Advertisement
Research Article

Plant-Associated Symbiotic Burkholderia Species Lack Hallmark Strategies Required in Mammalian Pathogenesis

  • Annette A. Angus equal contributor,

    equal contributor Contributed equally to this work with: Annette A. Angus, Christina M. Agapakis

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Christina M. Agapakis equal contributor,

    equal contributor Contributed equally to this work with: Annette A. Angus, Christina M. Agapakis

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Stephanie Fong,

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Shailaja Yerrapragada,

    Affiliation: Baylor College of Medicine, Houston, Texas, United States of America

    X
  • Paulina Estrada-de los Santos,

    Affiliation: Departamento de Microbiología, Escuela Nacional de Ciencias Biológicas, Instituto Politécnico Nacional, Prolongación de Carpio y Plan de Ayala, Ciudad de México, Distrito Federal, México

    X
  • Paul Yang,

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Nannie Song,

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Stephanie Kano,

    Affiliation: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Jésus Caballero-Mellado †,

    † Deceased.

    Affiliation: Genomic Sciences Center, National Autonomous University of México, Cuernavaca, Morelos, México

    X
  • Sergio M. de Faria,

    Affiliation: Embrapa Agrobiologia, Seropédica, Rio de Janeiro, Brazil

    X
  • Felix D. Dakora,

    Affiliation: Chemistry Department, Tshwane University of Technology, Arcadia Campus, Pretoria, South Africa

    X
  • George Weinstock,

    Affiliation: Dept. of Genetics, Washington Univ. School of Medicine, St. Louis, Missouri, United States of America

    X
  • Ann M. Hirsch mail

    ahirsch@ucla.edu

    Affiliations: Dept. of Molecular, Cell and Developmental Biology, University of California Los Angeles, Los Angeles, California, United States of America, Molecular Biology Institute, University of California Los Angeles, Los Angeles, California, United States of America

    X
  • Published: January 08, 2014
  • DOI: 10.1371/journal.pone.0083779

Abstract

Burkholderia is a diverse and dynamic genus, containing pathogenic species as well as species that form complex interactions with plants. Pathogenic strains, such as B. pseudomallei and B. mallei, can cause serious disease in mammals, while other Burkholderia strains are opportunistic pathogens, infecting humans or animals with a compromised immune system. Although some of the opportunistic Burkholderia pathogens are known to promote plant growth and even fix nitrogen, the risk of infection to infants, the elderly, and people who are immunocompromised has not only resulted in a restriction on their use, but has also limited the application of non-pathogenic, symbiotic species, several of which nodulate legume roots or have positive effects on plant growth. However, recent phylogenetic analyses have demonstrated that Burkholderia species separate into distinct lineages, suggesting the possibility for safe use of certain symbiotic species in agricultural contexts. A number of environmental strains that promote plant growth or degrade xenobiotics are also included in the symbiotic lineage. Many of these species have the potential to enhance agriculture in areas where fertilizers are not readily available and may serve in the future as inocula for crops growing in soils impacted by climate change. Here we address the pathogenic potential of several of the symbiotic Burkholderia strains using bioinformatics and functional tests. A series of infection experiments using Caenorhabditis elegans and HeLa cells, as well as genomic characterization of pathogenic loci, show that the risk of opportunistic infection by symbiotic strains such as B. tuberum is extremely low.

Introduction

The genus Burkholderia encompasses a wide range of species, including human pathogens listed as potential bioterrorist threats, opportunistic human and plant pathogens, and beneficial plant symbionts that fix nitrogen in legume root nodules. Although characteristics that benefit rhizosphere bacteria, such as ecological and nutritional flexibility, antibiotic resistance, root adherence, biofilm formation, osmotolerance, and competition for mineral nutrients may contribute to the virulence of opportunistic pathogens [1], phylogenetic evidence distinguishes the true symbionts from the opportunistic pathogens in Burkholderia [2], [3].

Since it was removed from Pseudomonas ribosomal RNA group II and moved into Burkholderia in 1992 [4], the genus has undergone significant taxonomic changes, with several strains transferred to Ralstonia as early as 1995 [5]. Approximately a decade after the original transfer of seven plant and animal pathogens to Burkholderia, considerable evidence began to accumulate from 16S rDNA-based phylogenetic studies indicating that this genus consisted of two distinct lineages (see references in [3]). One lineage contains species that consist of 1) mainly mammalian pathogens, e.g., the B. pseudomallei/mallei group, 2) the opportunistic pathogens, mainly the B. cepacia complex (BCC), 3) the plant pathogens, such as B. glumae and B. gladioli, and 4) some environmental (saprophytic) species. The second lineage includes 1) many saprophytic species that have potential for bioremediation of xenobiotics, e.g., B. unamae and B. xenovorans, 2) species that live in symbiotic relationships with plants, either as nitrogen-fixing inhabitants of legume nodules, such as B. tuberum and B. phymatum, and 3) plant growth-promoting bacteria (PGPB), for example, B. phytofirmans.

Trees based on other genes such as acdS [6] or recA [7] also supported the separation into two distinct clades. Perin et al. [8] not only obtained a separation into two lineages based on 16S RNA phylogeny, but also found that genes encoding two virulence factors, cblA (giant cable pili) and esmR, (BCESM, an epidemic strain marker [9]), were not detected in the clade containing the symbiotic and legume-nodulating species. By contrast, many members of the other clade possessed these gene sequences. In addition to these studies, our MLSA analysis of 77 genome sequences based on five concatenated gene sequences determined that two major groups, A and B, were delineated, based not only on phylogeny, but also on GC content [3], [10]. The B group consists of the mammalian and plant pathogens as well as the opportunistic pathogens and some environmental species, whereas the A group is divided into two subgroups, which includes many environmental and plant-associated species [3].

The goal of this report is to characterize the members of the A group more fully and propose that they be used as replacements for the opportunistic, pathogenic Burkholderia species, namely the BCC, which had been recommended for agricultural use or are already employed in some countries as inocula or biocontrol agents (BCA). Examples are B. vietnamiensis, which fixes nitrogen in association with rice roots in Asia [11], and B. cenocepacia and other BCC bacteria, which have been suggested for use as BCA because they kill pathogenic fungi [12]. However, major concerns about putting opportunistic pathogens into the soil have been voiced [13], [14] because some species, e.g., B. vietnamiensis, are common inhabitants of the lungs of cystic fibrosis (CF) patients [15], [16]. The net result is that restrictions have been placed on using BCC member species for crop use in the U.S. [17].

The centers of origin of the symbiotic Burkholderia species are South Africa and Brazil [10]. Many southern hemisphere soils are highly acidic, arid, and low in nutrients [18]. Thus, species of the A group have significant agricultural potential for use as inocula for legume production in areas with such soils. We sequenced the genomes of four diazotrophic Burkholderia species in the A group, one of which nodulates legumes (Table 1). The four genomes sequenced are large, ranging from ca. 8.29 Mbp (B. silvatlantica SRMrh20T) to ca. 9.95 Mbp (B. unamae MTI641T). Here, we expand upon the analyses made by Perin et al. [8] and Estrada-de los Santos et al. [3], addressing the occurrence in these species and other members of the A clade of known virulence determinants implicated in Burkholderia pathogenesis [19], such as 1) motility, chemotaxis, and attachment; 2) antibiotic resistance; and 3) the type 3, 4, and 6 secretion systems (Fig. 1). We also performed functional tests to determine the pathogenic properties of the symbiotic species versus the pathogenic strains, namely by examining the extent of pathogenicity to inoculated Caenorhabditis elegans nematodes and HeLa cells.

thumbnail

Figure 1. Distribution of virulence and symbiotic loci across Burkholderia species.

