Scholarly article on topic ' A Novel Glycolipid Biosurfactant Confers Grazing Resistance upon Pantoea ananatis BRT175 against the Social Amoeba Dictyostelium discoideum '

A Novel Glycolipid Biosurfactant Confers Grazing Resistance upon Pantoea ananatis BRT175 against the Social Amoeba Dictyostelium discoideum Academic research paper on "Biological sciences"

Share paper
Academic journal
OECD Field of science

Academic research paper on topic " A Novel Glycolipid Biosurfactant Confers Grazing Resistance upon Pantoea ananatis BRT175 against the Social Amoeba Dictyostelium discoideum "


Applied and Environmental Science

| CrossMark

' ^-dlckfbr updates

A Novel Glycolipid Biosurfactant Confers Grazing Resistance upon Pantoea ananatis BRT175 against the Social Amoeba Dictyostelium discoideum

Derek D. N. Smith,3 Arvin Nickzad,b £ Eric Déziel,b John Stavrinides3

Department of Biology, University of Regina, Regina, Saskatchewan, Canada"; INRS-Institut Armand-Frappier, Laval, Québec, Canadab

ABSTRACT Pantoea is a versatile genus of bacteria with both plant- and animal-pathogenic strains, some of which have been suggested to cause human infections. There is, however, limited knowledge on the potential determinants used for host association and pathogenesis in animal systems. In this study, we used the model host Dictyostelium discoideum to show that isolates of Pantoea ananatis exhibit differential grazing susceptibility, with some being resistant to grazing by the amoebae. We carried out a high-throughput genetic screen of one grazing-resistant isolate, P. ananatis BRT175, using the D. discoideum pathosystem to identify genes responsible for the resistance phenotype. Among the 26 candidate genes involved in grazing resistance, we identified rhlA and rhlB, which we show are involved in the biosynthesis of a biosurfactant that enables swarming motility in P. ananatis BRT175. Using liquid chromatography-mass spectrometry (LC-MS), the biosurfactant was shown to be a glycolipid with monohexose-C10-C10 as the primary congener. We show that this novel glycolipid biosurfactant is cytotoxic to the amoebae and is capable of compromising cellular integrity, leading to cell lysis. The production of this biosurfactant may be important for bacterial survival in the environment and could contribute to the establishment of opportunistic infections.

IMPORTANCE The genetic factors used for host interaction by the opportunistic human pathogen Pantoea ananatis are largely unknown. We identified two genes that are important for the production of a biosurfactant that confers grazing resistance against the social amoeba Dictyostelium discoideum. We show that the biosur-factant, which exhibits cytotoxicity toward the amoebae, is a glycolipid that incorporates a hexose rather than rhamnose. The production of this biosurfactant may confer a competitive advantage in the environment and could potentially contribute to the establishment of opportunistic infections.

KEYWORDS: biosurfactants, Pantoea, Dictyostelium, opportunistic infections

Received 26 November 2015 Accepted 1

December 2015 Published 20 January 2016 Citation Smith DDN, Nickzad A, DezielE, Stavrinides J. 2016. A novelglycolipid biosurfactant confers grazing resistance upon Pantoea ananatis BRT175 against the social amoeba Dictyostelium discoideum. mSphere 1(1): e00075-15. doi:10.1128/mSphere.00075-15. Editor Katherine McMahon, University of Wisconsin

Copyright © 2016 Smith et al. This is an open-access article distributed under the terms of the Creative Commons Attribution 4.0 Internationallicense.

Address correspondence to John Stavrinides,


c a CD 2


Pantoea is a genus of Gram-negative bacilli in the Enterobacteriaceae and a close relative of human-pathogenic genera Klebsiella and Enterobacter. Pantoea includes epiphytic and pathogenic members that have been identified throughout the environment, including clinical settings. Infections caused by members of Pantoea are known to occur primarily in immunocompromised individuals with preexisting conditions and can result in abscesses, pneumonia, or bacteremia (1-6); however, healthy individuals may be infected through penetrative injury by plant vegetation, which can result in cutaneous infections or develop into septic arthritis (6, 7). More concerning are the clinical cases of fatal bacteremia in neonates caused by contaminated parenteral nutrition as well as bacteremia in immunocompromised adults (1, 3-6, 8). Many members of Pantoea, such as Pantoea ananatis, while considered common environ-

mental microbes, have been suggested to be opportunists with human-pathogenic potential (9, 10).

P. ananatis was originally isolated from pineapple as the causative agent of fruitlet brown rot (11). Many isolates have also been found to cause disease in a wide range of plant species but are also reported to colonize humans opportunistically (9). A study examining virulence potential showed that a P. ananatis pineapple isolate was especially virulent in an embryonated hen egg model compared to five clinical Pantoea agglomerans isolates (12). Similarly, quantitative growth assays have shown that closely related isolates of P. ananatis can vary greatly in their growth potential in plant and insect model hosts (13), suggesting the presence of specific genetic factors that mediate host association (14-16). This has been explored further in a comparative genomics analysis of eight P. ananatis genomes, which determined that isolates readily

exchange genetic factors involved in host- and niche-specific colonization (17). Candi- ^

date disease factors were suggested to include a putative adhesin, multiple type VI o

secretion systems, and even type I fimbriae (17,18). The presence of animal cell-specific l

type III secretion systems has also been noted in several strains, although their §

involvement in host association and specificity is still unclear (19, 20). There is currently limited functional information on these and other genetic factors in this species that may contribute to opportunism and human pathogenicity. O

Model pathosystems are excellent tools for identifying candidate disease factors in 3

pathogenic bacteria. Dictyostelium discoideum has been used as a model host for t

host-pathogen interactions due to its tractability, its similarities to mammalian cells in /

its cellular response to virulence factors, and its ability to phagocytose bacteria (21-25). 3

Resistance to D. discoideum grazing can be used to identify isolates with possible p

virulence potential (26). Pseudomonas aeruginosa and Burkholderia pseudomallei mu- e

tants that are attenuated for virulence in the D. discoideum model are also attenuated 3

in more complex model hosts like fruit flies and mice (22, 25). The D. discoideum s

Q. CD Q.

pathosystem has been used to identify and assess the involvement of a variety of animal-specific virulence factors in host association, including the type VI secretion system, the type III secretion system, and various cytotoxins (25, 27-30). In this study, we used D. discoideum as a model host to screen for genetic factors that may enable 3

P. ananatis to exploit animal hosts. One strain, P. ananatis BRT175, which was shown to u

have a grazing-resistant phenotype, was subjected to a genetic screen to identify the e

genetic determinants involved in resisting D. discoideum feeding. We show that two

genes, rhlA and rhlB, are involved in producing a novel biosurfactant that is cytotoxic ^

to D. discoideum. 1


Qualitative assay identifies grazing-resistant P. ananatis isolates. The grazing u

resistance of 10 phylogenetically characterized P. ananatis isolates (13) was evaluated t

using a qualitative assay in which the plaque formation and sporulation on Esche-richia coli B/r, the standard food source for D. discoideum, were used as a reference (Table 1). Grazing resistance was variable between the P. ananatis isolates and ranged from minimal plaque formation to full plaque formation and sporulation. P. ananatis BRT175 was the most resistant isolate, with minimal plaque formation and no sporulation when challenged with 10,000, 1,000, or 100 D. discoideum cells on modified SM (MSM) agar (Fig. 1). Similarly, P. ananatis M232A, LMG20103, and 15320 also showed a grazing-resistant phenotype with no sporulation. P. ananatis B7, BRT98, and 26SR6 showed an intermediate phenotype with large plaque formation occurring even when only 100 D. discoideum cells were applied. P. ananatis Cit30-11, LMG5342, and 17671 were completely susceptible to D. discoideum grazing, with large plaques forming and sporulation occurring in all treatments. Interestingly, the sister taxon isolate to P. ananatis BRT175, P. ananatis 17671, was one of the least grazing-resistant isolates, with plaque and spore formation being evident throughout the lawn. Grazing resistance and susceptibility did not appear correlated with phylogenetic relatedness within

TABLE 1 Bacterial and eukaryotic strains used in this study

Species and strain


Source or reference

Pantoea ananatis 15320 17671 26SR6 B7





Rifampin Rifampin Rifampin Rifampin

Ricea Ricea

Maize leaf6 Maize6 Strawberry^ Strawberry6 Navel orange leaf6 Maize6 Eucalyptus^ Human woundd

Escherichia coli HB101 (RK600) VPE42(pBSL118) B/r

Dictyostelium discoideum AX2-214

Chloramphenicol Kanamycin, ampicillin

Streptomycin, ampicillin

^International Collection of Microorganisms from Plants.

