBL activity), thereby using the same nomenclature as for other bacterial pathogens36,37. The XDR iNTS isolates from this study show MDR in combination with resistance to the two alternative treatment options ceftriaxone and AZI.
Sublineage II.1 was identified in three independent surveillance sites in the DRC, suggesting this sublineage is relatively widespread in the region, although further surveillance is required to confirm the burden14,38,39,40.
All except three of the S. Typhimurium ST313 lineage II.1 isolates described here fall into the XDR category defined for S. Typhi36,37. Within the DRC setting, the only available antibiotics for treatment of XDR iNTS infections are fluoroquinolones. Importantly, DCS iNTS is present in DRC, with one pan-resistant (XDR + DCS) isolate identified in this study. The emergence of this XDR iNTS sublineage II.1 increases the urgency for advancements in other strategies, such as vaccination, to combat the disease.
Antibiotic use might have provided the selection pressure driving the emergence of this sublineage. Within SSA, the antibiotic AZI has been used in mass drug administrations for the elimination of Trachoma, and has also recently been tested to reduce childhood mortality41. In the DRC, it is not clear which antibiotics are in routine use, as only 30% of patients have access to the regular healthcare system, and 40% rely on self-medication42. MDR in ST313 sublineage II.1 is linked here with the IncHI2 plasmid pSTm-ST313-II.1. Intriguingly, previous reports have associated iNTS S. Typhimurium in SSA with IncHI2 plasmids10,11,43.
The acquisition of antibiotic resistance and the accumulation of genomic signatures associated with host adaptation by sublineage II.1 suggest further specialization to a human niche16,17. Sublineage II.1 are monophasic, a phenotype similar to typhoidal Salmonella44. A large recombination event took place at the fljB locus, resulting in loss of phase II flagellin production, while the phase I flagellin gene fliC remained intact. Bacterial flagellin plays an important role in the host innate immune response and is a stimulator of innate immunity through Tlr545,46. Strikingly, a pandemic of monophasic S. Typhimurium ST34 causing gastrointestinal infections has recently been identified, with some strains of this pandemic causing bloodstream infections in Vietnam47,48. Sublineage II.1 have a reduced capacity to form multicellular communities compared to lineage II18, again with similarity to S. Typhi19. Bacterial biofilms are important for both resistance to environmental stresses and survival outside the host. S. Typhimurium ST313 sublineage II.1 isolates also show a lower capacity for the metabolism of carbon sources, in line with the findings that S. Typhimurium ST313 has a reduced metabolic capacity compared to S. Typhimurium ST1917.
Survival in macrophages was experimentally assessed, given the observed mutations in sublineage II.1, such as loss of fljB, which can affect macrophage survival20. However, we did not find significant differences between lineage II and sublineage II.1 in macrophage infection assays. Likewise, II.1 isolates did not show a reproducible increased colonization of deeper tissue during intravenous or oral mouse infections. Although our genomic, biofilm and metabolic data show signatures for increased human adaption of lineage II, S. Typhimurium ST313 lineage II.1 isolates are thus far not host restricted.
In conclusion, in this study we identified an on-going outbreak of sublineage II.1 emerging from the current African S. Typhimurium ST313 pandemic. Sublineage II.1 is associated with XDR driven by an IncHI2 plasmid named pSTm-ST313-II.1, harbouring resistance to AZI and ESBL production. In addition, sublineage II.1 also shows evolutionary signatures associated with host adaptation. Extended bloodstream surveillance in the endemic regions of S. Typhimurium ST313 will be crucial to further track the spread of XDR ST313 sublineage II.1 and to timely detect the emergence of sublineages with novel antibiotic resistance profiles.
Isolate selection from bloodstream surveillance
The DRC isolates originated from blood cultures sampled at the referral hospital of Saint Luc in Kisantu (Kongo Central province), the University Hospital of Kinshasa, the referral Hospital St. Joseph and Monkole Hospital from Kinshasa (Kinshasa province), the referral hospital of Bwamanda (Tshopo province), the referral hospital of Kabondo and the university hospital of Kisangani (CUKIS) and associated health centres (Sud-Ubangi province) in the DRC14,24,40. These hospitals have participated in the microbiological surveillance network since 2007 coordinated by the National Institute of Biomedical Research (INRB) in Kinshasa, DRC, in collaboration with the Institute of Tropical Medicine (ITM) in Antwerp, Belgium. Blood cultures were sampled in patients suspected of bloodstream infections according to standard indications and methods as described elsewhere14.
All available AZI resistant S. Typhimurium available to this study were included (n = 54). A sample of 27 representative non-AZI resistant S. Typhimurium isolates were selected as controls for this analysis. Most health facilities across the country lack capacity for diagnosing bacterial bloodstream infections and we have therefore no information about bloodstream infections elsewhere in DRC except as part of outbreak research38,39. The surveillance sites included in this study were not consistently active because of stock ruptures, staff movements, funding and insecurity. All isolates were stored in tubes of Trypticase Soya Agar (Oxoid, Basingstoke, UK) and shipped to ITM for confirmation and further identification.