Virulence-associated loci were identified using BLASTP against characteristic sequences (B. pseudomallei or B. cenocepacia ATPases for secretion systems, B. pseudomallei pilus genes for pilus-related clusters (red), and B. tuberum nifH and nodA sequences (green)). Non-canonical or truncated clusters are indicated in pink, and clusters highly associated with virulence for the Type 3 and Type 6 secretion systems are denoted with an asterisk.

doi:10.1371/journal.pone.0083779.g001
thumbnail

Table 1. Bacterial strains used in this study.

doi:10.1371/journal.pone.0083779.t001

Materials and Methods

Bioinformatics Analysis of Virulence Loci

Protein sequences associated with virulence in B. pseudomallei (for chemotaxis, attachment, Type 3 and Type 6 secretion systems; T3SS and T6SS) or B. cenocepacia (for the Type 4 secretion system; T4SS) were used to search the genomes of other Burkholderia strains using BLASTP. Top hits were identified and cluster arrangements of gene neighborhoods were verified using the Integrated Microbial Genomes tools (https://img.jgi.doe.gov/). Consensus Neighbor-Joining phylogenetic trees were constructed in MEGA 5.1 [20] using CLUSTALW alignment of several concatenated protein sequences with the p-distance method and 1000 bootstrap replicates.

Culture of Bacteria

The bacteria used for experimental analysis are listed in Table 1. For routine culture, Burkholderia strains were grown on either liquid or solidified LB minus NaCl medium at 30°C, with the exception of B. thailandensis E264 [21], which was grown at 37°C for 48 h. E. coli OP50 [22] was grown on LB agar at room temperature for 24 h. Bacillus simplex 237 [23] grew up overnight at 30°C on LB agar. Prior to inoculation or seeding assay plates, all strains were grown in broth culture in the appropriate medium with aeration under the temperatures and for the times indicated previously. Broth cultures were adjusted to an OD600 = 0.1 with phosphate-buffered saline (PBS) to normalize cell numbers.

Antibiotic Resistance Assays

The following bacteria strains were tested for antibiotic resistance: Burkholderia tuberum STM678T, B. silvatlantica PVA5 and SRMrh20T, B. unamae MTI641T, B. vietnamiensis G4, B. gladioli BSR3, and B. thailandensis E264 (Table 1).

In a preliminary experiment using premade antibiotic discs, we screened for antibiotics that could be used in a hole-punch filter paper experiment. The stocks for the antibiotics used for the filter paper disc assay were: ampicillin (100 µg/ml), kanamycin (30 µg/ml), chloramphenicol (25 µg/ml), gentamicin (40 µg/ml), rifampicin (15 µg/ml), streptomycin (100 µg/ml), erythromycin (15 µg/ml), nalidixic acid (25 µg/ml), and tetracycline (30 µg/ml).

From agar-grown cultures, a single colony from each plate was transferred to a 5 mL liquid culture incubated overnight at 30°C on a shaker. One milliliter of the culture was taken and centrifuged. The supernatant was removed and the bacteria were re-suspended in PBS. The solution was then diluted to an OD600 of 0.1. Using a cotton swab, the bacterial suspensions were spread onto agar plates. Five µL of dilutions of each antibiotic stock were added to previously autoclaved hole-punch discs, which were allowed to dry for approximately 15 min before placing them onto the bacteria-inoculated plates. The plates were incubated at 30°C until a bacterial lawn was evident, usually 1–2 days depending on the strain. Colonies were examined for zones of clearing (susceptible) or no clearing (resistant) around them [24]. A photograph was taken of each plate from the same height and at the same magnification. The radii of the clearing zones were determined by measuring on the photograph the number of pixels from the paper disc to the edge of the clearing. The pixel number was converted to millimeters using the standard conversion of 3.81 pixels per millimeter. The experiment was performed twice and a heat map summarizing the average values of five replicates for the highest concentration of the antibiotic stock was generated in R version 2.15.2.

Culture of Mammalian Cells and Experimental Assay

Human cervical carcinoma cells (HeLa cells) were routinely cultured and passaged in T-75 flasks with Dulbecco's Modified Eagle Medium (DMEM; Gibco Life Technologies)/10% Fetal Bovine Serum (FBS; Gibco Life Technologies)/1% antibiotics (penicillin/streptomycin) and incubated at 37°C with 5% CO2. Cells were grown to 70–80% confluency and passaged approximately every 3–4 days and carried to a maximum of 25 passages from original stocks. Cells were washed with calcium-magnesium-free phosphate-buffered saline (CMF-PBS) prior to treatment with trypsin and before assays. For in vitro cytotoxicity assays, HeLa cells grown in a multi-well round-bottom plate format were washed with sterile CMF-PBS, inoculated with bacteria for an MOI (multiplicity of infection) of 50, or mock inoculated with medium alone and incubated for 4, 8, or 24 h. After the appropriate incubation period, cytotoxicity was measured via lactate dehydrogenase (LDH) release using the Cyto Tox 96 Non-Radioactive Assay kit (Promega). All work was carried out in a sterile class II laminar flow hood.

Maintenance of C. elegans and Experimental Assay

C. elegans Bristol-N2 cultures were maintained according to methods described in Stiernagle [25]. Briefly, the worms were routinely grown on nematode growth agar medium (NGM) seeded with E. coli OP50, and incubated at 22°C. Nematodes from plates in which the bacterial lawn had cleared were passaged onto fresh plates with E. coli OP50 by aseptically transferring plugs of agar with worms on the surface. For the slow killing assays, stock plates were washed with sterile water to suspend worms and eggs, then stage-synchronized for harvesting L3-L4 larvae according to methods described earlier [25] and transferred onto NGM agar plates seeded with the bacterial strain under investigation. The initial numbers of live worms were counted and then monitored every 24 h at the same time of the day over 72 h to assess the effects of bacterial toxicity; however, some experiments continued for as long as 5 days. Death was assessed by a lack of motility and response to touch with a sterile platinum loop. All experiments were performed a minimum of three times to verify the nematode response.

For the competition experiments, the nematodes were seeded onto solidified NGM equidistant from two bacterial lawns–one comprised of B. thailandensis E264 and the other consisted of either the symbiotic Burkholderia species or E. coli OP50. Measurements were made as described above.

Genomes

The four genomes sequenced for this study and their accession numbers are: B. tuberum STM678 (Accession Number PRJNA30619), B. unamae MTI641 (PRJNA59741), B. silvatlantica PVA5 (PRJNA51165) and B. silvatlantica SRMrh20 (PRJNA41353).

Results

Genetic/Genomic Analyses

Flagella, Chemotaxis, and Attachment: A number of extracellular and surface structures are involved in B. pseudomallei pathogenesis, including capsular polysaccharide, Type IV pili, tad-type pili, and Type I fimbriae [19], [26]. The B. pseudomallei genome contains genes encoding a full complement of such virulence factors, including the capsule [27], two Type IV pilin clusters [28], three tad-type pili, and six Type I fimbriae [29] (Fig. 1). The environmental and symbiotic strains contain significantly fewer such clusters, with capsule genes present in only B. silvatlantica SRMrh20T and PVA5. All strains except the mammalian pathogens lack the Type IV pilus cluster pilB. The environmental and symbiotic species, except for B. phytofirmans and B. xenovorans (Fig. 1), contain only one Type I fimbriae cluster. In general, the pathogenic species have multiple clusters of Type I fimbriae. Except for B. phenoliruptrix Br3459, which has 3 of the four types, the environmental and nodulating species have either one or two types of tad pili (Fig. 1).

Bacterial motility is frequently associated with pathogenesis, and conflicting studies have shown that Burkholderia flagella are important for motility and infectivity under certain conditions. Although an early genetic study reported that interruption of the B. pseudomallei fliC gene with a transposon did not disrupt infection in diabetic rats or Syrian hamsters [30], a subsequent analysis showed that a B. pseudomallei fliC knockout was avirulent in intranasal infection of BALB/c mice [31]. More recently, a second flagellar gene cluster (fla2) responsible for intracellular motility was identified in Burkholderia thailandensis [32].