6Steven Lindow, University of California, Berkeley. cGwyn Beattie, Iowa State University. ^Teresa Coutinho, University of Pretoria.

DBS0305924 (75) DBS0235534 (75)


the P. ananatis species group (13), as isolates at both extremes of grazing resistance are closely related.

Transposon mutagenesis identifies multiple genetic factors linked to grazing resistance. To identify the genetic factors involved in grazing resistance, the grazing-resistant P. ananatis BRT175 was selected for mutagenesis and a high-throughput genetic screen was initiated for D. discoideum grazing susceptibility. A total of 3,789 mutants of P. ananatis BRT175 were screened, and 36 wells were identified as containing a grazing-susceptible mutant, as indicated by large plaque formation and/or sporulation. These 36 mutants were shown to represent 26 candidate genes that influence bacterial grazing resistance. Representative mutants from each of the 26 candidate genes were tested for growth deficiencies, with many of the mutants showing little or no defect in growth rate or growth density relative to the wild type (see Fig. S1 in the supplemental material). These 26 genes included quorum-sensing-related autoinducer synthase homologs of phzI and eanI, as well as purine and pyrimidine biosynthesis genes guaB and pyrC, pyrD, and carB (Table 2). Also identified was the dsbB gene, which is involved in a two-component system that forms disulfide bonds in periplasmic proteins (31-33), as well as the thioredoxin system component trxB, which plays an important role in replication during intracellular growth (34).

The screen also identified rhlA and rhlB as being important for grazing resistance. The rhlA and rhlB genes, which were recovered once and four times, respectively (Table 2), are adjacent genes in the P. ananatis BRT175 genome. Homologs of these rhlA and rhlB genes encode enzymes responsible for the biosynthesis of rhamnolipids in Pseudomonas aeruginosa and a few Burkholderia species (35). The transposon insertion in the rhlA::Tn5 mutant (mutant 28C8) occurred near nucleotide 385 of the 837-bp open reading frame, which would induce a polar mutation if the genes are coregulated and in a putative operon (36, 37). The transposon insertion in the rhlB::Tn5 mutant (mutant 32C5) occurred near nucleotide 531 of the 1,173-bp open reading frame. Both rhl mutants had severe impairment in grazing resistance, with amoebal sporulation being evident after 7 days of grazing compared to no sporulation and minimal plaque formation on wild-type P. ananatis BRT175. The rhlA::Tn5 mutant was even more susceptible, showing complete grazing susceptibility with as few as 500 amoebae being sufficient for sporulation, whereas 2,000 or more amoebae were necessary for sporulation on the rhlB::Tn5 mutant (Fig. 2A).

rhlA is involved in biosynthesis of a glycolipid biosurfactant. To establish the involvement of a biosurfactant, we measured and compared surface tension and

c a CD 2


FIG 1 Qualitative assay of resistance of P. ananatis isolates to D. discoideum grazing. Ten thousand, 1,000, and 100 Dictyostelium discoideum AX2-214 cells were applied to dried bacterial lawns and monitored for 7 days for plaque formation and sporulation. E. coli B/r is used as the food source for D. discoideum and was included as a reference. The buffer SorC was used for the no-amoeba control.

emulsification activities of culture extracts from P. ananatis BRT175 and the rhlA::Tn5 mutant. Wild-type culture extracts were found to reduce the surface tension of water from 72 to 40 mN/m, whereas the rhlA::Tn5 culture extracts could reduce the water surface tension only to 62 mN/m. Accordingly, the mutant extracts had almost no emulsification activity compared to the wild type (Fig. 3). These results suggested the production of an extracellular biosurfactant and the involvement of the rhlA product in its synthesis.

To determine if the biosurfactant was a rhamnolipid, we analyzed the extracts from the wild type and the rhlA::Tn5 cultures using liquid chromatography-mass spectrometry (LC-MS) protocols developed for rhamnolipids. Wild-type extracts had three peaks with m/z values of 519, 547, and 575, which were absent from the rhlA::Tn5 culture extracts (Fig. 4), but none of these corresponded to any of the approximately 60 different known rhamnolipid congeners (38). To investigate this unexpected result, we used tandem mass spectrometry (MS/MS) fragmentation to further analyze the m/z 519 pseudomolecular ion, the most abundant molecule requiring rhlA for its biosynthesis. This biosurfactant was determined to be a monohexose-C10-C10, although the exact nature of the sugar moiety is still undetermined (Fig. 5). The two other identified masses (m/z 547 and m/z 575) appear to correspond to congeners containing hydroxy-dodecanoic (C12) and hydroxytetradecanoic (C14) acid moieties as side chain fatty acids. Further investigation will be required to fully identify the exact nature of these new biosurfactants.


СЛ o


a CD 2


TABLE 2 Locations of Tn5 transposon gene insertions in grazing-susceptible mutantsd

Grazing phenotype and locus0 Gene

Predicted function


Mutant designation(s)

Grazing susceptible L585_12500 L585_05285 L585_21390

L585_04860 L585_22810

L585_16630 L585_21750

L585_20040 L585_10945

L585_00065 L585_00075

L585_10950 Enhanced grazing susceptible L585_10305


L585_16795 L585_21810 L585_03130 L585_21385 L585_03125 L585_04515


L585_19770 L585_21595 L585_04660

L585_15360 L585_21170

ompR cpxA

phzR/luxR sdiA ptsN


ds6B serC

srmB yagG

motA flhD

guaB pyrD pnp

prfC pyrC

Transcriptional regulator Y

Histidine kinase Y

[Intergenic space-upstream] Y

transcriptional regulator PTS sugar transporter subunit IIA Y

Transcriptional regulator (polar Y

mutation of nagC) Disulfide bond formation protein Y

3-Phosphoserine/ Y

phosphohydroxythreonine aminotransferase RNA helicase N

[Intergenic space-upstream] Y

uncharacterized member of the GPH family of galactose-pentose-hexuronide transporters (symporter) Flagellar motor protein N

[Intergenic space-upstream] N

transcriptional regulator and flagellar apparatus operon Acylhomoserine lactone synthase Y

Hypothetical protein (rrf2 domain, Y badM-like transcriptional regulator)

[Intergenic space-downstream] Y aerobic respiration control sensor protein

Carboxy-terminal protease Y

Thioredoxin reductase Y

Rhamnosyltransferase I, subunit B Y

Autoinducer synthase Y

Rhamnosyltransferase I, subunit A N

Aspartate carbamoyltransferase Y

catalytic subunit

Carbamoyl phosphate synthase Y

large subunit

IMP dehydrogenase Y

Dihydroorotate dehydrogenase Y

Polynucleotide phosphorylase/ N


Peptide chain release factor 3 N

Dihydroorotase Y

28H12 35D8, 18A11 10E5

19E7 26A5

26H9 28G12

36D8 31C1

42A7, 42H16

16A5, 16A2,6 16A1,6 16H126 24A2, 24A5c

14G9 39D5

32C5, 24H12, 25E4, 40C2

25E1, 26F46

4H11 28H8 30D8

8F6 35F10

^Mutants exhibiting plaque formation were scored as grazing susceptible, whereas mutants in which 4 out of 8 test wells exhibited spore formation were classified as enhanced grazing susceptible. The NCBI accession number for the draft annotated whole-genome shotgun sequence is ASJH01000000. ^Mutant not tested for swarming capability. cMutant did not swarm.

^Abbreviations: PTS, phosphotransferase; Y, yes; N, no.


сn о

CD 2 t


rhlA but not rhlB is essential for full swarming motility. Because rhamnolipids can aid in swarming motility in some species (39-41), we compared the swarming proficiency of the rhl mutants relative to that of the wild type. Wild-type P. ananatis BRT175 exhibits a characteristic dendritic pattern on 0.5% modified SM agar (Fig. 2B and C), whereas the rhlA::Tn5 mutant is deficient in swarming on 0.5% modified SM agar and 0.5% modified M9 agar (Fig. 2B and C). The rhlB::Tn5 mutant was still capable of swarming on both medium types (Fig. 2B and C). The three other rhlB::Tn5 mutants (25E4, 24H12, and 40C2), each of which appeared to have a unique transposon insertion site, also retained swarming activity on 0.5% modified SM agar. To determine whether swarming motility was an indicator for grazing resistance, all isolates in the P. ananatis group were tested for swarming proficiency. Grazing-susceptible P. ananatis

rhlA rhlB

rhlAv.Tn5 (28C8) MA rhlB

rhlBr.Tn5 (32C5) rhlA rhlB

A 8000 4000 2000 8000 4000 2000 8000 4000 2000

8000 4000 2000

rCc V

1000 500 250

FIG 2 Grazing and swarming phenotypes of Pantoea ananatis BRT175 biosurfactant mutants. The predicted operon is shown at the top for each strain, with a red "X" indicating the disrupted gene. (A) Grazing of P. ananatis BRT175 at different cell densities (250 to 8,000 cells) of D. discoideum AX2-214 after a 7-day incubation. WT, wild type. (B) Swarming after a 24-h incubation on 0.5% modified SM agar. (C) Swarming after 48 h on 0.5% modified M9 agar.