At ITM, isolates biochemically confirmed as Salmonella spp. were serotyped using commercial antisera (Sifin, Berlin, Germany) according to the Kauffmann-White scheme49. A representative selection of the isolates (10%) was sent to the National Reference Centre in Belgium for confirmation of serotype. Antibiotic susceptibility testing of all isolates was done by disk diffusion (Neo Sensitabs, Rosco, Taastrup, Denmark) according to the National Committee for Clinical Laboratory Standards (CLSI) guidelines; for ciprofloxacin and AZI, minimal inhibitory concentration (MIC-values) were determined with the E-test macromethod (bioMérieux). Interpretation of results was performed according to the most recent CLSI guideline50. Isolates with intermediate susceptibility were considered resistant. MDR was defined as co-resistance to all three first-line antibiotics ampicillin, chloramphenicol and trimethoprim-sulfamethoxazole15. ESBL production was assessed by double disk method according to CLSI guidelines50. For ciprofloxacin, the susceptibility breakpoint of ≤0.064 mg L−1 was used; the term decreased ciprofloxacin susceptibility was used to indicate MIC values >0.064 mg L−1 and <1 mg L−1, and ciprofloxacin resistance was reserved for MIC values ≥1 mg L−150. For AZI, isolates were considered resistant at MIC values ≥16 mg L−150. Ethical approval for the Microbiological Surveillance was granted by the Institutional Review Board at the ITM in Antwerp, by the Ethics Committees of the Antwerp University (Belgium) and the School of Public Health (Kinshasa, DRC).
Illumina and Pacbio whole-genome sequencing
DNA from all 81 strains was purified using the Gentra PureGene Yeast/Bact Kit (Qiagen, Hilden, Germany), following the manufacturer’s guidelines and DNA was sequenced on an Illumina HiSeq platform (Illumina, San Diego, USA). Illumina adapter content was removed from the reads using Trimmomatic v.0.3351. Public available Illumina sequencing data from 153S. Typhimurium strains originating from DRC, Mali, Nigeria, Uganda, Kenya, Malawi and Mozambique and a selection of 42 non-African genomes were included in the further genomics analysis9,10,11,12,26. This is a convenience sample including all publicly available African iNTS genomes. Strains are summarized in Supplementary Data 2.
A high-quality reference genome sequence of sublineage II.1 isolate 10433_3 was constructed using the PacBio RS II platform (PacBio, Menlo Park, CA, USA). The PacBio Template Prep Kit (PacBio, Menlo Park, CA, USA) and BluePippin™ Size Selection System protocol were used to prepare size-selected libraries (20 kb) from 5 μg of sheared and concentrated DNA. Sequencing was performed using the magnetic bead collection protocol, a 20,000 bp insert size, stage start, and 180-min movies. Sequence reads were assembled using HGAP v3 28 of the SMRT analysis software v2.3.0 (Pacbio, Menlo Park, CA, USA). The fold coverage to target when picking the minimum fragment length for assembly was set to 30 and the approximate genome size was set to 3 Mbp. The assembly was circularized using Circlator v1.1.352. Finally, the circularized assembly was polished using the PacBio RS_Resequencing protocol and Quiver v1 of the SMRT analysis software v2.3.053. Automated annotation was performed using PROKKA v1.1154 and genus specific databases from RefSeq55. The final assembled bacterial chromosome consisted of 4,877,289 bp, and two plasmid sequences of 274,695 bp and 94,649 bp.
Read mapping, variant detection, and phylogenetic analysis
Illumina HiSeq reads were mapped to the S. Typhimurium reference genomes of ST313 lineage II (D23580, FN424405.156) and ST313 sublineage II.1 (10433_3, ERZ1030005, this study) using SMALT v0.7.4 to produce a BAM file.
SMALT was used to index the reference using a kmer size of 20 and a step size of 13 and the reads were aligned using default parameters but with the maximum insert size set as 3 times the mean fragment size of the sequencing library. PCR duplicate reads were identified using Picard v1.92 (Broad Institute, Cambridge, MA, USA) and flagged as duplicates in the BAM file.
Variation detection was done using samtools mpileup v0.1.19 with parameters -d 1000 -DSugBf and bcftools v0.1.1957 to produce a BCF file of all variant sites, using the option to call genotypes at variant sites. The bcftools variant quality score was set to be greater than 50 (quality < 50), mapping quality was set to be greater than 30 (map_quality < 30), the allele frequency was required to be either 0 for bases called the same as the reference, or 1 for bases called as a SNP (af1 < 0.95), the majority base call was set to be present in minimal 75% of the reads mapping at the base (ratio < 0.75), the minimum mapping depth was four reads (depth < 4), at least two of these four had to map to each strand (depth_strand < 2), strand_bias was set to be less than 0.001, map_bias less than 0.001 and tail_bias less than 0.001. Otherwise, the base was called as uncertain and removed.
A pseudo-genome was constructed by substituting the base calls in the BCF file in the reference genome, uncertain sites were substituted with Ns. Insertions with respect to the reference genome were ignored, deletions were filled with N’s in the pseudo-genome.