All strains of Burkholderia in our analysis share a cluster of flagellar and chemotaxis-related genes with high sequence homology and high synteny (Fig. 1, Fig. 2A). In the A group of Burkholderia spp. (3), the chemotaxis and flagellar genes are clustered together and adjacent to one another on the chromosome (Fig. 2B). In contrast, the cluster found in members of the pathogenic clade or B group (3) is split into four different regions across the chromosome, except in B. mallei, where the cluster is divided into 5 regions (Fig. 2C). On the other hand, the fla2 cluster is present only in a small percentage of strains from the B. pseudomallei clade, which includes B. pseudomallei 1655, 406e, 668, DM98, and MSHR305, B. thailandensis E264, Bt, and TX DOH, and B. oklahomensis EO147 and CG786 (Fig. 2D). Flagella have also been identified as virulence factors in the opportunistic pathogen B. cenocepacia [33], which has a second cluster showing divergence from the B. pseudomallei cluster (Fig. 2E).

thumbnail

Figure 2. Flagellar gene clusters in Burkholderia.

All Burkholderia strains share a highly similar chemotaxis and flagellar gene cluster (fla1) on chromosome 1. Although the A group and the pathogenic B group share high homology in gene sequence and chromosomal arrangement, a phylogenetic analysis of five concatenated protein sequences (FliC, FlgM, FlgE, FlhB, FlgJ) shows a distinct clustering of the two lineages [A]. Additionally, the A group cluster is arranged entirely sequentially [B] whereas the pathogenic B cluster is split into four different regions throughout chromosome 1 (the B. mallei cluster is split into 5 regions)[C]. The fla1 gene cluster is responsible for Burkholderia motility on soft agar, but not for intracellular motility or plaque formation in models of infection [32]. A second flagellar gene cluster on chromosome 2 (fla2) is necessary for this intracellular motility. This second cluster is present only in the pathogenic strains, i.e. B. pseudomallei, B. thailandensis, and B. oklahomensis [D], and a similar cluster exists on chromosome 2 of the opportunistic pathogen B. cenocepacia [E].

doi:10.1371/journal.pone.0083779.g002

Type 3 secretion system: The T3SS is a hallmark of pathogenic Burkholderia species. B. pseudomallei carry three such clusters on chromosome 2 (Fig. S1). The T3SS-3 locus (BPSS1529-BPSS1552) is homologous to the T3SS that modulates intracellular behavior of the human pathogens Salmonella and Shigella [19] and has been shown to be essential for endosome escape in B. pseudomallei infection [32]. Clusters homologous to B. pseudomallei T3SS-3 are present only in the B. pseudomallei and the B. cepacia groups and were not found in the plant pathogens or in any of the A group environmental or symbiotic strains (3* in Fig. 1).

Although the functions of T3SS clusters 1 and 2 in B. pseudomallei infection are less well-characterized [26], B. pseudomallei T3SS-1 (BPSS1390-BPSS1410) and T3SS-2 (BPSS1610-BPSS1629), both show homology to the T3SS of the plant pathogen Ralstonia solanacearum. T3SS-1 homologs are not present in B. mallei [34] or in the infection model B. thailandensis E264 [21], but homologous clusters were found in the plant pathogens and two of the A group strains, namely B. graminis and B. phenoliruptrix, a recently sequenced nodulator of Mimosa flocculosa [35]. A fourth type of T3SS operon dissimilar to the three found in B. pseudomallei is also present in the environmental strains B. phytofirmans [36] and B. xenovorans [37] (Fig. S1). This cluster is homologous to the T3SS operon in the endophytic plant pathogen Herbaspirillum rubrisubalbicans [38]. Mitter et al. [36] reported that the genes for the needle-forming component of the T3SS in B. phytofirmans PsJN appear to be missing (see Fig. S1). Genes encoding proteins for the various types of T3SS were absent in B. tuberum, B. unamae, the two B. silvatlantica strains, and the vast majority of the A group species (Fig. 1).

Type 4 secretion system: The T4SS is involved in a number of functions important for pathogenesis [39], [40]. Two T4SS have been identified in Burkholderia cenocepacia, one chromosomally-encoded VirB/D4 type involved in plasmid mobilization, and a larger plasmid-borne cluster associated with plant tissue water-soaking infection [41]. Although neither T4SS is found in the B. pseudomallei group, variants are found throughout the B. cepacia cluster and the environmental diazotrophic Burkholderia strains (Fig. 1,3), including the non-pathogenic, N2-fixing species shown in Table 1. Only members of the BCC and the plant pathogens possess the plasmid-borne, pathogenesis-associated T4SS cluster, although variants of the standard VirB/D4 exist in up to three copies in some of the environmental Burkholderia genomes.

thumbnail

Figure 3. Phylogenetic analysis of Type 4 secretion system clusters in Burkholderia species.

Three clusters with a unique gene organization have the characteristic VirB and VirD4 proteins found in the Agrobacterium tumefaciens cluster. A fourth, truncated cluster (yellow) is also found in many Burkholderia strains, including B. tuberum STM678T, but is unlikely to contribute to secretion.

doi:10.1371/journal.pone.0083779.g003

The Burkholderia VirB/D4 T4SS loci cluster into four types based on phylogenetic analysis of six concatenated genes, VirB1-6, each with a unique chromosomal arrangement (Fig. 3). B. unamae MTI641T, B. silvatlantica SRMrh20T, and B. silvatlantica PVA5 each contain clusters similar to the B. cenocepacia plasmid mobilization T4SS. B. silvatlantica PVA5 also contains a second arrangement shared with several of the opportunistic and plant pathogen strains, whereas B. tuberum STM678T has only a conserved, but truncated and non-canonical cluster that likely is not involved in secretion (Fig. 3). None of the four symbiotic Burkholderia genomes that we analyzed in detail have orthologs of virAG, the two-component system that regulates the vir operon in A. tumefaciens.

Type 6 secretion system: T6SS regulons are a commonly described feature of virulent bacterial species [42], [43]. Six different T6SS gene clusters have been identified in the B. pseudomallei genome [44] with distinct roles in pathogenesis and survival [45]. T6SS-5 is required for pathogenesis of B. thailandensis, whereas T6SS-1 has been shown to be involved in bacterial cell-cell interactions. Deletion of members of the T6SS-1 cluster leads to cells that are less able to compete with other bacterial cells in biofilms [45]. The other clusters are poorly characterized, but the B. pseudomallei T6SS-4 shows homology with the R. leguminosarum imp region (Fig. 4).

thumbnail

Figure 4. Relationship between the Burkholderia Type 6 secretion systems and arrangement of gene clusters.

Clusters were identified with BLASTP against the B. pseudomallei T6SS-2, and a concatenated neighbor-joining phylogenetic tree was generated in MEGA 5.1 using highly divergent protein sequences–VgrG, Hcp, ClpV, IcmF, and the lysozyme-like protein VC_A0109. The gene arrangements of the cluster were manually verified. Although B. oklahomensis EO147 was found to have five T6SS clusters (Fig. 1), it was excluded from the analysis because the draft quality of the genome sequence did not allow for full reconstruction of the gene arrangement of the operon. The four symbiotic strains emphasized in this study are highlighted in bold. The R. leguminosarum imp region clusters with the T6SS-4 group and is indicated with an asterisk. The T6SSa and TG6SSb clusters are found only in the environmental and symbiotic Burkholderia species.

doi:10.1371/journal.pone.0083779.g004

We performed a phylogenetic analysis of five concatenated protein sequences–VgrG, Hcp, ClpV, IcmF, and VC_A0109, a sequence encoding a lysozyme-like protein that is highly divergent between different strains–from the range of Burkholderia species spanning the pathogenic, environmental, and symbiotic clades identified in Fig. 1 (Fig. 4). All Burkholderia species analyzed had at least one T6SS cluster, but only B. pseudomallei had the full set of six. The other mammalian pathogens namely, B. mallei, B. thailandensis, and B. oklahomensis each had 5 clusters including the pathogenicity-associated T6SS-5, although T6SS-1 was truncated in B. mallei. The environmental and symbiotic species on average have 2 distinct T6SS clusters, but no T6SS-5 cluster (5* in Fig. 1). The phylogenetic clustering of the Burkholderia T6SS operons also identified two new clades with unique cluster arrangements (Fig. 4). These two clusters, here labeled T6SS-a and T6SS-b, are largely found only in the environmental and symbiotic strains. B. tuberum STM678T has three T6SS regulons, including one with homology to B. pseudomallei T6SS-2 and one to T6SS-4. B. unamae MTI641T has two clusters, one similar to T6SS-4, and the unique cluster T6SS-b, whereas B. silvatlantica SRMrh20T and B. silvatlantica PVA5 each have only one cluster, the T6SS-b operon (Fig. 4).