Cit30-11 and LMG5342 and E. coli B/r showed no motility (Fig. 6), whereas P. ananatis 17671, a grazing-susceptible isolate, had a different motility phenotype, as it appeared to move mostly linearly from the point of inoculation. P. ananatis 17671 did not form dendrites, nor did it form what is commonly referred to as a "featureless mat" (42), which is one of the motility patterns formed by some swarming bacteria. P. ananatis LMG20103, M232A, B7, 15320, BRT98, and 26SR6, which represent both grazing-


C/J ~D

c a CD 2

n CD C/J

WT rhlA- t Control -

m V > )

FIG 3 Emulsification activity of culture extracts of P. ananatis BRT175 strains against n-hexadecane. The wild-type (WT) extract exhibits emulsifying activity, whereas the extract from the rhlA::Tn5 (mutant 28C8) culture lacks any emulsifying activity, with the height of the hydrophobic phase being identical to the negative control (reagent-grade water).

Scan ES-4.57e5

......I l'l I. I r I


I ii'lii |i I I'll if I p

» ГЦ I ut '"l'i»'1' 'T ' h''"' ■ » r^^' 11 ' ■ '^'l' ■'■'■ i ......... ' I nil |l'n .fi I и; itii

L'l 111 Л P 'I

\ mTj n iti'h t it 11 i n^ I i'i 1

Scan ES-

b 3.09e5

200 220 240 260 280 300 320 340 360 380 400 420 440 460 480 500 520 540 560 580 600 FIG 4 Triple-quadrupole ESI-MS spectra of P. ananatis BRT175 culture extracts obtained in negative ionization mode. Pseudomolecular ions [M-H]~ are observed at m/z 519, 547, and 575 for the wild-type strain (a), which are absent in culture extracts of the rhlA::Tn5 strain (mutant 28C8) (b). The y axis shows relative abundance considering the highest ion as 100%; the x axis shows m/z for each ion. The pseudomolecular ion at m/z 271 corresponds to 16-hydroxyhexadecanoic acid, which was added as an internal standard.

1 o ш

resistant and intermediate strains, formed primarily a "featureless mat" phenotype with some dendrite-like protrusions visible in B7, LMG20103, M232A, and BRT98 trials (Fig. 6).

The biosurfactant produced by P. ananatis BRT175 is cytotoxic to D. discoideum. To evaluate whether the new biosurfactant produced by P. ananatis BRT175 has a cytotoxic or inhibitory effect at concentrations produced within culture media, D. discoideum cells were exposed to cell-free culture medium conditioned with either wild-type P. ananatis BRT175, the rh!A::Tn5 mutant, or the rh!B::Tn5 mutant (Kruskal-Wallis test, significant P = 0.02). In three independent plaque assay experiments, no plaques formed on plates seeded with amoebae that had been exposed to wild-type-conditioned culture medium (P = 0.0305) (Fig. 7A). Amoebae exposed to rh!A::Tn5



a CD 2


FIG 5 Daughter ions produced upon fragmentation of the m/z 519 pseudomolecular ion, using MS/MS. The proposed structure and fragmentation pattern are illustrated.

FIG 6 Swarming motility patterns of wild-type P. ananatis strains and E. coli B/r. All images represent the motility patterns observed after incubation for 24 h at 21°C following a single point inoculation on 0.5% modified SM agar. B7-A and B7-B represent two different swarming phenotypes of P. ananatis B7.

strain-conditioned medium formed plaques similar to the number seen in the control (P = 0.2728). Interestingly, the rh!B::Tn5 strain-conditioned medium also did not allow for plaque formation (P = 0.0305). Amoeba cell viability assays using trypan blue staining were consistent with these results (Kruskal-Wallis test, P = 0.04), with exposure to the wild-type-conditioned culture medium leaving mostly cellular debris (P = 0.0064) (Fig. 7B). Cells exposed to the rh!B::Tn5 strain-conditioned medium were still


C/J ~D

c a CD 2

c CD C/J

FIG 7 Mean plaque and cell viability counts after exposure to conditioned culture medium. The figure was generated in R using ggplot2 (72, 73). (A) Plaque-forming units were enumerated after 25 min of room-temperature exposure to medium conditioned with either wild-type P. ananatis BRT175, the rhlA::Tn5 strain (mutant 28C8), or the rhlB::Tn5 strain (mutant 32C5). Each data point represents the mean from three independent experiments with the standard error reported. The asterisk denotes statistical significance using Dunn's test (P = 0.0305). (B) D. discoideum AX2-214 cells were enumerated after exposure to medium conditioned with either wild-type P. ananatis BRT175, the rhlA::Tn5 strain (mutant 28C8), or the rhlB::Tn5 strain (mutant 32C5) for 20 min at room temperature. Each data point represents the mean from three independent experiments with the standard error reported. The asterisk denotes statistical significance using Dunn's test (P = 0.0064).

FIG 8 Phylogenetic trees of RhlA and RhlB homologs. Radial (unrooted) neighbor-joining phylogenies of representative RhlA (A) and RhlB (B) homologs, constructed using the Jones-Taylor-Thornton amino acid model, with complete gap deletion. Only bootstrap values greater than 70% are shown. In addition to the P. ananatis strains used in this study, other representative taxa included Burkholderia cenocepacia H111 (CDN64069), Burkholderia glumae BGR1 (ACR31008), Burkholderia pseudomallei 1106a (ABN94800), Dickeya dadantii 3937 (YP_003882762), Lonsdalea quercina (WP_026742016), Pantoea stewartii subsp. stewartii DC283 (EHU02365), Pseudomonas aeruginosa PAO1 (NP_252169), and Serratia marcescens FGI94 (AGB82844).

largely intact, but many cells showed trypan blue uptake, indicating loss of membrane integrity (P = 0.1065); there was also no significant difference between the rhlA::Tn5 strain-conditioned medium and the control (P = 0.4549).

rhlA and rhlB are distributed among isolates of P. ananatis. A survey of the distribution of the P. ananatis BRT175 rhlA and rhlB genes using BLAST identified the closest homologs in several other sequenced isolates of P. ananatis, including P. ananatis LMG20103 (43), LMG5342 (44), AJ13355, and PA13, as well as in unpublished draft genomes of P. ananatis 15320, BRT98, 26SR6, Cit30-11, and 17671. Homologs were also identified in Pantoea stewartii subsp. stewartii DC283, which is a sister species to P. ananatis (13). Independent genealogies of the two genes constructed using representative sequences from a variety of species show partial congruence of the major clades, with monophyly of the P. ananatis-P. stewartii homologs; however, the most recent common ancestor of the P. ananatis rhlA gene is shared with Lonsdalea quercina, whereas the P. ananatis rhlB gene is more closely related to the Serratia marcescens homolog (Fig. 8). In the Serratia and Dickeya lineages, the rhlA and rhlB genes are not adjacent to each other as in the P. ananatis isolates.