Recombinant regions in the chromosome such as prophage regions and the fljB ORF in the chromosome were removed from the alignment and checked using Gubbins v1.4.1058. SNP sites were extracted from the alignment using snp-sites59 and used to construct a maximum likelihood phylogeny. RAxML v8.2.860 with substitution model GTRCAT. Support for nodes on the trees was assessed using 1000 bootstrap replicates. A comprehensive tree, with reads mapped to ST313 lineage II (D23580, FN424405.156) was rooted on S. Paratyphi A270 (ERR326600). Based on this tree, lineage II and sublineage II.1 isolates were identified and a high-resolution lineage II tree was constructed based on mapping to ST313 sublineage II.1 (10433_3, this study) and rooted to S. Typhimurium ST313 strain DT2. Trees were visualized using Figtree v1.4.2 and iTOL61. The comprehensive phylogenetic tree with spatiotemporal metadata, based on mapping against D23580 and rooted on S. Paratyphi A270 is made publicly available on MicroReact62 (https://microreact.org/project/xS5Xw6b3A).
Bayesian phylogenetic analysis
We used BEAST2 v2.4.863 to date evolutionary events, determine the substitution rate and produce a time-tree of African S. Typhimurium with tip-dates defined as the year of isolation (Supplementary Data 2). BEAUti xml’s were manually modified to specify the number of invariant sites in the genome. We employed a general time reversible (GTR) substitution model with gamma distributed rate heterogeneity. In addition, an uncorrelated log-normal relaxed molecular clock64 was used to model the variation of evolutionary (substitution) rates across branches. The extended Bayesian skyline plot (EBSP) demographic method65 was selected as this model does not depend on a prespecified parametric model of demographic history and the method has been proven to indicate the most appropriate demographic model for any given dataset. Earlier BEAST analyses on a related dataset identified the molecular clock model and tree prior used here to have the highest support by using Bayes factor (ratio of the marginal likelihoods of two competing models) based model selection9.
All parameters were estimated jointly in a BEAST2 analysis using 10 independent chains of 500 million MCMC generations, with samples taken every 50,000 generations. Log files were inspected in Tracer v1.6 for convergence, proper mixing, and sufficient sampling, assessed by whether the chain length produced an effective sample size (ESS) for all parameters larger than 300. A 30% burn-in was removed from each run, and LogCombiner v2.5.0 was used to combine log and tree files of the independent BEAST2 runs. Parameter medians and 95% highest posterior density (HPD) intervals were finally estimated from 70,000 sampled MCMC generations. The entire analysis was replicated on five random subsets of 100 taxa of the dataset to test if the results were affected by sampling bias.
The entire analysis was run while sampling only from the prior, to ensure that prior parameters were not causing over-constraining of the calculations. The resulting parameter distributions were compared in Tracer. The posterior sample of the time-trees were summarized in TreeAnnotator v2.5.2 to produce a maximum clade credibility tree with the posterior estimates of node heights visualized on it.
Genomic rearrangements and SNP analysis
Large genomic rearrangements were identified by analysis of the aligned reference genome sequences using the Artemis Comparison Tool (ACT).
A VCF file containing all SNP sites was extracted using snp-sites59 from all strains included in this study. Conserved SNPs between lineage II and lineage II.1 isolates were extracted using custom calculations in R v.3.3.3, thereby comparing SNPs with the D23580 reference sequence and annotation (FN424405.1). SNPs that were conserved in 51 of the 53 sublineage II.1 strains, and not present in lineage II strains were subjected to a functional analysis. These SNPs were functionally studied by comparison with the D23580 annotation56. Ortholog loci in S. Typhimurium LT2 (NC_003197.2) were identified using BLASTN 2.6.0+.
For SNPs present in coding regions, the effect of the SNP on the respective amino acid sequence was assessed. For non-synonymous SNPs, the PAM1 value and delta bitscore value was included. The higher the PAM1 value, the more frequent specific amino acid substitutions are observed. Delta bitscores were calculated by subtracting the bitscore for a given HMM domain in lineage II from the bitscore of the orthologous domain lineage II.1 strains66.
To calculate the invasiveness index per strain, sequence reads of each sample were mapped against the S. Typhimurium SL1344 reference genome (FQ312003.1) using BWA mem v0.7.1267 to produce a BAM file thereby using default parameters but maximum insert size changed to 3 times the mean fragment size of the sequencing library. We used Picard (http://broadinstitute.github.io/picard) to identify optical duplicates generated during library preparation. SNPs were called using samtools v1.2 mpileup68, variants with coverage < 10 or quality < 30 were filtered and excluded. SNP calls were used to produce variant coding sequences. Protein sequences were then screened using phmmer to identify the closest homologs to the 196 predictive genes used by the invasiveness index model. These genes were then scored against profile hidden Markov models (HMMs) for these protein families from the eggNOG database to test for uncharacteristic patterns of sequence variation. Bitscores produced in the comparison of each protein sequence to its respective protein family HMM were then used as input to the model. The groups were compared using a Mann Whitney U-test.
Sequence typing, resistance, and plasmid analysis
Resistance genes were determined from the raw Illumina sequencing data using ariba v 2.11.169 with CARD database version 1.1.870. SNPs explaining a DCS phenotype was checked individually for strains showing DCS. The gyrA, gyrB, parC, parE, acrB sequences of reference sequence from S. Typhimurium LT2 (NC_003197.2) were compared to assemblies of the DCS strains using BLASTN 2.6.0+. The presence of plasmid replicons was determined from raw Illumina reads using SRST271 with the complementary P18 plasmid replicon database.