Antibiotic Resistance Assays

Generally, soil bacteria that are opportunistic pathogens are considered to be resistant to multiple antibiotics [1], [46]. For this reason, we examined the antibiotic resistance of several plant-associated and environmental species compared to B. thailandensis E264, B. vietnamiensis G4, and B. gladioli BSR3. Like many pathogenic bacteria, B. thailandensis, exhibited varying ranges of resistance to the antibiotics tested except for chloramphenicol (25 µg/ml), to which it was significantly sensitive. B. thailandensis E264 was completely resistant to ampicillin (100 µg/ml) and erythromycin (15 µg/ml) with a lesser degree of resistance to most of the other antibiotics tested (Fig. 5). The two other members of the B clade [3] tested, B. gladioli BSR3 and B. vietnamiensis G4, demonstrated full resistance to ampicillin, and B. gladioli also exhibited complete resistance to tetracycline (30 µg/ml). Both showed varying resistance to other antibiotics, except for nalidixic acid (25 µg/ml; B. gladioli) and kanamycin (30 µg/ml; B. vietnamiensis). Of the four symbiotic strains tested, all were highly sensitive to many of the antibiotics evaluated. However, several showed resistance to ampicillin, e.g., B. silvatlantica SRMrh20T, which was fully ampicillin-resistant, whereas B. silvatlantica PVA5 showed resistance to nalidixic acid and tetracycline.

thumbnail

Figure 5. Antibiotic-resistance profiles of pathogenic and symbiotic Burkholderia species.

Relative resistance to a panel of antibiotics for the four environmental and symbiotic strains emphasized in this study compared to the pathogenic B. thailandensis E264, the opportunistic pathogen B. vietnamiensis G4, and the plant pathogen B. gladioli BSR3. The average clearing of five replicate experiments at the highest antibiotic concentration are represented in the heat map. Full resistance (no clearing) is indicated with an asterisk.

doi:10.1371/journal.pone.0083779.g005

Functional Assays

Symbiotic Burkholderia species are not pathogenic to the nematode C. elegans: Exposing the model organism C. elegans to bacterial strains is frequently used to assess the severity of bacterial pathogenesis [47], [48]. Using the “slow killing” assay, we compared the effects of the standard nematode food source, E. coli OP50 to B. thailandensis E264, as well as to a number of Burkholderia species from the A group (Fig. 6). A recently isolated plant growth-promoting bacterial (PGPB) species, Bacillus simplex 237, from the Negev Desert [23], had been shown to be avirulent and was used as a control (data not shown). A preliminary test using two P. aeruginosa stains demonstrated that nematode death was evident within 48 h (data not shown).

thumbnail

Figure 6. Symbiotic Burkholderia species are not pathogenic in vitro to the nematode C. elegans using the slow-killing assay.

The edge of bacterial lawns of test Burkholderia strains were seeded with age-synchronized C. elegans N2 juvenile worms on nematode growth agar (NGM) plates. An initial count of live worms was made, and again after 24, 48, and 72 h. The percent of survivors were enumerated based on a comparison of live worms present after 72 h versus the initial count. Four symbiotic species of Burkholderia (B. tuberum STM678T, B. silvatlantica PVA5, B. silvatlantica SRMrh20T, B. unamae MTI641T) and one pathogenic species (B. thailandensis E264) were compared against the control, E coli OP50. Only the pathogenic species showed a significant and dramatic reduction in the number of live worms over the course of the experiments. All other test strains showed nearly 100% survival. Data from 48 h after the start of the experiment are shown. Error bars indicate standard error.

doi:10.1371/journal.pone.0083779.g006

Bacterial pathogenesis was assessed by the percent survival of nematodes after 48 h of exposure to the bacterial lawn. When placed on lawns of the control or symbiotic strains, the nematodes were active inside the bacterial lawn. They grew and laid eggs, continuing their normal life cycle as they consumed the bacteria. In contrast, nematodes placed in the B. thailandensis E264 lawn remained around the periphery of the lawn and became immobile. Many nematodes died within the first 24 h in response to B. thailandensis E264, but a few survived up to 24 h after the start of the experiment, and all were dead after 72 h. The exact cause of death may have been due to either direct toxicity of the pathogen to the nematode or starvation from avoiding the only food provided. Further studies regarding the mechanism of pathogenesis is of interest, but beyond the scope of this study.

The symbiotic Burkholderia species are a preferred food source over B. thailandensis E264 for C. elegans: Because we observed that the nematodes avoided the pathogenic B. thailandensis E264, we designed a “competition” experiment to determine whether chemical attractants played a role in pathogenesis. In earlier studies [49], [50], prior diet and the secretion of bacterial volatile compounds were shown to influence the choice of food for C. elegans. Most notably, nematodes avoid pathogenic bacteria when offered a preferred nutritional source, such as E. coli. If given a choice between two different bacterial lawns, the nematodes consistently avoided B. thailandensis E264 and chose the symbiotic Burkholderia species or E. coli (Fig. 7). Although the B. thailandensis E264 lawns were devoid of C. elegans, track marks were visible demonstrating that the nematodes explored the lawns before choosing the other food source. Within 24 h, the nematodes were active in the symbiotic Burkholderia lawn or surrounding agar surface. From these experiments, we concluded that the nematodes avoided the pathogenic Burkholderia species and were attracted to and fed upon the symbiotic species, where they were active and able to reproduce. This experiment provided evidence indicating the lack of pathogenesis in the symbiotic species towards this invertebrate model.

thumbnail

Figure 7. Symbiotic Burkholderia species are the preferred nutritional source of C. elegans compared to a pathogenic species.

E. coli and symbiotic Burkholderia species were individually compared to B. thailandensis E264 to examine the response of the nematode C. elegans to a nutritional preference. Live worms were age-synchronized and seeded into the center of a nematode growth agar (NGM) plate equidistant from a lawn of B. thailandensis E264 and the aforementioned non-pathogenic strains. Counts of live worms were taken initially after seeding, and at 24, 48, and 72 h intervals. In each competition assay, the B. thailandensis lawn was either avoided or contained mostly dead worms, whereas live worms thrived within the lawns of E. coli OP50 or symbiotic Burkholderia species. Error bars indicate standard error.

doi:10.1371/journal.pone.0083779.g007

Symbiotic Burkholderia species are not pathogenic to mammalian cells in vitro: To expand our understanding of the host-microbe interactions of symbiotic Burkholderia species, we investigated whether the symbiotic species were toxic to mammalian cells in culture. Pathogenic bacteria invade eukaryotic cells causing cells to lyse via mechanical injury and/or toxin secretion. Either mechanism results in a release of cellular components into the surrounding environment as well as morphological changes in cell structure and attachment to neighboring cells and the culture surface.

To address the capacity of symbiotic Burkholderia to exert common pathogenic strategies on mammalian cells, we performed cytotoxicity assays on HeLa cells. After 8 or 24 h of incubation, cellular toxicity was assessed with quantification of LDH release and microscopic analysis (Fig. 8; Fig. S2). Initially (8 h post-inoculation), LDH release was two-fold greater for cells infected with B. thailandensis E264 compared to symbiotic Burkholderia, which showed levels slightly above baseline. By 24 h post-inoculation, the HeLa cells were completely cleared by B. thailandensis E264, at LDH release levels higher than cells treated with detergent. Microscopic observation showed that HeLa cells rounded up and did not maintain an intact monolayer. In addition, significant bacterial replication had taken place within the rounded-up cells. However, HeLa cells inoculated with symbiotic Burkholderia species were similar in appearance to uninfected cells (Fig. S2). Taken together, these results suggest that the symbiotic species are not harmful to mammalian cells in vitro.

thumbnail

Figure 8. Symbiotic Burkholderia species are not toxic to HeLa cells in culture.