This work explored the genetic factors responsible for grazing resistance and/or virulence of P. ananatis in a D. discoideum pathosystem. The qualitative grazing assay identified four out of 10 isolates as having a resistant phenotype (limited plaque formation), three as having intermediate phenotypes (plaque formation but no sporulation), and three as having a susceptible phenotype (plaque and spore formation) (Fig. 1). Sister isolates P. ananatis BRT175 and P. ananatis 17671 showed phenotypes on

1 o 0) Q. CD

C/J ~D

—5 0

H J C H CD 2

c CD C/J

the two extremes of the grazing resistance spectrum, supporting the presence of specific genetic factors that contribute to this phenotype. It has been shown that there are differences in the flexible genomic complement of P. ananatis isolates, such that the species appears to have an open genome (17), which facilitates the introduction of substantial genetic variability and the acquisition of isolate-specific virulence traits. In the case of grazing resistance, the method by which such factors confer the grazing-resistant phenotype may be through one of several mechanisms. The plaque formation with no sporulation, for example, may suggest that the bacteria interfere with the D. discoideum life cycle, as shown with Salmonella enterica subsp. Typhimurium (45). S. enterica inhibits the D. discoideum starvation response through the type III secretion system (45), thereby preventing sporulation. We were unable to identify any type III secretion system in P. ananatis BRT175 that might function analogously (46). However, isolates within the P. ananatis group may use other secretion systems, which are known to be responsible for producing cytotoxic factors by some bacteria (18, 47). It is also O

possible that bacteria produce antifeeding factors, such that the amoebae starve to i

death. Serratia marcescens produces serrawettin W2, a surfactant that causes Caeno- a

rhabditis elegans to avoid feeding on the bacteria (48). Another mechanism to explain the grazing phenotype is the direct killing of the predatory amoebae. A wide variety of toxins and virulence factors are activated in a density-dependent manner through O

quorum sensing regulation in a number of pathogenic bacteria (49-51), which may D

directly target the amoebae. Several of the 26 candidate loci implicated in grazing t

resistance were genes involved in biosynthetic pathways that had been shown previ- //

ously to be involved in virulence in humans and animal model systems (Table 2). 3

Of the candidate genes identified, the rhamnolipid biosynthesis genes rhlA and rhlB p

were of particular interest due to their involvement in the production of rhamnolipids r

and their importance in the virulence of the opportunistic human pathogens P. aerugi- .

nosa and Burkholderia spp. (52-54). Typically, rhlA and rhlB are in an operon (55, 56), s

and this may be the case for P. ananatis BRT175 based on the collinearity and close .

proximity of the two coding regions in the genome sequence (46). In other systems, g

these genes direct the production of rhamnolipids, which act as wetting agents that O

enable swarming motility but which also have cytotoxic properties (40, 53). RhlA is D

necessary for the synthesis of 3-(3-hydroxyalkanoyloxy)alkanoic acids (HAA) (40). RhlB is u

the rhamnosyltransferase that transfers a dTDP-L-rhamnose to HAA to form a monor- (D

hamnolipid, while RhlC can transfer an additional rhamnose sugar to create a dirham- 2

Q. CD Q.

nolipid (40, 55, 57). Interestingly, these glycolipidic biosurfactants have been reported 2

only anecdotally in cultures of Enterobacteriaceae (38). In P. ananatis BRT175, the

products of rhlA and rhlB are responsible for the biosynthesis of a novel, hexose-based

surfactant. The lipid moieties primarily consist of hydroxydecanoic (C10) acid, much like D

the rhamnolipids produced by P. aeruginosa (58), but other congeners that likely u

consisted of hydroxydodecanoic (C12) or hydroxytetradecanoic (C14) acid were de- s

tected. This glycolipid also exhibits emulsification and surface tension reduction properties, which are known characteristics of rhamnolipid biosurfactants (38).

The culture medium conditioned by the growth of P. ananatis BRT175 was cytotoxic based on our observations in a plaque assay and trypan blue staining of exposed cells. The cytotoxicity of the wild-type-conditioned medium is consistent with previous work in P. aeruginosa that showed rapid lysis of D. discoideum cells (30) and polymorphonuclear leukocytes (53) after exposure to rhamnolipid extracts. While we did not observe plaque formation after exposure to rhlB::Tn5 strain supernatant, trypan blue staining revealed compromised cells, suggesting the retention of some level of cytotoxicity likely due to the production of the fatty acid component of the biosurfactant by RhlA (Fig. 2A). In P. aeruginosa, the HAA precursor still possesses some surfactant properties (39,40), which also explains the capacity of the rhlB::Tn5 strain to still swarm, albeit differentially from wild type (Fig. 2B and C). Rhamnolipid-free and HAA-dependent P. aeruginosa swarming can lead to a reduced swarming zone (40) and altered motility patterns (39). Another study examining the influence of rhamnolipids

and HAA on swarming motility patterns found that HAA can inhibit dendritic tendril formation and can cause repulsion of cells away from concentrations of HAA (59).

Our analysis of the distribution of the rhlA and rhlB homologs revealed that these two genes are common to all P. ananatis strains analyzed. The qualitative differences in the grazing resistance phenotypes between P. ananatis BRT175, P. ananatis BRT98, P. ananatis LMG20103, P. ananatis LMG5342, P. ananatis Cit30-11, P. ananatis 26SR6, P. ananatis 17671, and P. ananatis 15320 are not attributable solely to the presence of rhlA-rhlB genes, as all 8 genomes carry the genes (Fig. 8). This suggests that differences in regulation, other unidentified genetic factors, or combinations thereof are involved in the P. ananatis-D. discoideum interaction. Nonetheless, the persistence of these genes in the P. ananatis lineage suggests that they play an important role in the biology of this species. Furthermore, the presence of these genes in the sister species P. stewartii could suggest acquisition by the P. ananatis-P. stewartii common ancestor, although

additional P. stewartii isolates will need to be surveyed to test this hypothesis. The 0

origin of acquisition is not entirely clear, particularly given that the closest homolog of n

the P. ananatis-P. stewartii rhlA gene is that from the enteric bacterium L. quercina, o

whereas the P. ananatis-P. stewartii rhlB gene is closest to the homolog from a different d

enteric bacterium, S. marcescens (Fig. 8). Because the homologs are not adjacent in the cc

Serratia genome, this could indicate that P. ananatis rhlA and rhlB have come from O

different sources. Alternatively, the Pantoea homologs may have been transferred to 3

some of the other enteric organisms individually, although there are insufficient t

representative sequences from this group to determine whether this is the case. :

The evolutionary arms race between microorganisms competing for the same m

environmental niche is thought to be an evolutionary driver for opportunistic patho- p

gens (60-62). This predatory relationship of environmental amoebae with bacteria, for e

example, may select for traits in prey that confer resistance to phagocytosis but which e

have the potential for exaptation as virulence factors that function against the cells of a

the innate immune system (30, 53, 61, 63). Such determinants may enable those same m

isolates to exploit additional hosts, effectively expanding their host range to include r

animals and humans. Unraveling the key genetic factors that enable strains of Pantoea /

spp. to colonize different hosts will provide important insight into the pathogenic n

capabilities of this highly versatile group. u


Cell growth and culturing. Overnight cultures of Pantoea and Escherichia coli were grown at 30°C and 2

37°C, respectively, in Miller LB broth (BD, Franklin Lakes, NJ) with shaking at 220 rpm under appropriate

antibiotic selection and conditions (Table 1) (50 ^g/ml kanamycin, 150 ^g/ml ampicillin, 50 ^g/ml °

rifampin, 38 ^g/ml chloramphenicol). Dictyostelium discoideum AX2-214 cultures were incubated at 21°C and maintained in petri dishes containing 10 ml HLF1 (Formedium, Hunstanton, United Kingdom) HL5 medium with vitamins and microelements, supplemented with 13.5 g/liter glucose, 300 ^g/ml strepto- <<

mycin, and 150 ^g/ml ampicillin. Cells were passaged every 4 to 6 days following a 100-fold dilution, and (Q

fresh stocks were prepared axenically from spores after 3 to 4 weeks of passaging (64). Spores were e

harvested from SM/5 plates (2 g/liter glucose, 2 g/liter Bacto peptone [BD], 0.2 g/liter yeast extract [BD], t

0.2 g/liter MgSO4-7H2O, 1.9 g/liter KH2PO4, 1.0 g/liter K2HPO4, 1.5% agar [BD], pH 6.5) with E. coli B/r as a food source (64). Cultures for downstream assays were prepared via a 100- to 200-fold dilution of confluent cells in Erlenmeyer flasks containing HL5 at no more than 20% of the maximum volume. The cells were incubated at room temperature and shaken at 180 rpm. Cells were harvested during log-phase growth (typically 3 X 106 to 6 X 106 cells/ml) by centrifuging 15 to 50 ml of cell culture three times at 500 X g for 5 min and resuspending the pellet each time in Sorensen's buffer with calcium (SorC) (2 g/liter KH2HPO4 0.29 g/liter Na2HPO4, 50 ^M CaCl2, pH 6.0). The final pellet was resuspended in 1 ml of SorC. Cells were enumerated in a hemocytometer and diluted to appropriate concentrations for downstream applications.

