ORIGINAL RESEARCH article
The Potato Yam Phyllosphere Ectosymbiont Paraburkholderia sp. Msb3 Is a Potent Growth Promotor in Tomato
- 1Molecular Systems Biology (MOSYS), Department of Functional and Evolutionary Ecology, University of Vienna, Vienna, Austria
- 2Vienna Metabolomics Center (VIME), University of Vienna, Vienna, Austria
- 3Division of Structural and Functional Botany, Department of Botany and Biodiversity Research, University of Vienna, Vienna, Austria
- 4Research Unit for Comparative Microbiome Analysis, German Research Center for Environmental Health, Helmholtz Zentrum München, Neuherberg, Germany
- 5Archaea Biology and Ecogenomics Division, Department of Functional and Evolutionary Ecology, University of Vienna, Vienna, Austria
The genus Paraburkholderia includes a variety of species with promising features for sustainable biotechnological solutions in agriculture through increasing crop productivity. Here, we present a novel Paraburkholderia isolate, a permanent and predominant member of the Dioscoreae bulbifera (yam family, Dioscoreaceae) phyllosphere, making up to 25% of the microbial community on leaf acumens. The 8.5 Mbp genome of isolate Msb3 encodes an unprecedented combination of features mediating a beneficial plant-associated lifestyle, including biological nitrogen fixation (BNF), plant hormone regulation, detoxification of various xenobiotics, degradation of aromatic compounds and multiple protein secretion systems including both T3SS and T6SS. The isolate exhibits significant growth promotion when applied to agriculturally important plants such as tomato, by increasing the total dry biomass by up to 40%. The open question about the “beneficial” nature of this strain led us to investigate ecological and generic boundaries in Burkholderia sensu lato. In a refined phylogeny including 279 Burkholderia sensu lato isolates strain Msb3 clusters within Clade I Paraburkholderia, which also includes few opportunistic strains that can potentially act as pathogens, as revealed by our ecological meta-data analysis. In fact, we demonstrate that all genera originating from the “plant beneficial and environmental” (PBE) Burkholderia species cluster include opportunists. This indicates that further functional examinations are needed before safe application of these strains in sustainable agricultural settings can be assured.
Plants harbor diverse microbial communities whose members can establish a wide range of beneficial interactions with their host. At the root level many of these interactions have been heavily studied (Philippot et al., 2013) and the findings, usually concerning facultative mutualistic associations, have revolutionized our understanding of plants and agricultural processes. Much less focus has been directed toward the phyllosphere of plants, and despite findings outlining the importance of this habitat, our understanding of it is still lacking behind while the major focus is still on understanding plant-pathogen interactions (Vorholt, 2012).
Certain bacterial groups are commonly found in plant shaped environments, as for example members of the Burkholderia sensu lato (s.l.) species complex. Many members of Burkholderia s.l. have been isolated and observed in association to plants; some as pathogens (Burkholder, 1942, 1950; Lee et al., 2005) or as plant growth promoting rhizobacteria (PGPR) and β-rhizobia (Estrada-De Los Santos et al., 2001; Compant et al., 2008; Suarez-Moreno et al., 2012) and others as secondary metabolite producing wardens of their host plant (Van Oevelen, 2002; Lemaire et al., 2011; Carlier and Eberl, 2012; Lemaire et al., 2012a, b; Sieber et al., 2015; Carlier et al., 2016; Pinto-Carbo et al., 2018). The later are of exceptional nature, as they usually colonize glandular structures within the leaf mesophyll, referred to as “leaf-nodules.” These phyllosphere colonizers affiliated with the genus Caballeronia are thought to produce secondary metabolites to protect their hosts from herbivores. These obligate symbionts are uncultivable and have largely reduced genomes (Carlier and Eberl, 2012; Pinto-Carbo et al., 2016). This discovery gave great relevance to the leaf as an important habitat for beneficial interactions and to Burkholderia s.l. species as beneficial interaction partners. The specificity of the symbiosis, however, confines efforts trying to transfer these traits or species to economically important crop plants. Recently, the occurrence of the leaf nodule symbiosis has been described in the yam family, Dioscoreaecea (Carlier et al., 2017; Pinto-Carbo et al., 2018; De Meyer et al., 2019). The sansibar yam, Dioscorea sansibarensis, is considered the only species of the monocot family, in which nodule formation occurs, and interestingly, the facultative symbiont, Orrella dioscoreae, carries a large genome and can be cultured. It belongs to the family Alcaligenaceae within the order Burkholderiales. In this interaction the bacteria invade a pre-existing gland, formed by a folding of the upper-epidermis on the leaf acumen. Trichomes develop into the bacteria-filled lumen. They are thought to play a role in the exchange of nutrients (Miller and Reporter, 1987; Carlier et al., 2017).