The PacBio reference sequence of plasmid pSTm-ST313-II.1 (S. Typhimurium DRC, this study) was searched for similar nucleotide sequences publicly available using NCBI Blast with the Nucleotide collection (nt), update 2017/07/13. Pairwise comparisons were done using BRIG72. pSTm-ST313-II.1 was compared with plasmids R478 (Serratia marcescens USA, BX664015), pKST313 (S. Typhimurium, LN794248) and pSTm-A54650 (S. Typhimurium, LK056646). A de novo assembly was performed based on Illumina sequences of isolate 5390_4 (This study)73 and the assembly of the plasmid sequence was used for pairwise comparative analysis. Hereto, the contigs of the assembly were reordered using Mauve version 2015_02_2574 and the 12 contigs homologous to pSTm-ST313-II.1 were retained for further analysis.
Presence of fljB (FljB) and fliC (FliC) were confirmed at the DNA and protein level for a S. Typhimurium reference lineage II (isolate 9412_3) and sublineage II.1 (10433_3) strain. DNA was extracted from both strains using Gentra Puregene Yeast/Bact. Kit (Qiagen, USA) and PCR-amplified using fljB (fljB-F and fljB-R) and fliC (fliC-F and fliC-R) specific primers (Supplementary Table 5).
For protein samples, overnight cultures were centrifuged at 1500 g and pellets were suspended in 300 µL phosphate-buffered saline (PBS, pH 7.4). The suspension was homogenized using FastPrep-24 (MP Biomedicals, Santa Ana, California, USA) and centrifuged at 15,000 rpm. 10 µL of the supernatant was diluted 1:1 with sample buffer (Laemmle, Sigma-Aldrich, St. Louis, Missouri, US) before loading on SDS-page gel (12%). After running (45 min 100 V) the gel was coloured with Coomassie blue.
Strains were grown in 10 ml low salt LB Broth overnight, diluted 1:100 in PBS and 5 µL was spotted onto rdar phenotype plates (1.5% Agar, 1% Tryptone, 0.5% Yeast Extract, 20 µg mL−1 Coomassie Brilliant Blue, 40 µg mL−1 Congo Red in water)75. The plates were incubated at 27 °C without inversion for 84 h, phenotype analysed and photographed. Colonies were quantitatively analysed using the IRIS software76.
Four S. Typhimurium ST313 lineage II (12299_3, 9266_3, 9412_3 and D23580) and four S. Typhimurium sublineage ST313 sublineage II.1 (10393_3, 10433_3,12306_3 and 8866_3) isolates were analysed on the OmniLog phenotype MicroArray (PM) platform, in three independent biological replicates each. Overnight cultures cells were transferred with a sterile swab to 15 mL IF-0 (12.5 mL IF-0 with 2.5 mL H2O) and stirred to obtain a uniform suspension. Turbidity of the suspension was adjusted to 42% transmittance T by using the Biolog Turbidimeter. Plates PM 1 and PM 2 were inoculated with 100 µL per well of the cell suspension mix diluted 1:5 in IF-0 containing 1.2% dye mix A. All plates were covered by anaerobic sealing foil (Roche) and incubated in the Omnilog phenotype MicroArray system for 48 h at 37 °C. Statistical calculations and visualization were done in R (R Core Team) by using the opm package77. The curve parameters were estimated using spline fitting. The mean of the area under the curve (AUC) was compared between sublineage II.1 versus lineage II strains using a linear model based on a Tukey-type contrast using the opm_mcp function from the multcomp package78.
Mutant strains S. Typhimurium D23580 ΔasmA, S. Typhimurium D23580 ΔyhjJ, S. Typhimurium D23580 ΔyhjK and S. Typhimurium D23580 ΔwxzC were constructed. Hereto, the Kanamycin resistance gene (kan) was PCR-amplified from pKD4 using Q5 HotStart DNA Polymerase (New England Biolabs, Massachusetts, U.S.A.) and gene specific oligos (Integrated DNA Technologies, Illinois, USA) for asmA (asmA-F and asmA-R), wzxC (wzxC-F and wzxC-R), yhjJ (yhjJ-F and yhjJ-R) and yhjK (yhjK-F and yhjK-R), listed in Supplementary Table 5. DNA was prepared by gel extraction (Qiagen, Hilden, Germany) and ethanol precipitation.
The pSIM18 vector carrying the lambda RED recombinase system79 was electroporated into S. Typhimurium D23580 using 10.5 ng DNA at a setting of 2.5 kV, 200 ohms and 25 µF (Bio-Rad MicroPulser, California, USA). 750 µL of SOC outgrowth medium (Thermo Fisher Scientific, Massachusetts, USA) was added and cells grown at 30 °C for 90 min, 100 μL aliquots were plated out onto plates containing Hygromycin and colonies recovered next day. The subsequent S. Typhimurium D23580::pSIM18 was used to create the mutant strains.