Qualitative screen for grazing-resistant isolates. A collection of Pantoea isolates (13) was evaluated for grazing resistance using a modified qualitative D. discoideum assay (26). Cells from an overnight Pantoea culture were centrifuged at 10,000 X g for 5 min and resuspended in an equal volume of SorC twice. To ensure consistency of inoculations across qualitative grazing plates, bacterial cell densities were standardized to a final optical density at 600 nm (OD600) of 1.0 in SorC by taking absorbance readings from 200-u.l samples using a BioTek Epoch microplate spectrophotometer (BioTek, Winooski, VT) in 96-well plates (Greiner Bio-One, model 655180; Monroe, NC). Fifty microliters of each bacterial suspension was spotted and allowed to dry onto 24-well plates containing 1.5 ml modified SM agar per well (65) (10 g/liter glucose, 10 g/liter Bacto peptone [BD], 1 g/liter yeast extract [BD], 1 g/liter MgSO4-7H2O, 1.9 g/liter KH2PO4, 0.6 g/liter K2HPO4, 1.5% agar [BD], pH 6.5). Suspensions of D. discoideum were pipetted

in 5-jU.l aliquots onto the center of each well at 10,000,1,000, and 100 total cells. Escherichia coli B/r, which is used as the food source for D. discoideum, served as a control. Isolates were identified as grazing resistant if plaque formation was reduced or absent and sporulation did not occur after exposure to 10,000 D. discoideum cells after 7 days of incubation at 21°C (in darkness). The experiment consisted of two replicates, and experiments were repeated twice with similar results.

Genetic screening and mutant characterization. Mutagenesis was carried out using a triparental mating approach, whereby the RK600 helper plasmid was used to introduce the pBSL118 plasmid, carrying a mini-Tn5 transposon (kanamycin resistance), into P. ananatis BRT175 (rifampin resistance) (Table 1). Aliquots of each overnight culture (1 ml) were pelleted and resuspended in 100 ¡l LB and mixed in a 1:1:1 ratio. This triparental mixture (100 ¡l) was spotted on LB agar plates and incubated overnight at 30°C. A portion of the bacterial lawn was then scraped from the plate with the edge of a sterile spreader and spread on an LB plate containing rifampin and kanamycin. Following incubation for 24 to 48 h at 30°C, individual transposon mutants were picked and grown overnight at 30°C with shaking at 150 rpm in 96-well plates containing 100 ¡l modified SM broth (recipe as described above, without agar, pH 6.0 to 6.4) per well. The following day, 5 ¡l from each well was plated on a corresponding 96-well modified SM agar plate, allowed to dry, and overlaid with 2 ¡l of D. discoideum at 500 cells/juJ. Plates were monitored for up to 7 days for wells containing susceptible mutants, which were characterized by enhanced plaque formation and/or sporulation. Susceptible mutants were retested in replicates of 8 for confirmation of the phenotype (Table 2).

DNA was extracted from each mutant using the E.Z.N.A bacterial DNA kit (Omega Bio-Tek, Norcross, GA)

The location of the transposon insertion in each mutant was determined by inverse PCR (66). Briefly, a

per the manufacturer's directions. About 1 to 2 ¡g of genomic DNA was digested for 2 h at 37°C using Q.

HincII or PstI (New England Biolabs, Whitby, Ontario, Canada) in a 20-A reaction volume using 20 units r

of enzyme and according to the manufacturer's instructions. Ten microliters of heat-inactivated digest ® was added to 3 ¡A T4 DNA ligase (New England Biolabs), 167 ¡A double-distilled water (ddH2O), and 20 ¡A

10X T4 buffer to be incubated for 16 h at 16°C. Ligations were purified using the E.Z.N.A Cycle Pure kit t

(Omega Bio-Tek) and eluted into a 30-u.l volume. Typically, 5 ¡A of purified ligation had sufficient :

template to be amplified in a 25- to 50-A PCR mixture using EconoTaq DNA polymerase (Lucigen Corp., ^

Middleton, WI) per the manufacturer's instructions, using the primers NPT + 772 (5'-TTCGCAGCGCATCG s

CCTTCTATC-3') and NPT-41 (5'-AGCCGAATAGCCTCTCCACCCAAG-3' ). Cycling conditions were one de- h

naturation cycle of 94°C for 120 s, followed by 40 cycles of 94°C for 30 s, 63°C for 30 s, and 72°C for 240 s, e

and one polymerization cycle of 72°C for 300 s. Amplification was verified by gel electrophoresis, and e

single amplicons were excised and gel purified from any reactions with multiple amplicons using the a E.Z.N.A gel extraction kit (Omega Bio-Tek) per the manufacturer's instructions. Amplicons were sequenced by Génome Québec (Montréal, Québec, Canada). Insertion sites were confirmed by BLAST analysis against the annotated P. ananatis BRT175 genome (46).

rhlA-rhlB mutant phenotypic characterization assays. To determine the relative differences in

grazing susceptibility caused by the interruption of rhlA and rhlB, cultures of P. ananatis BRT175, the O

rhlA::Tn5 strain (mutant 28C8), and the rhlB::Tn5 strain (mutant 32C5) were grown overnight at 30°C in j

modified SM broth. An 0.5-ml sample of each strain culture was added to 5 ml of fresh modified SM broth C

and incubated for another 40 min at 30°C to dilute the cultures and increase the proportion of live cells. e

Cell densities were standardized to an OD600 of ~0.125 from 200-,u,l samples using the plate spectro- 2

photometer in 96-well plates (as described above). D. discoideum cells were diluted half-fold eight times ,

starting at 1,600 cells/¡l. A 12.5-u.l volume of bacteria was spotted on modified SM agar and allowed to 2

dry. Five microliters of each of the dilution series of D. discoideum cells was then placed on separate spots 1

in order of decreasing concentration. Experiments were performed twice with two replicates each. (D

To create conditioned culture medium for the cytotoxicity assays, P. ananatis BRT175, P. ananatis O"

BRT175 rhlA::Tn5 (mutant 28C8), and P. ananatis BRT175 rhlS::Tn5 (mutant 32C5) were each grown at 21°C g

for 6 days with shaking at 220 rpm in modified M9 medium (2 mM MgSO4, 20 g/liter glucose, 0.1 mM u

CaCl2, 1/5 dilution of 5X M9 salts [64 g/liter Na2HPO4, 15 g/liter KH2PO4, 2.5 g/liter NaCl, 13.78 g/liter S

NaNO3]). Sodium nitrate was substituted for ammonium chloride as it has been shown to be a preferred nitrogen source in Pseudomonas aeruginosa for surfactant production (67). Filtration was performed to retain products exported by the bacteria while excluding bacterial cells. Cultures were centrifuged, the bacterial pellet was discarded, and supernatants were filter sterilized using 0.2- to 0.22-u.m polyether sulfone (PES) bottle top filters. The supernatants and control media were adjusted to pH 6.52 ± 0.02 and resterilized using 0.2- to 0.22-^m PES syringe filters to standardize pH values for downstream assays. Supernatants were kept at 4°C between experiments.

These supernatants were then used in PFU assays to assess D. discoideum cell viability after exposure to conditioned culture medium. Overnight cultures of E. coli B/r were centrifuged twice for 2 min at 12,000 X g and resuspended in 1 ml SorC each time. The final E. coli suspension was then diluted to an OD600 of ~0.1 (200 ¡l, 96-well plate). The D. discoideum cells (harvested as described above) were diluted to 15 cells/¡l in SorC. Aliquots of 90 ¡l of modified M9 culture medium conditioned by P. ananatis BRT175, P. ananatis BRT175 rhlA::Tn5 (mutant 28C8), or P. ananatis BRT175 rhlS::Tn5 (mutant 32C5) or unconditioned culture medium as the control were prepared. Ten microliters of amoebae was then added to the 90 ¡l of medium and incubated for 25 min at 21°C. Three hundred microliters of the prepared E. coli suspension was added after incubation. The entire volume was pipetted on a 60-mm petri dish containing SM/5 medium and dried while on a rotary shaker to help evenly distribute the liquid. The plates were incubated at 21°C, and plaque counts were taken after 3 to 4 days. Statistical comparisons were performed using the Kruskal-Wallis test and Dunn's test (68) for pairwise comparisons

of the mean plaque counts from three independent experiments between the control and each treatment.