Symbiotic Burkholderia species (B. tuberum STM678T, B. silvatlantica PVA5, B. silvatlantica SRMrh20T, B. unamae MTI641T) were compared to B. thailandensis E264 to determine if they were toxic to mammalian cells grown in culture. HeLa cells were grown until confluent and inoculated with an MOI of 50. After 8 and 24 h, samples of the supernatant of the inoculated and sham-inoculated cells were examined for LDH release using the Cyto-Tox 96 assay kit and spectrophotometric reading at 490 nm. At 8 h, only the positive control cells treated with detergent showed significant cell lysis. B. thailandensis E264 caused cell lysis about three times greater than that of the negative control (medium only). The effect of the symbiotic species was not statistically different from that of the negative control. At 24 h, B. thailandensis E264-induced morbidity had surpassed the detergent control, while the cytotoxicity caused by the symbiotic species increased only slightly from the earlier time point. Error bars indicate standard error.

doi:10.1371/journal.pone.0083779.g008

Discussion

The genus Burkholderia is a large group of bacteria composed of more than 70 species living in diverse habitats. Many of these have recently been discovered to be associated with plants either as diazotrophs or plant growth-promoting bacteria [51]. Because Burkholderia spp. are generally thought of as disease-causing agents, several authors have advocated that Burkholderia species not be used as inocula for plants [13], . Our aim in this report is to demonstrate that the two major phylogenetic groups of Burkholderia comprise distinct lineages, not only as previously shown by analyzing 16S rRNA and other gene phylogenies, but also by examining the Burkholderia genomes for virulence determinants as well as by using functional tests to determine pathogenicity.

Burkholderia pathogenesis is mediated by a number of virulence loci controlling different aspects of the progression of virulence from attachment, invasion, endosome escape, intracellular motility, formation of multinucleate giant cells, and cellular toxicity [19]. Many microbial virulence loci are under the control of quorum sensing (QS) systems, and AHL-mediated QS has been shown to be important in Burkholderia pseudomallei virulence [52], [53]. Although QS systems are widespread throughout Burkholderia, pathogens and opportunistic pathogens have much more complex QS systems than the symbiotic and environmental species [54]. The BraI/R QS systems among species in the A group are highly similar to each other (>75%) and cluster in a clade distinct from that of the pathogenic B group, which also has multiple QS systems.

Our bioinformatics analysis of the phylogenetic distribution of other major virulence loci across the genus Burkholderia shows that significant differences exist between the A and B clades (as defined by [3]). In particular, we analyzed the distribution of Type 3, 4, and 6 secretion systems across species of Burkholderia and found large differences across the different clades. T3SS have been shown to be necessary for pathogenesis in a number of organisms, including intracellular pathogens such as Salmonella, Shigella, and B. pseudomallei. Across Burkholderia, T3SS operons are found primarily in the true and opportunistic pathogens. Very few environmental and symbiotic strains contain T3SS operons, and of those that do, none have the T3SS-3 sequences most highly associated with virulence. For example, although B. phytofirmans PsJN harbors T3SS sequences, C. elegans worms were not affected by this strain in the slow-killing assay nor did HeLa cells lyse in response to bacterial inoculation (A.A. Angus, A. Sessitsch, and A.M. Hirsch, unpublished results). These results are consistent with the lack of the cell invasion genes in this T3SS (Fig. S1).

The T4SS is involved in a wide range of virulence-associated behaviors, including conjugative transfer of DNA, release of DNA molecules into the environment, DNA uptake and transformation, and the translocation of effector molecules to target cells. The T4SS was originally discovered in the plant pathogen Agrobacterium tumefaciens, where it transfers the T-DNA region responsible for transforming normal plant tissues into a crown gall or hairy root. The core A. tumefaciens T4SS channel is composed of 11 VirB proteins and the nucleoside triphosphatase VirD4. In Burkholderia, the T4SS is absent from the B. pseudomallei group, but was present in multiple copies in environmental strains. However, the T4SS operon in the B. tuberum genome was truncated and divergent in sequence from bona fide T4SS.

Although T6SS regulons are a commonly described feature from virulent bacterial species [44], one of the earliest discoveries of this assembly of genes was from the nodulating alpha-proteobacterium, Rhizobium leguminosarum strain RBL5523 [55], [56]. Normally, strain RBL5523 induces the formation of uninfected nodules on pea whereas it effectively nodulates vetch [55]. A Tn5 insertion into a gene (called impJ for the “impaired in nitrogen fixation phenotype”) of a group of 14 genes led instead to an effective (Fix+) nodule phenotype on pea [55]. The effect on nodulation was temperature-dependent and correlated with the secretion of four isozymes into the supernatant of the wild-type bacterial culture after growth at a higher temperature [56]. All Burkholderia genomes analyzed contained at least one T6SS operon, with most having multiple clusters and B. pseudomallei having six. None of the environmental and symbiotic strains have the T6SS-5 cluster associated with virulence in the pathogenic Burkholderia, and the T6SS operons of several non-pathogenic strains also cluster into two distinct clades with different gene arrangements than the six clusters of B. pseudomallei.

Regarding flagella and chemotaxis, pathogenic species often have genes for two flagellar systems, one of which is employed for swimming through liquids, whereas the other is used for swarming over surfaces or within viscous environments [57]. Recently, genetic knockouts paired with photothermal nanoblade delivery of B. thailandensis directly into the cytoplasm of mammalian cells identified a second flagellar gene cluster on chromosome 2, which is responsible for the intracellular motility required for cell-cell spread and infection progression [32]. A second motility system was not identified in the members of the A group.

Pathogenic Burkholderia species are frequently resistant to multiple antibiotics, and B. thailandensis E264 replicates this behavior, showing resistance to a broad spectrum of antibiotics (Fig. 5). By contrast, the symbiotic and environmental members of the A group were susceptible to the vast majority of antibiotics tested. In addition to being susceptible to most antibiotics, we earlier showed that B. tuberum was incapable of growing at 37°C and 40°C [58] when plated during the early growth phases. These are temperatures at which pathogenic microbes frequently grow, but nonpathogenic species do not [59]. Although stationary phase B. tuberum cultures were more tolerant of higher temperatures (unpublished), the bacterial cells took 4 days to recover from the high temperatures due to their slow growth. These results strongly suggest that the symbiotic species are not adapted to living at mammalian temperatures.

C. elegans has been employed in a number of earlier investigations to be an excellent model for testing whether similar or even identical functions are responsible for virulence in humans [47], [48]. Our functional analysis demonstrated that the four symbiotic strains highlighted in this study did not kill C. elegans. In contrast, B. thailandensis E264 was very effective in the slow-killing assay. Moreover, if given a choice between B. thailandensis and any of the symbiotic species for food, the nematodes always choose the latter, and reproduced under these conditions. Similarly, B. thailandensis E264 started to lyse HeLa cells as soon as 8 h after treatment, with the cells showing significant damage after 24 h. In contrast, the symbiotic species did not cause lysis and under the microscope, the cells incubated with bacteria from the A group were identical in appearance to uninfected cells. These results strongly indicate that the symbiotic species lack the virulence determinants that are required for killing HeLa cells.