S. Typhimurium D23580::pSIM18 was grown overnight at 30 °C and then diluted 1 in 100 the next day in low salt LB plus 100 µg mL−1 Hygromycin B (Thermo Fisher, Massachusetts, U.S.A.) and incubated for 3 h, shaking at 30 °C to an optical density (OD) of 0.4. The culture was heat-shocked at 42 °C for 15 min, cooled on ice for 10 min and then was spun for 10 min at 2500×g and washed twice in ice cold 10% glycerol. The cell pellet was finally resuspended in 140 µL of 10% glycerol and 60 µL aliquots were electroporated with 1 µg of DNA (Table 1) in a precooled 2 mm electroporation cuvette. Cells were then incubated in 500 µL of pre-warmed SOC outgrowth medium (Thermo Fisher Scientific, Massachusetts, USA) at 37 °C for 2 h. 3 × 100 µL aliquots were plated onto 50 µg mL−1 Kanamycin (Thermo Fisher, Massachusetts, USA) LB plates and grown overnight at 37 °C. The remaining volume was left at room temperature overnight and plated on 50 µg mL−1 Kanamycin and left to grow at 37 °C. The knock-out mutation was confirmed using Illumina sequencing.
THP-1 macrophage invasion and replication assay
THP-1 monocytes (European Collection of Authenticated Cell Cultures (ECACC), cat no. 88081201) were plated at 1 × 105 cells per well in RPMI (Gibco) with 2 mM L-glutamine (Sigma) and 10% foetal bovine serum (Sigma) with PMA (Phorbol 12-myristate 13-acetate, (Sigma) to differentiate to macrophages. After 72 h, media was changed to the supplemented RPMI (as defined above) for 24 h before infection. Bacterial isolates SL1344, D23580, 2101, 9266_3, 12299_3, 6948_3, 9412_3, 10055_3, 8866_3, 12155_3, 10393_3, and 10433_3 were inoculated in 10 mL low-salt lysogeny broth (LB) from frozen stocks and incubated at 37 °C, shaking for ~17.5 h prior to use. For infection, bacteria were diluted in PBS to an OD of 1 before adding to RPMI. 500 µL of bacteria in media were added to cells for a multiplicity of infection of 20:1 and incubated at 37 °C for 30 min. At 30 min, media containing bacteria was removed and replaced with media containing 0.1 mg mL−1 gentamicin. For the 1 h invasion timepoint, at 1 h post-infection, cells were washed 1x in PBS then lysed in 1% Triton, and serial dilutions at 10−1, 10−2, 10−3 prepared in PBS. 50 µL of each dilution was spotted on LB agar plates in 5 technical replicates of 10 µL spots and incubated at 37 °C. For the 6 h intracellular replication timepoint, gentamicin-containing media was replaced by the supplemented RPMI at 1 h post-infection and incubated at 37 °C for another 5 h. At 6 h post-infection, cells were washed 1× in PBS and lysed with 1% Triton, as for the cells at the 1 h timepoint. Agar plates were incubated until colony forming units were visible for counting to calculate viable bacteria per mL. Experiments were done in three biological replicates, mean and standard error of the mean was calculated for all strains.
Salmonella strains were grown static overnight in LB at 37 °C. Inoculations were prepared by diluting overnight culture in PBS. Inoculums were plated post infection on LB agar plates for confirmation. Groups of C57/Bl6 mice were pre-treated with 50 mg of Streptomycin by oral gavage and infected intravenously with 2 × 102 colony forming units (CFU) or orally with 2 × 106 CFU with each Salmonella strain. At day 4 post infection mice were culled and organs removed. Homogenised organs were serially diluted in PBS and 20 µL of each dilution were spotted into LB agar plates. CFUs were counted next day to calculate number of CFUs per organ. All experiments on animals were performed under a UK animal license that has been through local ethical review before being approved by Sanger—Animal Welfare and Ethical Review Body (AWERB) and performed according to the regulations of the UK Home Office Scientific Procedures Act (1986).
Requests for obtaining biological material (mutant strains) should be addressed to the corresponding author. Exchange of clinical isolates should always be in agreement with the ITM (Antwerp, Belgium) and INRB (Kinshasa, DRC), co-owning the bacterial isolates.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Sequence data that support the findings of this study have been deposited in SRA with accession codes as listed in Supplementary Data 1. The annotated Pacbio’d reference genome of Salmonella Typhimurium strain 10433_3 is uploaded to GenBank with accession ID ERS1310131. The generated phylogenetic tree (as presented in Fig. 2a) is publicly accessible in MicroReact: https://microreact.org/project/ZfwCFTj2-/d9f0ce6f. The source data underlying Fig. 6a, b and Supplementary Figs 6, 9–11 are provided as Source Data File. All other datasets generated during and/or analysed the current study are available from the corresponding author on reasonable request.
Crump, J. A., Sjolund-Karlsson, M., Gordon, M. A. & Parry, C. M. Epidemiology, clinical presentation, laboratory diagnosis, antimicrobial resistance, and antimicrobial management of invasive Salmonella infections. Clin. Microbiol Rev. 28, 901–937 (2015).
Reddy, E. A., Shaw, A. V. & Crump, J. A. Community-acquired bloodstream infections in Africa: a systematic review and meta-analysis. Lancet Infect. Dis. 10, 417–432 (2010).
Ao, T. T. et al. Global burden of invasive nontyphoidal Salmonella disease, 20101. Emerg. Infect. Dis. 21, 941–949 (2015).
Feasey, N. A., Dougan, G., Kingsley, R. A., Heyderman, R. S. & Gordon, M. A. Invasive non-typhoidal salmonella disease: an emerging and neglected tropical disease in Africa. Lancet 379, 2489–2499 (2012).