Cell viability was assessed using a trypan blue viability assay. This was performed by resuspending pelleted D. discoideum cells in 125 ¡A of filtered conditioned culture medium from either P. ananatis BRT175, P. ananatis BRT175 rhlA::Tn5, or P. ananatis BRT175 rhlB::TnS, with unconditioned modified M9 medium as a control. A stock of D. discoideum cells was prepared at ~4,000 cells/A for creating 250-A aliquots for each replicate. The cells were centrifuged for 5 min at 500 X g, and the supernatant was discarded. D. discoideum cells were resuspended and exposed to the conditioned culture medium and control for a minimum of 20 min at room temperature. One hundred twenty-five microliters of 0.4% trypan blue was added, and total and unstained cells were enumerated by counting 25 of the 0.040-mm2 squares on a hemocytometer. Each treatment was performed in triplicate. Most cells in the wild-type-conditioned culture medium treatment could not be enumerated as they were reduced to cellular debris. Statistical comparisons were performed using the Kruskal-Wallis test and Dunn's test (68) for pairwise comparisons of the mean viability counts from three independent experiments between the control and each treatment.

Swarming trials were performed by inoculating a single colony in the center of a modified SM agar plate containing 0.5% (wt/vol) agar and incubating it at 21°C for 24 h. P. ananatis BRT175 mutants were O

monitored for up to 48 h for swarming. Swarming assays were also performed on modified M9 agar w

plates containing 0.5% (wt/vol) agar by centrifuging cultures grown at 30°C and resuspending the l

bacterial pellet in the medium to an OD600 of ~0.4 (200 ¡l, 96-well plate). Ten microliters of concentrated O

culture was applied to the center of the agar plates and incubated at 21°C for 48 h. All images in this d

study were captured using an Epson Perfection V330 photo scanner at 600 to 1,200 dots per inch (DPI). d

Biosurfactant production and extraction. To characterize the structure of the biosurfactant, solvent f

extractions were performed on culture medium conditioned with either P. ananatis BRT175 or P. ananatis O

BRT175 rhlAvTnS (mutant 28C8). Cultures were grown in 200 ml MSM supplemented with 20 g/liter C

glucose and 2 g/liter NaNO3 in 1-liter Erlenmeyer flasks and incubated at 30°C with shaking at 250 rpm. t

MSM had the following composition: 2.5 g/liter KH2PO4, 1.5 g/liter K2HPO4 0.1 g/liter CaCl2-2H2O, p

0.4 g/liter MgSO4-7H2O, 2 ml/liter trace element solution (TES), pH adjusted to 7. The composition of TES /

was 2 g/liter FeSO4-7H2O, 1.5 g/liter MnSO4-H2O, 0.6 g/liter (NH4)6Mo7O24-4H2O, 1.4 g/liter ZnSO4-7H2O, 3

1.2 g/liter CoCl2-6H2O, 1.2 g/liter CuSO4-5H2O, and 2 g/liter sodium citrate-2H2O.

After 6 days of incubation, the cells were pelleted by centrifugation at 8,000 X g for 15 min, and the resulting supernatant was acidified with 1 N HCl to a pH of 2 to 3. The supernatant was then extracted twice with equal volumes of ethyl acetate. The organic fractions were then pooled and rotary evaporated, which yielded a crude extract containing the biosurfactant product. The final crude extract from 200 ml of culture was dissolved in 25 ml of MilliQ water to give an 8-fold-concentrated extract solution, which 3

was subsequently used for further analysis. O

Liquid chromatography-mass spectrometry analyses. The culture extracts of P. ananatis BRT175 g

and P. ananatis BRT175 rhlA::TnS (mutant 28C8) were dissolved in methanol, and 16-hydroxyhexadecanoic °

acid was added as an internal standard. Samples were analyzed by high-performance liquid chroma- n

tography (HPLC; Waters 2795, Mississauga, Ontario, Canada) equipped with a 6.4- by 150-mm Agilent C_

Zorbax Eclipse XDB-C8 reverse-phase column (particle size, 5 mm) using a water-acetonitrile gradient n

with a constant 2 mmol • litei—1 concentration of ammonium acetate (56). The detector was a mass CC

spectrometer (Quattro Premier XE; Waters). Analyses were performed in negative electrospray ionization 2

(ESI—), supplemented by the multiple-reaction monitoring (MRM) mode (69).

Surface tension and emulsification assays. The surface tension of the extract solutions of P. anana- 0

tis BRT175 and P. ananatis BRT175 rhlA::TnS (mutant 28C8) strains was measured by the du Nouy ring —i

method using a Fisher tensiometer model 20 (Fisher Scientific, Pittsburgh, PA). The instrument was C

calibrated against water, and measurements were performed in triplicate at room temperature. The y

emulsifying activity of culture extracts was tested against n-hexadecane. Three-milliliter aliquots of g

extract solutions of P. ananatis BRT175 and P. ananatis BRT175 rhlA::TnS (mutant 28C8) were mixed with e

2 ml of n-hexadecane and vortexed at high speed for 2 min. The emulsion was observed after letting the tt

tubes stand at room temperature for 60 min. The lipophilic dye Sudan black was added to the n-hexadecane to increase contrast.

Phylogenetic analyses. Homologs of the P. ananatis BRT175 rhlA and rhlB genes were identified using BLAST against both complete and draft genome sequences available at NCBI. Alignments were made using ClustalX2 with default parameters using iteration after each alignment step. Neighbor-joining phylogenies were constructed using MEGA6 (70) with the Jones-Taylor-Thornton amino acid model, complete gap deletion, and 500 bootstrap replicates.

Growth comparisons of P. ananatis BRT175 mutants. P. ananatis BRT175 and TnS mutants were inoculated into 10 ml of modified SM broth in a 15-ml conical tube, which was then tightly sealed and incubated overnight at 30°C without shaking (71). Overnight cultures were standardized to an OD600 of ~0.2 (300 A, 96-well plate). Of the standardized culture, 50 ¡l was added to 250 ¡l of modified SM broth in a 96-well plate to be grown at 30°C for 18 h with continuous medium shaking, and OD600 readings were taken every 20 min in a BioTek Synergy HT plate reader. Each experiment was performed three times independently with 6 replicates per strain. Nine mutants were tested per plate, with P. ananatis BRT175 being used as a reference control for each set of mutants. Only one mutant per affected gene was tested (Table 2). Figure S1 in the supplemental material was generated in R using ggplot2 (72, 73).

Nucleotide sequence accession numbers. The rhlA and rhlB genes from P. ananatis 15320, BRT98, Cit30-11, 26SR6, and 17671 have been deposited in GenBank under accession numbers KM819089, KM819090, KM819091, KM819092, KT455465, KT455466, KT455467, KT455468, KT455469, and KT455470.

C/J ~D


Supplemental material for this article may be found at mSphere.00075-15.

Figure S1, PDF file, 628 KB.


We acknowledge the kind contributions of Steven Lindow, Teresa Coutinho, Gwyn Beattie, and the International Collection of Microorganisms from Plants. We thank Andrew Cameron, Tzu-Chiao Chao, Dae-Yeon Suh, Lucas Robinson, Alyssa Walterson, and Morgan Kirzinger for their valuable input and feedback on the manuscript. We thank the dictyBase organization for being an invaluable resource and for providing the

D. discoideum strain used in this work.

This work was funded by Discovery Grants from the Natural Sciences and Engineering Research Council of Canada to J.S. and E.D., a Leaders Opportunity Fund (no. 28591) from the Canada Foundation for Innovation to J.S., and the University of Regina Faculty of Science. D.D.N.S. was supported by a Canadian Institutes of Health Research Master's Award and University of Regina Faculty of Graduate Studies and Research scholarships.

E.D. holds the Canada Research Chair in Sociomicrobiology.


Government of Canada | Natural Sciences and Engineering Research Council of Canada (NSERC) provided funding to John Stavrinides and Eric Deziel. Government of Canada | Canadian Institutes of Health Research (CIHR) provided funding to Derek D. N. Smith. Canada Foundation for Innovation (CFI) provided funding to John Stavrinides.


1. Bergman KA, Arends JP, Scholvinck EH. 2007. Pantoea agglomerans septicemia in three newborn infants. Pediatr Infect Dis J 26:453-454.

2. Shubov A, Jagannathan P, Chin-Hong PV. 2011. Pantoea agglomerans pneumonia in a heart-lung transplant recipient: case report and a review of an emerging pathogen in immunocompromised hosts. Transpl Infect Dis 13:536-539. De Baere T, Verhelst R, Labit C, Verschraegen G, Wauters G, Claeys G, Vaneechoutte M. 2004. Bacteremic infection with Pantoea ananatis. J Clin Microbiol 42:4393-4395. -4395.2004.