Taken together, these data demonstrate that the symbiotic and environmental Burkholderia species are highly unlikely to be pathogenic to mammals based on both functional and genomic data. Furthermore, the presence of pathogenic strains in the same taxonomic genus is not an accurate predictor of the presence of virulence loci in the genomes of other members of the genus or of virulence to animal cells in vitro. Notably, a parallel situation exists in the more commonly used agricultural alpha-rhizobia strains (Rhizobiaceae and Bradyrhizobiaceae), yet few concerns are raised regarding the use of these bacteria as inoculants. Rhizobium (formerly Agrobacterium) radiobacter has been isolated from respiratory secretions of CF patients [60] and reported as causing bacteremia in cancer patients [61], [62], among other conditions (cited in the previous papers). Kuykendall et al. [63] compared the chromosomes of several bacteria from three families, Rhizobiaceae, Bartonellaceae, and Bradyrhizobiaceae, and found genome blocks with highly conserved genes as well as genes encoding proteins that were characteristic of either a symbiotic or parasitic lifestyle. Even though Sinorhizobium meliloti is the closest known relative of ‘Candidatus Liberibacter asiaticus’, the causative agent of citrus greening disease, little overall synteny was observed between the chromosomes of the two species. A similar result was found for all five members of the Rhizobiales although microsyntenous blocks that encode core functions were detected [63]. The bottom line is that different clusters of genes and different G+C content of genomes correlate with either the symbiotic or parasitic lifestyle in the Rhizobiaceae [63].

For the Bradyrhizobiaceae, the genus Apifia causes nosocomial infections and based on 16S RNA phylogeny, is related to several Bradyrhizobium spp. that are used as inocula for plants [64]. The provisionally named Bradyrhizobium enterica has recently been isolated from two patients with cord colitis and a draft genome was assembled [65]. Its closest relative based on an analysis of a subset of 400 core genes is Bradyrhizobium japonicum USDA 110, albeit supported by a very low bootstrap value. Moreover, no evidence yet exists to show that Bradyrhizobium enterica is the definitive cause of cord colitis.

The situation described for the Rhizobiaceae and Bradyrhizobiaceae resembles that of the Burkholderiaceae in that pathogenic species are grouped together with symbiotic and beneficial species. However, in the past, the names of the genera for the nitrogen-fixing and environmental species versus the pathogens differed in Rhizobiaceae and Bradyrhizobiaceae, but recent evidence demonstrates that Rhizobium and Bradyrhizobium also contain opportunistic human pathogens. The situation is the same for the genus Burkholderia, which encompasses bacteria expressing a number of diverse lifestyles. However, using MLSA [3], we could show that the B clade consists of opportunistic, plant, and mammalian pathogens as well as some environmental strains, whereas the A clade contains environmental and symbiotic species. The lack of virulence determinants in the A clade genomes studied herein as well as the differences in behavior observed between symbiotic and pathogenic Burkholderia species lends even more support to the separation of the A group from the B clade and the delineation of each as distinct genera. In addition, it suggests the potential for safe application of the plant-associated Burkholderia species in an agricultural context, especially for promoting crop growth in acidic, arid soils.

Supporting Information

Figure S1.

Gene arrangement of the three Type 3 secretion system clusters in B. pseudomallei K96243 and a fourth type of cluster present only in the environmental strains B. phytofirmans PsJN and B. xenovorans LB400.

doi:10.1371/journal.pone.0083779.s001

(TIFF)

Figure S2.

Disruption of mammalian cell integrity does not occur upon inoculation with the symbiotic Burkholderia species. Images of HeLa cells inoculated with pathogenic or symbiotic species were visualized at 24 h. Only cells inoculated with B. thailandensis E264 showed cell rounding and clumping. Cells inoculated with symbiotic species appeared similar to those that were sham-inoculated with medium only. Magnification, 1000×.

doi:10.1371/journal.pone.0083779.s002

(TIFF)

Acknowledgments

We thank Dr. Imke Schroeder and Dr. C. Todd French (UCLA) for their help in annotating the genes of the T6SS in the plant-associated species and advice about pathogenic loci in Burkholderia, respectively. The Alex van der Bliek lab (UCLA) is acknowledged for providing the C. elegans N2 stock and the Alison Frand lab (UCLA) for assistance with imaging analysis of C. elegans. We thank Chelsea Hu for assistance with the bioinformatics analysis and Dr. Stefan J. Kirchanski for his comments on the manuscript.

Author Contributions

Conceived and designed the experiments: AAA CMA AMH. Performed the experiments: AAA CMA SF. Analyzed the data: CMA AAA AMH SY PES PY NS SK. Contributed reagents/materials/analysis tools: CMA AAA AMH JCM SMdF FDD GW. Wrote the paper: AAA CMA AMH FDD PES. For his pioneering research on the Symbiotic Burkholderia species: JCM.