Kariuki, S. et al. Characterisation of community acquired non-typhoidal Salmonella from bacteraemia and diarrhoeal infections in children admitted to hospital in Nairobi, Kenya. BMC Microbiol 6, 101 (2006).
Kariuki, S. et al. Invasive multidrug-resistant non-typhoidal Salmonella infections in Africa: zoonotic or anthroponotic transmission? J. Med Microbiol 55, 585–591 (2006).
MacLennan, C. A. et al. Dysregulated humoral immunity to nontyphoidal Salmonella in HIV-infected African adults. Science 328, 508–512 (2010).
Branchu, P., Bawn, M. & Kingsley, R. A. Genome variation and molecular epidemiology of Salmonella enterica Serovar Typhimurium Pathovariants. Infect. Immun. 86, e00079–18 (2018).
Okoro, C. K. et al. Intracontinental spread of human invasive Salmonella Typhimurium pathovariants in sub-Saharan Africa. Nat. Genet 44, 1215–1221 (2012).
Kariuki, S. et al. Ceftriaxone-resistant Salmonella enterica serotype typhimurium sequence type 313 from Kenyan patients is associated with the blaCTX-M-15 gene on a novel IncHI2 plasmid. Antimicrob. Agents Chemother. 59, 3133–3139 (2015).
Feasey, N. A. et al. Drug resistance in Salmonella enterica ser. Typhimurium bloodstream infection, Malawi. Emerg. Infect. Dis. 20, 1957–1959 (2014).
Msefula, C. L. et al. Genotypic homogeneity of multidrug resistant S. Typhimurium infecting distinct adult and childhood susceptibility groups in Blantyre, Malawi. PLoS One 7, e42085 (2012).
Crump, J. A. & Heyderman, R. S. A perspective on invasive Salmonella Disease in Africa. Clin. Infect. Dis. 61(Suppl 4), S235–S240 (2015).
Kalonji, L. M. et al. Invasive Salmonella Infections at multiple surveillance sites in the Democratic Republic of the Congo, 2011–2014. Clin. Infect. Dis. 61(Suppl 4), S346–S353 (2015).
WHO. Background document: The diagnosis, treatment and prevention of typhoid fever. (2003).
Langridge, G. C. et al. Patterns of genome evolution that have accompanied host adaptation in Salmonella. Proc. Natl Acad. Sci. USA 112, 863–868 (2015).
Okoro, C. K. et al. Signatures of adaptation in human invasive Salmonella Typhimurium ST313 populations from sub-Saharan Africa. PLoS Negl. Trop. Dis. 9, e0003611 (2015).
Singletary, L. A. et al. Loss of multicellular behavior in epidemic african nontyphoidal Salmonella enterica Serovar Typhimurium ST313 strain D23580. MBio 7, e02265 (2016).
Ramachandran, G., Aheto, K., Shirtliff, M. E. & Tennant, S. M. Poor biofilm-forming ability and long-term survival of invasive Salmonella Typhimurium ST313. Pathog. Dis. 74, ftw049 (2016).
Ramachandran, G., Perkins, D. J., Schmidlein, P. J., Tulapurkar, M. E. & Tennant, S. M. Invasive Salmonella Typhimurium ST313 with naturally attenuated flagellin elicits reduced inflammation and replicates within macrophages. PLoS Negl. Trop. Dis. 9, e3394 (2015).
Hammarlof, D. L. et al. Role of a single noncoding nucleotide in the evolution of an epidemic African clade of Salmonella. Proc. Natl. Acad. Sci. USA 115, E2614–E2623 (2018).
Parsons, B. N. et al. Invasive non-typhoidal Salmonella typhimurium ST313 are not host-restricted and have an invasive phenotype in experimentally infected chickens. PLoS Negl. Trop. Dis. 7, e2487 (2013).
Lunguya, O. et al. Antimicrobial resistance in invasive non-typhoid Salmonella from the Democratic Republic of the Congo: emergence of decreased fluoroquinolone susceptibility and extended-spectrum beta lactamases. PLoS Negl. Trop. Dis. 7, e2103 (2013).
Ley, B. et al. Invasive Salmonella enterica serotype typhimurium infections, Democratic Republic of the Congo, 2007-2011. Emerg. Infect. Dis. 20, 701–704 (2014).
Kariuki, S. & Onsare, R. S. Epidemiology and genomics of invasive nontyphoidal Salmonella infections in Kenya. Clin. Infect. Dis. 61(Suppl 4), S317–S324 (2015).
Leekitcharoenphon, P. et al. Genomics of an emerging clone of Salmonella serovar Typhimurium ST313 from Nigeria and the Democratic Republic of Congo. J. Infect. Dev. Ctries 7, 696–706 (2013).
Gomes, C. et al. Macrolide resistance mechanisms in Enterobacteriaceae: Focus on azithromycin. Crit. Rev. Microbiol 43, 1–30 (2017).
Lubelski, J., Konings, W. N. & Driessen, A. J. Distribution and physiology of ABC-type transporters contributing to multidrug resistance in bacteria. Microbiol Mol. Biol. Rev. 71, 463–476 (2007).
Thoma, L. & Muth, G. Conjugative DNA transfer in Streptomyces by TraB: is one protein enough? FEMS Microbiol Lett. 337, 81–88 (2012).