In the present study we investigate the prevalence of a bacterial strain of the genus Paraburkholderia in the phyllosphere of the potato yam, Dioscorea bulbifera (L.), an edible yam species cultivated in large parts of the tropics due to its potato-like aerial tubers. Similar to D. sansibarensis, D. bulbifera possesses prominent leaf acumens and they are densely covered with secretory trichomes. As most other known cases of leaf symbiosis are conserved throughout entire lineages (Lemaire et al., 2011), we hypothesized that the tendency of D. sansibarensis to engage in beneficial associations with bacterial partners may be mirrored in closely related non-nodulated Dioscorea species. Indeed, we detected and isolated Paraburkholderia sp. strain Msb3 from leaf acumens of Dioscorea bulbifera. Here, we describe its ecology and its potential. To gain insights into its role on its host plant, its genetic and metabolic repertoire and its potential for agricultural applications we conducted targeted amplicon sequencing experiments on its host, sequenced and annotated its genome, determined its phylogenetic position and tested its performance in plant growth assays. We hypothesize that this association represents an early stage in the development of a more intimate symbiotic association as described in D. sansibarensis and propose to use strain Msb3 as a model to study the genetic prerequisites for such a development and to determine its effect on other plant hosts. Additionally, to tackle safety concerns associated with bacteria of the Burkholderia s.l. species complex, we analyze a large amount of metadata in order to map opportunistic pathogenicity within Burkholderia s.l. onto a robust phylogenetic framework and challenge many earlier generalizations.
Materials and Methods
Several D. bulbifera individuals were raised from bulbils and were grown in the greenhouse under natural photoperiods at 25 ± 5°C. The parent bulbil has been propagated in the greenhouse through reproductive underground tubers for a number of years before the present study. The plants used for the present study were raised in 20 L pots containing seven parts garden soil (150−600 mg L–1 N, 150−600 mg L–1 P2O5, 200−900 mg L–1 K2O, 150 mg L–1 Mg, pH = 5–6.5) (Franz Kranzinger GmbH, Spezialerden-Erzeugung, Straßwalchen, Austria), one part perlite and one part quartz sand (grain size 0.5 mm) and were consistently fertilized throughout their growth period using 0.05% WUXAL® Super (Hauert MANNA Düngerwerke GmbH, Nürnberg, Germany) consisting of 8% N (2.3% NO3–, 3.7% NH4+, 2% Urea), 8% P2O5, 6% K2O and trace elements in water (conductivity 0.51 mS). Leaves used for analysis were clipped from the vine. Experiments were conducted on greenhouse grown plants over a period of 3 years: isolation of bacteria and initial detection through amplification of target genes was performed during its growth period in autumn and winter of 2017/2018. Samples used for community profiling through amplicon sequencing and re-cultivation of strain Msb3 were taken in the subsequent natural growth period in the autumn of 2018. Samples used for microscopic analyses and localization of bacteria through general DNA staining procedures were harvested throughout both of these periods. Leaves used for fluorescence in situ hybridization (FISH) for the specific detection of Burkholderia s.l. species were harvested between December 2019 and February 2020.
Isolation of Bacteria
Fresh leaves were rinsed briefly with water and subsequently divided into ca. 2 cm x 4 cm pieces. The pieces were surface-sterilized in a 2.8% (w/v) sodium hypochlorite (NaClO) solution for 5 min, in ethanol (EtOH) for 1 min and sterile ddH2O for 1 min. Leaf acumens and sections were carefully ground with sterile mortar and pestle in 2 mL of sterile 0.4% sodium chloride solution. Serial dilutions were plated on tryptic soy agar medium (TSA) (7.5 g agar in 1 L tryptic soy broth medium, TSB) (Carl Roth GmbH & Co., KG, Karlsruhe, Germany) and incubated aerobically at room temperature (RT) (ca. 22°C) in the dark for 48 h. Single bacterial colonies were transferred to a new TSA plate and clonal colonies were used for colony PCR. Bacteria were stored in 30% glycerol in TSB at −80°C after initial identification. All subsequent analyses were done with bacteria grown from a cryo-stock batch generated from a clonal colony directly after its identification to ensure plasmid preservation.