References

  1. 1. Berg G, Eberl L, Hartmann A (2005) The rhizosphere as a reservoir for opportunistic human pathogenic bacteria. Environ Microbiol 7: 1673–1685. doi: 10.1111/j.1462-2920.2005.00891.x
  2. 2. Suárez-Moreno ZR, Caballero-Mellado J, Coutinho BG, Mendoça-Previato L, James EK, et al. (2012) Common features of environmentally and potentially beneficial plant-associated Burkholderia. Microb Ecol 63: 249–266. doi: 10.1007/s00248-011-9929-1
  3. 3. Estrada-de los Santos P, Vinuesa P, Martínez-Aguilar L, Hirsch AM, Caballero-Mellado J (2013) Phylogenetic analysis of Burkholderia species by Multilocus Sequence Analysis. Curr Microbiol 67: 51–60. doi: 10.1007/s00284-013-0330-9
  4. 4. Yabuuchi E, Kosako Y, Oyaizu H, Yano I, Hotta H, et al. (1992) Proposal of Burkholderia gen. nov. and transfer of seven species of the genus Pseudomonas homology group II to the new genus, with the type species Burkholderia cepacia (Palleroni and Holmes 1981) comb. nov. Microbiol Immunol 36: 1251–1275. doi: 10.1111/j.1348-0421.1992.tb02129.x
  5. 5. Yabuuchi E, Kosako Y, Yano I, Hotta H, Nishiuchi Y (1995) Transfer of two Burkholderia and an Alcaligenes species to Ralstonia gen. Nov.: Proposal of Ralstonia pickettii (Ralston, Palleroni and Doudoroff 1973) comb. Nov., Ralstonia solanacearum (Smith 1896) comb. Nov. and Ralstonia eutropha (Davis 1969) comb. Nov. Microbiol Immunol 39: 897–904. doi: 10.1111/j.1348-0421.1995.tb03275.x
  6. 6. Onofre-Lemus J, Hernández-Lucas I, Girard L, Caballero-Mellado J (2009) ACC (1-aminocyclopropane-1-carboxylate) deaminase activity, a widespread trait in Burkholderia species, and its growth-promoting effect on tomato plants. Appl Environ Microbiol 75: 6581–6590. doi: 10.1128/aem.01240-09
  7. 7. Payne GW, Vandamme P, Morgan SH, LiPuma JJ, Coenye T, et al. (2005) Development of a recA gene-based identification approach for the entire Burkholderia genus. Appl Environ Microbiol 71: 3917–3927. doi: 10.1128/aem.71.7.3917-3927.2005
  8. 8. Perin L, Martinez-Aguilar L, Castro-Gonzalez R, Estrada-de Los Santos P, Cabellos-Avelar T, et al. (2006) Diazotrophic Burkholderia species associated with field-grown maize and sugarcane. Appl Environ Microbiol 72: 3103–3110. doi: 10.1128/aem.72.5.3103-3110.2006
  9. 9. Baldwin A, Sokol PA, Parkhill J, Mahenthiralingam E (2004) The Burkholderia cepacia epidemic strain marker is part of a novel genomic island encoding both virulence and metabolism-associated genes in Burkholderia cenocepacia. Infect Immun 72: 1537–1547. doi: 10.1128/iai.72.3.1537-1547.2004
  10. 10. Gyaneshwar P, Hirsch AM, Moulin L, Chen WM, Elliott GN, et al. (2011) Legume-nodulating betaproteobacteria: diversity, host range, and future prospects. Mol Plant Microbe Interact 24: 1276–1288. doi: 10.1094/mpmi-06-11-0172
  11. 11. O'sullivan LA, Weightman AJ, Jones TH, Marchbank AM, Tiedje JM, et al. (2007) Identifying the genetic basis of ecologically and biotechnologically useful functions of the bacterium Burkholderia vietnamiensis. Environ Microbiol 9: 1017–1034. doi: 10.1111/j.1462-2920.2006.01228.x
  12. 12. de Los Santos-Villalobos S, Barrera-Galicia GC, Miranda-Salcedo MA, Peña-Cabriales JJ (2012) Burkholderia cepacia XXVI siderophore with biocontrol capacity against Colletotrichum gloeosporioides. World J Microbiol Biotechnol 28: 2615–2623. doi: 10.1007/s11274-012-1071-9
  13. 13. Holmes A, Govan J, Goldstein R (1998) Agricultural use of Burkholderia (Pseudomonas) cepacia: a threat to human health? Emerg Infect Diseases 4: 221–227. doi: 10.3201/eid0402.980209
  14. 14. Torbeck L, Raccasi D, Guilfoyle DE, Friedman RL, Hussong D (2011) Burkholderia cepacia: this decision is overdue. PDA J Pharm Sci Technol 65: 535–543. doi: 10.5731/pdajpst.2011.00793
  15. 15. Magalhães M, de Britto MCA, Vandamme P (2002) Burkholderia cepacia genomovar III and Burkholderia vietnamiensis double infection in a cystic fibrosis child. J Cyst Fibros 1: 292–294. doi: 10.1016/s1569-1993(02)00101-7
  16. 16. Chiarini L, Bevivino A, Dalmastri C, Tabacchioni S, Visca P (2006) Burkholderia cepacia complex species: health hazards and biotechnological potential. Trends Microbiol 14: 277–286. doi: 10.1016/j.tim.2006.04.006
  17. 17. U.S. Environmental Protection Agency (2003) Burkholderia cepacia Complex; Significant New Use Rule. Federal Register 68: 35315–35320 Available: http://www.epa.gov/fedrgstr/EPA-TOX/2003​/June/Day-13/t15010.htm.
  18. 18. Sanchez PA (2010) Tripling crop yields in tropical africa. Nature Geosci 3: 299–300. doi: 10.1038/ngeo853
  19. 19. Galyov EE, Brett PJ, DeShazer D (2010) Molecular insights into Burkholderia pseudomallei and Burkholderia mallei pathogenesis. Annu Rev Microbiol 64: 495–517. doi: 10.1146/annurev.micro.112408.134030
  20. 20. Tamura K, Peterson D, Peterson N, Stecher G, Nei M, et al. (2011) MEGA5: Molecular Evolutionary Genetics Analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol 28: 2731–2739. doi: 10.1093/molbev/msr121
  21. 21. Haraga A, West TE, Brittnacher MJ, Skerrett SJ, Miller SI (2008) Burkholderia thailandensis as a model system for the study of the virulence-associated Type III secretion system of Burkholderia pseudomallei. Infect Immun 76: 5402–5411. doi: 10.1128/iai.00626-08
  22. 22. Reinke SN, Hu X, Sykes BD, Lemire BD (2010) Caenorhabditis elegans diet significantly affects metabolic profile, mitochondrial DNA levels, lifespan and brood size. Mol Gen Metab 100: 274–282. doi: 10.1016/j.ymgme.2010.03.013
  23. 23. Kaplan D, Maymon M, Agapakis CM, Lee A, Wang A, et al.. (2013) A survey of the microbial community in the rhizosphere of two dominant shrubs of the Negev Desert highlands, Zygophyllum dumosum (Zygophyllaceae) and Atriplex halimus (Amaranthaceae) using cultivation-dependent and -independent methods. Amer J Bot, doi:10.3732/ajb.1200615.
  24. 24. Bauer AW, Kirby WM, Sherris JC, Turck M (1966) Antibiotic susceptibility testing by a standardized single disk method. Am J Clin Pathol 45: 493–496.
  25. 25. Stiernagle T (2006) Maintenance of C. elegans. WormBook: 1–11.
  26. 26. Wiersinga WJ, van der Poll T, White NJ, Day NP, Peacock SJ (2006) Melioidosis: insights into the pathogenicity of Burkholderia pseudomallei. Nat Rev Micro 4: 272–282. doi: 10.1038/nrmicro1385
  27. 27. Reckseidler-Zenteno SL, DeVinney R, Woods DE (2005) The capsular polysaccharide of Burkholderia pseudomallei contributes to survival in serum by reducing complement factor C3b deposition. Infect Immun 73: 1106–1115. doi: 10.1128/iai.73.2.1106-1115.2005
  28. 28. Essex-Lopresti AE, Boddey JA, Thomas R, Smith MP, Hartley MG, et al. (2005) A type IV pilin, PilA, contributes to adherence of Burkholderia pseudomallei and virulence in vivo. Infect Immun 73: 1260–1264. doi: 10.1128/iai.73.2.1260-1264.2005
  29. 29. Holden MTG, Titball RW, Peacock SJ, Cerdeño-Tárraga AM, Atkins T, et al. (2004) Genomic plasticity of the causative agent of melioidosis, Burkholderia pseudomallei. Proc Natl Acad Sci USA 101: 14240–14245. doi: 10.1073/pnas.0403302101
  30. 30. DeShazer D, Brett PJ, Carlyon R, Woods DE (1997) Mutagenesis of Burkholderia pseudomallei with Tn5-OT182: isolation of motility mutants and molecular characterization of the flagellin structural gene. J Bacteriol 179: 2116–2125.
  31. 31. Chua KL, Chan YY, Gan YH (2003) Flagella are virulence determinants of Burkholderia pseudomallei. Infect Immun 71: 1622–1629. doi: 10.1128/iai.71.4.1622-1629.2003
  32. 32. French CT, Toesca IJ, Wu T-H, Teslaa T, Beaty SM, et al. (2011) Dissection of the Burkholderia intracellular life cycle using a photothermal nanoblade. Proc Natl Acad Sci USA 108: 12095–12100. doi: 10.1073/pnas.1107183108
  33. 33. Urban TA, Griffith A, Torok AM, Smolkin ME, Burns JL, et al. (2004) Contribution of Burkholderia cenocepacia flagella to infectivity and inflammation. Infect Immun 72: 5126–5134. doi: 10.1128/iai.72.9.5126-5134.2004