Gilmour, M. W., Thomson, N. R., Sanders, M., Parkhill, J. & Taylor, D. E. The complete nucleotide sequence of the resistance plasmid R478: defining the backbone components of incompatibility group H conjugative plasmids through comparative genomics. Plasmid 52, 182–202 (2004).
Prieto, A. I. et al. Roles of the outer membrane protein AsmA of Salmonella enterica in the control of marRAB expression and invasion of epithelial cells. J. Bacteriol. 191, 3615–3622 (2009).
Rivera-Chavez, F. et al. Salmonella uses energy taxis to benefit from intestinal inflammation. PLoS Pathog. 9, e1003267 (2013).
Wheeler, N. E., Gardner, P. P. & Barquist, L. Machine learning identifies signatures of host adaptation in the bacterial pathogen Salmonella enterica. PLoS Genet 14, e1007333 (2018).
Nuccio, S. P. & Baumler, A. J. Comparative analysis of Salmonella genomes identifies a metabolic network for escalating growth in the inflamed gut. MBio 5, e00929–00914 (2014).
Tacconelli, E. et al. Discovery, research, and development of new antibiotics: the WHO priority list of antibiotic-resistant bacteria and tuberculosis. Lancet Infect. Dis. 18, 318–327 (2018).
Klemm, E. J. et al. Emergence of an extensively drug-resistant Salmonella enterica Serovar Typhi clone harboring a promiscuous plasmid encoding resistance to fluoroquinolones and third-generation cephalosporins. MBio 9, e00105–e00118 (2018).
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).
Phoba, M. F. et al. Multidrug-resistant Salmonella enterica, Democratic Republic of the Congo. Emerg. Infect. Dis. 18, 1692–1694 (2012).
Phoba, M. F. et al. Salmonella enterica serovar Typhi producing CTX-M-15 extended spectrum beta-lactamase in the Democratic Republic of the Congo. Clin. Infect. Dis. 65, 1229–1231 (2017).
Falay, D. et al. Microbiological, clinical and molecular findings of non-typhoidal Salmonella bloodstream infections associated with malaria, Oriental Province, Democratic Republic of the Congo. BMC Infect. Dis. 16, 271 (2016).
Keenan, J. D. et al. Azithromycin to reduce childhood mortality in Sub-Saharan Africa. N. Engl. J. Med 378, 1583–1592 (2018).
ConfédérationSuisse. Focus RD Congo: Le système sanitaire à Kinshasa: médicaments et soins du VIH-sida, de l’hypertension artérielle, du diabète de type II et des troubles mentaux. (2014).
Harrois, D. et al. Prevalence and characterization of extended-spectrum beta-lactamase-producing clinical Salmonella enterica isolates in Dakar, Senegal, from 1999 to 2009. Clin. Microbiol Infect. 20, O109–O116 (2014).
McClelland, M. et al. Comparison of genome degradation in Paratyphi A and Typhi, human-restricted serovars of Salmonella enterica that cause typhoid. Nat. Genet 36, 1268–1274 (2004).
McQuiston, J. R., Fields, P. I., Tauxe, R. V. & Logsdon, J. M. Jr. Do Salmonella carry spare tyres? Trends Microbiol 16, 142–148 (2008).
Ikeda, J. S. et al. Flagellar phase variation of Salmonella enterica serovar Typhimurium contributes to virulence in the murine typhoid infection model but does not influence Salmonella-induced enteropathogenesis. Infect. Immun. 69, 3021–3030 (2001).
Petrovska, L. et al. Microevolution of Monophasic Salmonella Typhimurium during Epidemic, United Kingdom, 2005–2010. Emerg. Infect. Dis. 22, 617–624 (2016).
Mather, A. E. et al. New variant of multidrug-resistant Salmonella enterica Serovar Typhimurium associated with invasive disease in immunocompromised patients in Vietnam. MBio 9, e01056–18 (2018).
Grimont P. A. D., Weill F.-X. Antigenic formulae of the Salmonellae serovars. (World Health Organization, 2007).
CLSI. M100-S28: Performance Standards for Antimicrobial Susceptibility Testing. (2018).
Bolger, A. M., Lohse, M. & Usadel, B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics 30, 2114–2120 (2014).
Hunt, M. et al. Circlator: automated circularization of genome assemblies using long sequencing reads. Genome Biol. 16, 294 (2015).
Chin, C. S. et al. Nonhybrid, finished microbial genome assemblies from long-read SMRT sequencing data. Nat. Methods 10, 563–569 (2013).
Seemann, T. Prokka: rapid prokaryotic genome annotation. Bioinformatics 30, 2068–2069 (2014).
Pruitt, K. D., Tatusova, T., Brown, G. R. & Maglott, D. R. NCBI Reference Sequences (RefSeq): current status, new features and genome annotation policy. Nucleic Acids Res. 40, D130–D135 (2012).
Kingsley, R. A. et al. Epidemic multiple drug resistant Salmonella Typhimurium causing invasive disease in sub-Saharan Africa have a distinct genotype. Genome Res 19, 2279–2287 (2009).
Li, H. et al. The sequence alignment/map format and SAMtools. Bioinformatics 25, 2078–2079 (2009).