Lalas KM, Erichsen D. 2010. Sporadic Pantoea agglomerans bacteremia in a near-term female: case report and review of literature. Jpn J Infect Dis 63:290-291.

Cheng A, Liu C, Tsai H, Hsu M, Yang C, Huang Y, Liao C, Hsueh P.

2013. Bacteremia caused by Pantoea agglomerans at a medical center in Taiwan, 2000-2010. J Microbiol Immunol Infect 46:187-194. http://

6. Cruz AT, Cazacu AC, Allen CH. 2007. Pantoea agglomerans, a plant pathogen causing human disease. J Clin Microbiol 45:1989-1992. http://

7. De Champs C, Le Seaux S, Dubost JJ, Boisgard S, Sauvezie B, Sirot J. 2000. Isolation of Pantoea agglomerans in two cases of septic monoarthritis after plant thorn and wood sliver injuries. J Clin Microbiol 38:460-461.

8. Habsah H, Zeehaida M, Van Rostenberghe H, Noraida R, Wan Pauzi WI, Fatimah I, Rosliza AR, Nik Sharimah NY, Maimunah H. 2005. An outbreak of Pantoea spp. in a neonatal intensive care unit secondary to contaminated parenteral nutrition. J Hosp Infect 61:213-218. http://

9. Coutinho TA, Venter SN. 2009. Pantoea ananatis: an unconventional plant pathogen. Mol Plant Pathol 10:325-335. j.1364-3703.2009.00542.x.

10. Walterson AM, Stavrinides J. 2015. Pantoea: insights into a highly versatile and diverse genus within the Enterobacteriaceae. FEMS Microbiol Rev 39:968-984.

11. Serrano F. 1928. Bacterial fruitlet brown rot on pineapple in the Philippines. Philipp J Sci 36:271-305.

12. Volksch B, Thon S, Jacobsen ID, Gube M. 2009. Polyphasic study of

plant- and clinic-associated Pantoea agglomerans strains reveals indistinguishable virulence potential. Infect Genet Evol 9:1381-1391. http://

13. Nadarasah G, Stavrinides J. 2014. Quantitative evaluation of the host-colonizing capabilities of the enteric bacterium Pantoea using plant and insect hosts. Microbiology 160:602-615. mic.0.073452-0.

14. Kirzinger MWB, Nadarasah G, Stavrinides J. 2011. Insights into cross-kingdom plant pathogenic bacteria. Genes (Basel) 2:980-997. http://

15. Nadarasah G, Stavrinides J. 2011. Insects as alternative hosts for phytopathogenic bacteria. FEMS Microbiol Rev 35:555-575. http://

16. Stavrinides J, No A, Ochman H. 2010. A single genetic locus in the phytopathogen Pantoea stewartii enables gut colonization and patho-genicity in an insect host. Environ Microbiol 12:147-155. http://

17. De Maayer P, Chan WY, Rubagotti E, Venter SN, Toth IK, Birch PR, Coutinho TA. 2014. Analysis of the Pantoea ananatis pan-genome reveals factors underlying its ability to colonize and interact with plant, insect and vertebrate hosts. BMC Genomics 15:404. 10.1186/1471-2164-15-404.

18. Shyntum D, Venter S, Moleleki L, Toth I, Coutinho T. 2014. Comparative genomics of type VI secretion systems in strains of Pantoea ananatis from different environments. BMC Genomics 15:163. http://

19. Kirzinger MWB, Stavrinides J. 2012. Host specificity determinants as a genetic continuum. Trends Microbiol 20:88-93. 10.1016/j.tim.2011.11.006.

20. Kirzinger MWB, Butz CJ, Stavrinides J. 2015. Inheritance of Pantoea type III secretion systems through both vertical and horizontal transfer. Mol Genet Genomics 290:2075-2088. -015-1062-2.

21. Cosson P, Soldati T. 2008. Eat, kill or die: when amoeba meets bacteria. Curr Opin Microbiol 11:271-276. j.mib.2008.05.005.

22. Hasselbring BM, Patel MK, Schell MA. 2011. Dictyostelium discoideum as a model system for identification of Burkholderia pseudomallei viru-


C/J ~D

c a CD 2


lence factors. Infect Immun 79:2079-2088. IAI.01233-10.

23. Pan Y, Lin T, Hsu C, Wang J. 2011. Use of a Dictyostelium model for isolation of genetic loci associated with phagocytosis and virulence in Klebsiella pneumoniae. Infect Immun 79:997-1006. 10.1128/IAI.00906-10.

24. Lelong E, Marchetti A, Simon M, Burns JL, van Delden C, Köhler T, Cosson P. 2011. Evolution of Pseudomonas aeruginosa virulence in infected patients revealed in a Dictyostelium discoideum host model. Clin Microbiol Infect 17:1415-1420. -0691.2010.03431.x.

25. Alibaud L, Köhler T, Coudray A, Prigent-Combaret C, Bergeret E, Perrin J, Benghezal M, Reimmann C, Gauthier Y, Van Delden C, Attree I, Fauvarque M, Cosson P. 2008. Pseudomonas aeruginosa virulence genes identified in a Dictyostelium host model. Cell Microbiol 10:729 -740.

26. Froquet R, Lelong E, Marchetti A, Cosson P. 2008. Dictyostelium discoideum: a model host to measure bacterial virulence. Nat Protoc 4:25-30.

27. Pukatzki S, Kessin RH, Mekalanos JJ. 2002. The human pathogen Pseudomonas aeruginosa utilizes conserved virulence pathways to infect the social amoeba Dictyostelium discoideum. Proc Natl Acad Sci U S A 99:3159-3164.

28. MacIntyre DL, Miyata ST, Kitaoka M, Pukatzki S. 2010. The Vibrio cholerae type VI secretion system displays antimicrobial properties. Proc Natl Acad Sci U S A 107:19520-19524. pnas.1012931107.

29. Sperandio D, Decoin V, Latour X, Mijouin L, Hillion M, Feuilloley MGJ, Orange N, Merieau A. 2012. Virulence of the Pseudomonas fluo-rescens clinical strain MFN1032 towards Dictyostelium discoideum and macrophages in relation with type III secretion system. BMC Microbiol 12:223.

30. Cosson P, Zulianello L, Join-Lambert O, Faurisson F, Gebbie L, Benghezal M, Van Delden C, Curty LK, Köhler T. 2002. Pseudomonas aeruginosa virulence analyzed in a Dictyostelium discoideum host system. J Bacteriol 184:3027-3033. -3033.2002.

31. Totsika M, Heras B, Wurpel DJ, Schembri MA. 2009. Characterization of two homologous disulfide bond systems involved in virulence factor biogenesis in uropathogenic Escherichia coli CFT073. J Bacteriol 191: 3901-3908.

32. Qin A, Scott DW, Mann BJ. 2008. Francisella tularensis subsp. tularensis Schu S4 disulfide bond formation protein B, but not an RND-type efflux pump, is required for virulence. Infect Immun 76:3086-3092. http://

33. Denoncin K, Collet J. 2013. Disulfide bond formation in the bacterial periplasm: major achievements and challenges ahead. Antioxid Redox Signal 19:63-71.

34. Bjur E, Eriksson-Ygberg S, Âslund F, Rhen M. 2006. Thioredoxin 1 promotes intracellular replication and virulence of Salmonella enterica serovar Typhimurium. Infect Immun 74:5140-5151. 10.1128/IAI.00449-06.

35. Abdel-Mawgoud AM, Hausmann R, Lépine F, Müller MM, Déziel E. 2011. Rhamnolipids: detection, analysis, biosynthesis, genetic regulation, and bioengineering of production, p 13-55. In Soberon-Chavez G (ed), Biosurfactants: from genes to applications. Springer, Berlin, Germany.

36. Alexeyev MF, Shokolenko IN, Croughan TP. 1995. Improved antibiotic-resistance gene cassettes and omega elements for Escherichia coli vector construction and in vitro deletion/insertion mutagenesis. Gene 160:63-67.

37. Alexeyev MF, Shokolenko IN, Croughan TP. 1995. New mini-Tn5 derivatives for insertion mutagenesis and genetic engineering in gramnegative bacteria. Can J Microbiol 41:1053-1055. 10.1139/m95-147.

38. Abdel-Mawgoud AM, Lépine F, Déziel E. 2010. Rhamnolipids: diversity of structures, microbial origins and roles. Appl Microbiol Biotechnol 86:1323-1336.

39. Caiazza NC, Shanks RMQ, OToole GA. 2005. Rhamnolipids modulate swarming motility patterns of Pseudomonas aeruginosa. J Bacteriol 187: 7351-7361.