  34. 34. Whitlock GC, Mark Estes D, Torres AG (2007) Glanders: off to the races with Burkholderia mallei. FEMS Microbiol Lett 277: 115–122. doi: 10.1111/j.1574-6968.2007.00949.x
  35. 35. de Oliveira Cunha C, Goda Zuleta LF, Paula de Almeida LG, Prioli Ciapina L, Lustrino Borges W, et al. (2012) Complete genome sequence of Burkholderia phenoliruptrix BR3459a (CLA1), a heat-tolerant, nitrogen-fixing symbiont of Mimosa flocculosa. J Bacteriol 194: 6675–6676. doi: 10.1128/jb.01821-12
  36. 36. Mitter B, Petric A, Shin MW, Chain PS, Hauberg-Lotte L, et al. (2013) Comparative genome analysis of Burkholderia phytofirmans PsJN reveals a wide spectrum of endophytic lifestyles based on interaction strategies with host plants, Front Plant Sci. 4: 1–15 doi:10.3389/fpls.2013.00120/abstract.
  37. 37. Chain PS, Denef VJ, Konstantinidis KT, Vergez LM, Agulló L, et al. (2006) Burkholderia xenovorans LB400 harbors a multi-replicon, 9.73-Mbp genome shaped for versatility. Proc Natl Acad Sci USA 108: 15280–15287.. doi: 10.1073/pnas.0606924103
  38. 38. Schmidt MA, Balsanelli E, Faoro H, Cruz LM, Wassem R, et al.. (2012) The type III secretion system is necessary for the development of a pathogenic and endophytic interaction between Herbaspirillum rubrisubalbicans and Poaceae. BMC Microbiol 12: doi:10.1186/1471-2180-12-98.
  39. 39. Backert S, Meyer TF (2006) Type IV secretion systems and their effectors in bacterial pathogenesis. Curr Opin Microbiol 9: 207–217. doi: 10.1016/j.mib.2006.02.008
  40. 40. Cascales E, Christie PJ (2003) The versatile bacterial type IV secretion systems. Nat Rev Micro 1: 137–149. doi: 10.1038/nrmicro753
  41. 41. Zhang R, LiPuma JJ, Gonzalez CF (2009) Two type IV secretion systems with different functions in Burkholderia cenocepacia K56-2. Microbiology 155: 4005–4013. doi: 10.1099/mic.0.033043-0
  42. 42. Schwarz S, Hood RD, Mougous JD (2010) What is type VI secretion doing in all those bugs? Trends Microbiol 18: 531–537. doi: 10.1016/j.tim.2010.09.001
  43. 43. Bingle LE, Bailey CM, Pallen MJ (2008) Type VI secretion: a beginner's guide. Curr Opin Microbiol 11: 3–8. doi: 10.1016/j.mib.2008.01.006
  44. 44. Boyer F, Fichant G, Berthod J, Vandenbrouck Y, Attree I (2009) Dissecting the bacterial type VI secretion system by a genome wide in silico analysis: what can be learned from available microbial genomic resources? BMC Genomics 10: 104. doi: 10.1186/1471-2164-10-104
  45. 45. Schwarz S, West TE, Boyer F, Chiang W-C, Carl MA, et al. (2010) Burkholderia Type VI secretion systems have distinct roles in eukaryotic and bacterial cell interactions. PLoS Pathog 6: e1001068. doi: 10.1371/journal.ppat.1001068
  46. 46. Riesenfeld CS, Goodman RM, Handelsman J (2004) Uncultured soil bacteria are a reservoir of new antibiotic resistance genes. Environ Microbiol 6: 981–989. doi: 10.1111/j.1462-2920.2004.00664.x
  47. 47. Tan MW, Mahajan-Miklos S, Ausubel FM (1999) Killing of Caenorhabditis elegans by Pseudomonas aeruginosa used to model mammalian bacterial pathogenesis. Proc Natl Acad Sci USA 96: 715–720. doi: 10.1073/pnas.96.2.715
  48. 48. Zachow C, Pirker H, Westendorf C, Tilcher R, Berg G (2009) The Caenorhabditis elegans assay: a tool to evaluate the pathogenic potential of bacterial biocontrol agents. Euro Plant Path 125: 367–376. doi: 10.1007/s10658-009-9486-3
  49. 49. Niu Q, Huang X, Zhang L, Xu J, Yang D, et al. (2010) A Trojan horse mechanism of bacterial pathogenesis against nematodes. Proc Natl Acad Sci USA 107: 16631–16636. doi: 10.1073/pnas.1007276107
  50. 50. Cooper VS, Carlson WA, LiPuma JJ (2009) Susceptibility of Caenorhabditis elegans to Burkholderia infection depends on prior diet and secreted bacterial attractants. PLoS ONE 4: e7961. doi: 10.1371/journal.pone.0007961
  51. 51. Gyaneshwar P, Kumar GN, Parekh L (2002) Role of soil microorganisms in improving P nutrition of plants. Plant Soil 245: 83–93. doi: 10.1023/a:1020663916259
  52. 52. Ulrich RL, DeShazer D, Brueggemann EE, Hines HB, Oyston PC, et al. (2004) Role of quorum sensing in the pathogenicity of Burkholderia pseudomallei. J Med Microbiol 53: 1053–1064. doi: 10.1099/jmm.0.45661-0
  53. 53. Valade E, Thibault FM, Gauthier YP, Palencia M, Popoff MY, et al. (2004) The PmlI-PmlR quorum-sensing system in Burkholderia pseudomallei plays a key role in virulence and modulates production of the MprA protease. J Bacteriol 186: 2288–2294. doi: 10.1128/jb.186.8.2288-2294.2004
  54. 54. Suarez-Moreno ZR, Caballero-Mellado J, Venturi V (2008) The new group of non-pathogenic plant-associated nitrogen-fixing Burkholderia spp. shares a conserved quorum-sensing system, which is tightly regulated by the RsaL repressor. Microbiology 154: 2048–2059. doi: 10.1099/mic.0.2008/017780-0
  55. 55. Roest HP, Mulders IHM, Spaink HP, Wijffelman CA, Lugtenberg BJJ (1997) A Rhizobium leguminosarum biovar trifolii locus not localized on the sym plasmid hinders effective nodulation on plants of the pea cross-inoculation group. Mol Plant Microbe Interact 10: 938–941. doi: 10.1094/mpmi.1997.10.7.938
  56. 56. Bladergroen MR, Badelt K, Spaink HP (2003) Infection-blocking genes of a symbiotic Rhizobium leguminosarum strain that are involved in temperature-dependent protein secretion. Mol Plant Microbe Interact 16: 53–64. doi: 10.1094/mpmi.2003.16.1.53
  57. 57. McCarter LL (2004) Dual flagellar systems enable motility under different circumstances. J Mol Microbiol Biotechnol 7: 18–29. doi: 10.1159/000077866
  58. 58. Angus AA, Lee A, Lum MR, Shehayeb M, Hessabi R, et al. (2013) Nodulation and effective nitrogen fixation of Macroptilium atropurpureum (siratro) by Burkholderia tuberum, a nodulating and plant growth promoting beta-proteobacterium, are influenced by environmental factors. Plant Soil 369: 543–562. doi: 10.1007/s11104-013-1590-7
  59. 59. Araujo R, Rodrigues AG (2004) Variability of germinative potential among pathogenic species of Aspergillus. J Clin Microbiol 42: 4335–4337. doi: 10.1128/jcm.42.9.4335-4337.2004
  60. 60. Coenye T, Goris J, Spilker T, Vandamme P, LiPuma JJ (2002) Characterization of unusual bacteria isolated from respiratory secretions of cystic fibrosis patients and description of Inquilinus limosus gen. nov., sp. nov. J Clin Microbiol 40: 2062–2069. doi: 10.1128/jcm.40.6.2062-2069.2002
  61. 61. Paphitou NI, Rolston KVI (2003) Catheter-related bacteremia caused by Agrobacterium radiobacter in a cancer patient: case report and literature review. Infection 31: 421–424.
  62. 62. Chen CY, Hansen KS, Hansen LK (2008) Rhizobium radiobacter as an opportunistic pathogen in central venous catheter-associated bloodstream infection: case report and review. J Hosp Infect 68: 203–207. doi: 10.1016/j.jhin.2007.11.021
  63. 63. Kuykendall LD, Shao JY, Hartung JS (2012) Conservation of gene order and content in the circular Chromosomes of “Candidatus Liberibacter asiaticus” and other Rhizobiales. PLoS ONE 7: e34673. doi: 10.1371/journal.pone.0034673
  64. 64. La Scola B (2002) Description of Afipia birgiae sp. nov. and Afipia massiliensis sp. nov. and recognition of Afipia felis genospecies A. Int J Syst Evol Microbiol 52: 1773–1782. doi: 10.1099/ijs.0.02149-0
  65. 65. Bhatt AS, Freeman SS, Herrera AF, Pedamallu CS, Gevers D, et al. (2013) Sequence-based discovery of Bradyrhizobium enterica in cord colitis syndrome. N Engl J Med 369: 517–528. doi: 10.1056/nejmoa1211115
  66. 66. Caballero-Mellado J, Martinez-Aguilar L, Paredes-Valdez G, Estrada-de los Santos P (2004) Burkholderia unamae sp. nov., a N2-fixing rhizospheric and endophytic species. Int J Syst Evol Microbiol 54: 1165–1172. doi: 10.1099/ijs.0.02951-0
  67. 67. Seo Y-S, Lim J, Choi BS, Kim H, Goo E, et al. (2011) Complete genome sequence of Burkholderia gladiolii BSR3. J Bact 193: 3149 doi: 10.1128/JB.00420-11.