Croucher, N. J. et al. Rapid phylogenetic analysis of large samples of recombinant bacterial whole genome sequences using Gubbins. Nucleic Acids Res. 43, e15 (2015).
Page, A. J. et al. SNP-sites: rapid efficient extraction of SNPs from multi-FASTA alignments. Micro. Genom. 2, e000056 (2016).
Stamatakis, A. RAxML version 8: a tool for phylogenetic analysis and post-analysis of large phylogenies. Bioinformatics 30, 1312–1313 (2014).
Letunic, I. & Bork, P. Interactive tree of life (iTOL) v3: an online tool for the display and annotation of phylogenetic and other trees. Nucleic Acids Res. 44, W242–W245 (2016).
Argimon, S. et al. Microreact: visualizing and sharing data for genomic epidemiology and phylogeography. Micro. Genom. 2, e000093 (2016).
Bouckaert, R. et al. BEAST 2: a software platform for Bayesian evolutionary analysis. PLoS Comput Biol. 10, e1003537 (2014).
Drummond, A. J., Ho, S. Y., Phillips, M. J. & Rambaut, A. Relaxed phylogenetics and dating with confidence. PLoS Biol. 4, e88 (2006).
Heled, J. & Drummond, A. J. Bayesian inference of population size history from multiple loci. BMC Evol. Biol. 8, 289 (2008).
Wheeler, N. E., Barquist, L., Kingsley, R. A. & Gardner, P. P. A profile-based method for identifying functional divergence of orthologous genes in bacterial genomes. Bioinformatics 32, 3566–3574 (2016).
Li, H. & Durbin, R. Fast and accurate short read alignment with Burrows-Wheeler transform. Bioinformatics 25, 1754–1760 (2009).
Li, H. A statistical framework for SNP calling, mutation discovery, association mapping and population genetical parameter estimation from sequencing data. Bioinformatics 27, 2987–2993 (2011).
Hunt, M. et al. ARIBA: rapid antimicrobial resistance genotyping directly from sequencing reads. Micro. Genom. 3, e000131 (2017).
McArthur, A. G. et al. The comprehensive antibiotic resistance database. Antimicrob. Agents Chemother. 57, 3348–3357 (2013).
Inouye, M. et al. SRST2: Rapid genomic surveillance for public health and hospital microbiology labs. Genome Med 6, 90 (2014).
Alikhan, N. F., Petty, N. K., Ben Zakour, N. L. & Beatson, S. A. BLAST Ring Image Generator (BRIG): simple prokaryote genome comparisons. BMC Genom. 12, 402 (2011).
Page, A. J. et al. Robust high-throughput prokaryote de novo assembly and improvement pipeline for Illumina data. Micro. Genom. 2, e000083 (2016).
Darling, A. C., Mau, B., Blattner, F. R. & Perna, N. T. Mauve: multiple alignment of conserved genomic sequence with rearrangements. Genome Res 14, 1394–1403 (2004).
Romling, U. Characterization of the rdar morphotype, a multicellular behaviour in Enterobacteriaceae. Cell Mol. Life Sci. 62, 1234–1246 (2005).
Kritikos, G. et al. A tool named Iris for versatile high-throughput phenotyping in microorganisms. Nat. Microbiol 2, 17014 (2017).
Vaas, L. A. et al. opm: an R package for analysing OmniLog(R) phenotype microarray data. Bioinformatics 29, 1823–1824 (2013).
Hothorn, T., Bretz, F. & Westfall, P. Simultaneous inference in general parametric models. Biom. J. 50, 346–363 (2008).
Datsenko, K. A. & Wanner, B. L. One-step inactivation of chromosomal genes in Escherichia coli K-12 using PCR products. Proc. Natl. Acad. Sci. USA 97, 6640–6645 (2000).
Becker A. B. & Wilks A. R. Constructing a Geographical Database. AT&T Bell Laboratories Statistics Research Report , (1995).
We are grateful to Ado Van Assche (K.U. Leuven, Leuven, Belgium), Eke van Zwol and Janah Vandenhoeck (Institute of Tropical Medicine, ITM, Antwerp, Belgium) for assistance with Biolog experiments; to Simon Harris, Jacqueline Keane, Nick Thomson and the Pathogen Informatics team (Wellcome Sanger Institute, Hinxton, Cambridge, United Kingdom) for the support and Bieke Tack for critical reading. This work was funded by the Belgian Directorate of Development Cooperation (DGD) through Project 2.01 of the Third Framework Agreement between the Belgian DGD and ITM, Belgium; the Flemish Interuniversity Council (VLIR-UOS); the Flemish Ministry of Sciences (EWI; SOFI project IDIS and fellowship SVP); the Baillet Latour Fund (The Bacterial Infections in the Tropics (BIT) research cluster at ITM Antwerp, Belgium); the FWO Research Foundation—Flanders (travel grant to SVP.) and the Wellcome Trust. GD is supported by The Wellcome Trust and the NIMR BRC AMR Theme at Cambridge.
The authors declare no competing interests.
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Van Puyvelde, S., Pickard, D., Vandelannoote, K. et al. An African Salmonella Typhimurium ST313 sublineage with extensive drug-resistance and signatures of host adaptation. Nat Commun 10, 4280 (2019). https://doi.org/10.1038/s41467-019-11844-z
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