40. Déziel E, Lépine F, Milot S, Villemur R. 2003. rhlA is required for the production of a novel biosurfactant promoting swarming motility in Pseudomonas aeruginosa: 3-(3-hydroxyalkanoyloxy)alkanoic acids

(HAAs), the precursors of rhamnolipids. Microbiology 149:2005-2013. http://dx.doi.Org/10.1099/mic.0.26154-0.

41. Nickzad A, Lepine F, Deziel E. 2015. Quorum sensing controls swarming motility of Burkholderia glumae through regulation of rhamnolipids. PLoS One 10:e0128509. journal.pone.0128509.

42. Kearns DB. 2010. A field guide to bacterial swarming motility. Nat Rev Microbiol 8:634-644.

43. De Maayer P, Chan WY, Venter SN, Toth IK, Birch PRJ, Joubert F, Coutinho TA. 2010. Genome sequence of Pantoea ananatis LMG20103, the causative agent of eucalyptus blight and dieback J Bacteriol 192: 2936-2937.

44. De Maayer P, Chan WY, Rezzonico F, Bühlmann A, Venter SN, Blom J, Goesmann A, Frey JE, Smits THM, Duffy B, Coutinho TA. 2012. Complete genome sequence of clinical isolate Pantoea ananatis LMG 5342. J Bacteriol 194:1615-1616.

45. Sillo A, Matthias J, Konertz R, Bozzaro S, Eichinger L. 2011. Salmonella typhimurium is pathogenic for Dictyostelium cells and subverts the starvation response. Cell Microbiol 13:1793-1811. 10.1111/j.1462-5822.2011.01662.x.

46. Smith DDN, Kirzinger MWB, Stavrinides J. 2013. Draft genome sequence of the antibiotic-producing epiphytic isolate Pantoea ananatis BRT175. Genome Announc 1:e00902-13. genomeA.00902-13.

47. Pukatzki S, Ma AT, Sturtevant D, Krastins B, Sarracino D, Nelson WC, Heidelberg JF, Mekalanos JJ. 2006. Identification of a conserved bacterial protein secretion system in Vibrio cholerae using the Dictyostelium host model system. Proc Natl Acad Sci U S A 103:1528-1533. http://

48. Pradel E, Zhang Y, Pujol N, Matsuyama T, Bargmann CI, Ewbank JJ. 2007. Detection and avoidance of a natural product from the pathogenic bacterium Serratia marcescens by Caenorhabditis elegans. Proc Natl Acad Sci U S A 104:2295-2300.

49. Antunes LCM, Ferreira RBR, Buckner MMC, Finlay BB. 2010. Quorum sensing in bacterial virulence. Microbiology 156:2271-2282. http://

50. Pearson JP, Pesci EC, Iglewski BH. 1997. Roles of Pseudomonas aerugi-nosa las and rhl quorum-sensing systems in control of elastase and rhamnolipid biosynthesis genes. J Bacteriol 179:5756-5767.

51. Deep A, Chaudhary U, Gupta V. 2011. Quorum sensing and bacterial pathogenicity: from molecules to disease. J Lab Physicians 3:4-11.

52. Zulianello L, Canard C, Köhler T, Caille D, Lacroix J, Meda P. 2006. Rhamnolipids are virulence factors that promote early infiltration of primary human airway epithelia by Pseudomonas aeruginosa. Infect Immun 74:3134-3147.

53. Jensen PO, Bjarnsholt T, Phipps R, Rasmussen TB, Calum H, Christoffersen L, Moser C, Williams P, Pressler T, Givskov M, Hoiby N. 2007. Rapid necrotic killing of polymorphonuclear leukocytes is caused by quorum-sensing-controlled production of rhamnolipid by Pseudomonas aeruginosa. Microbiology 153:1329-1338. mic.0.2006/003863-0.

54. Häussler S, Rohde M, von Neuhoff N, Nimtz M, Steinmetz I. 2003. Structural and functional cellular changes induced by Burkholderia pseu-domallei rhamnolipid. Infect Immun 71:2970-2975. 10.1128/IAI.71.5.2970-2975.2003.

55. Ochsner UA, Fiechter A, Reiser J. 1994. Isolation, characterization, and expression in Escherichia coli of the Pseudomonas aeruginosa rhlAB genes encoding a rhamnosyltransferase involved in rhamnolipid biosurfactant synthesis. J Biol Chem 269:19787-19795.

56. Dubeau D, Deziel E, Woods DE, Lepine F. 2009. Burkholderia thailan-densis harbors two identical rhl gene clusters responsible for the biosynthesis of rhamnolipids. BMC Microbiol 9:263. 10.1186/1471-2180-9-263.

57. Rahim R, Ochsner UA, Olvera C, Graninger M, Messner P, Lam JS, Soberön-Chavez G. 2001. Cloning and functional characterization of the Pseudomonas aeruginosa rhlC gene that encodes rhamnosyltransferase 2, an enzyme responsible for di-rhamnolipid biosynthesis. Mol Microbiol 40: 708-718.

58. Deziel E, Lepine F, Milot S, Villemur R. 2000. Mass spectrometry monitoring of rhamnolipids from a growing culture of Pseudomonas aeruginosa strain 57rp. Biochim Biophys Acta 1485:145-152. http://

59. Tremblay J, Richardson A, Lepine F, Deziel E. 2007. Self-produced



с a CD 2


extracellular stimuli modulate the Pseudomonas aeruginosa swarming motility behaviour. Environ Microbiol 9:2622-2630. 10.1111/j.1462-2920.2007.01396.x.

Brüssow H. 2007. Bacteria between protists and phages: from antip-redation strategies to the evolution of pathogenicity. Mol Microbiol 65:583-589. Matz C, Kjelleberg S. 2005. Off the hook—how bacteria survive protozoan grazing. Trends Microbiol 13:302-307. j.tim.2005.05.009.

Brown SP, Cornforth DM, Mideo N. 2012. Evolution of virulence in opportunistic pathogens: generalism, plasticity, and control. Trends Microbiol 20:336 -342. Adiba S, Nizak C, van Baalen M, Denamur E, Depaulis F. 2010. From grazing resistance to pathogenesis: the coincidental evolution of virulence factors. PLoS One 5:e11882. journal.pone.0011882.

Fey P, Kowal AS, Gaudet P, Pilcher KE, Chisholm RL. 2007. Protocols for growth and development of Dictyostelium discoideum. Nat Protoc 2:1307-1316.

65. Sussman M. 1966. Biochemical and genetic methods in the study of cellular slime mold development, p 397-410. In Prescott D (ed), Methods in cell physiology, vol 2. Academic Press, New York, NY.

66. Ochman H, Gerber AS, Hartl DL. 1988. Genetic applications of an inverse polymerase chain reaction. Genetics 120:621-623.

67. Guerra-Santos L, Kappeli O, Fiechter A. 1984. Pseudomonas aerugi-nosa biosurfactant production in continuous culture with glucose as carbon source. Appl Environ Microbiol 48:301-305.

68. Dinno A. 2015. Dunn.Test: Dunn's test of multiple comparisons using rank sums. R package version 1.2.4. R Foundation for Statistical Computing, Vienna, Austria.

69. Abdel-Mawgoud AM, Lepine F, Deziel E. 2014. Liquid chromatography/ mass spectrometry for the identification and quantification of rhamnolipids. Methods Mol Biol 1149:359-373. -0473-0_30.

70. Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. 2013. MEGA6: Molecular Evolutionary Genetics Analysis version 6.0. Mol Biol Evol 30:2725-2729.

71. Hall BG, Acar H, Nandipati A, Barlow M. 2014. Growth rates made easy. Mol Biol Evol 31:232-238. mst187.

72. R Core Team. 2014. R: a language and environment for statistical computing. R Foundation for Statistical Computing, Vienna, Austria.

73. Wickham H. 2009. ggplot2: elegant graphics for data analysis. Springer, New York, NY.

74. Kessler B, De Lorenzo V, Timmis KN. 1992. A general system to integrate lacZ fusions into the chromosomes of gram-negative eubacteria: regulation of the Pm promoter of the TOL plasmid studied with all controlling elements in monocopy. Mol Gen Genet 233:293-301.

75. Fey P, Dodson RJ, Basu S, Chisholm RL. 2013. One stop shop for everything Dictyostelium: DictyBase and the Dicty Stock Center in 2012. Methods Mol Biol 983:59-92. -302-2_4.