Physico-Chemical Characterization of Strain Msb3
The effect of different temperatures and antibiotics was examined by growing bacteria on plate (TSA) as well as in liquid culture (TSB). Growth on TSA was used to determine temperature boundaries, then growth rates at different temperatures were determined through comparison of the optical density (OD) at 600 nm of bacteria that were inoculated to a starting OD600 of 0.05, grown in 200 mL TSB in Erlenmeyer flasks, steadily shaking at 200 rpm for 24 h. All conditions were grown in triplicates and technical triplicates were measured for individual flasks. Temperatures tested included 20°C, 22°C, 25°C, 30°C, 35°C, 36°C, 37°C, and 42°C. The same approach was used to determine the minimal inhibitory concentrations of following antibiotics: ampicillin (50−200 μg/mL); cefalexin (10−40 μg/mL); chloramphenicol (12.5−50 μg/mL); carbenicillin (50−100 μg/mL); streptomycin (25−50 μg/mL); and kanamycin (50−200 μg/mL).
Growth enabled by utilization of a specific substrate as sole carbon source was determined by comparison of the OD600 following growth in 1 × M9 salts minimal medium (Sigma-Aldrich Handels GmbH, Vienna, Austria) containing 2 mM MgSO4 and 0.1 mM CaCl2 with and without addition of test substrate, comparing relative growth after 16 h to glucose (100%) as a control.
DNA Extraction From Pure Culture
Strain Msb3 was grown from cryo-stock in liquid culture overnight at RT in TSB (Carl Roth GmbH & Co., KG). 4 mL (OD600 = 0.8) were transferred into a 15 mL tube and centrifuged at 2400 × g for 8 min to sediment biomass. Cells were washed in TE and subsequently lysed using lysozyme (Thermo Fisher Scientific, Waltham, MA, United States). Lytic activity was stopped using Proteinase K (Thermo Fisher Scientific). This approach was chosen to prevent excessive shearing of DNA molecules in order to produce long sequencing reads. Extraction of total chromosomal and plasmid DNA was performed following a standard phenol/chloroform/isoamyl alcohol (PCI) extraction protocol as described below.
DNA Extractions From Plants
Leaves and leaf acumens of D. bulbifera were either surface sterilized with NaClO for 3 min, followed by EtOH for 1 min and washed with ddH2O (9 × 30 s) or left untreated. Due to insufficiently clean DNA for reproducible downstream applications using standard procedures we comprised a new PCI (Thermo Fisher Scientific) based extraction protocol for clean nucleic acid extraction from plants. The crude plant extract is mixed with a polyvinylpolypyrrolidon (PVPP) suspension which binds tannins and polyphenols and the mixture can subsequently be removed with particles through centrifugation. The method presented here is a modified version of the PVPP based protocol presented by Kasajima et al. (2013) and relies on the same principal. DNA was extracted from 25−100 mg of dried or frozen leaf tissue. The homogenized tissue was mixed and washed with alkaline PVPP buffer (Tris–HCl, pH 9.5, 50 mM; EDTA, 10 mM; NaCl, 4 M; CTAB, 1%; PVPP, 0.5%; 2-mercaptoethanol, 1%) and the supernatant was used for further DNA extraction following a standard PCI protocol. Chloroform phase separation was repeated three times to enhance phenol residue removal. DNA was precipitated in 0.03 M NaOAc and 70% EtOH at −20°C or 0.05 M NaCl and isopropanol at RT for 1 h and stored in ddH2O at −20°C.
PCR Amplification and Sequencing of gyrB and 16S rRNA Genes
DNA extracted from D. bulbifera as well as colonies grown on agar plate were used as a template for amplification. Primers 27F/1492R (Frank et al., 2008) were used to amplify 16S rRNA genes. For the amplification of gyrB-genes the genus specific primer pair “gyrB,” designed by Spilker et al. (2009) for the genus Burkholderia s.l. was used. All oligonucleotides used in this study were obtained from Microsynth (Microsynth AG, Balgach, Switzerland) and are summarized in Table 1.
Amplification of target DNA with the DreamTaq DNA Polymerase (Thermo Fisher Scientific) was performed in a 30 μL reaction volume, consisting of 21.05 μL sterile ddH2O, 6 μL 10x Dream Taq Green Buffer (incl. 20 mM MgCl2), 0.6 μL dNTP Solution Mix (10 mM of each dNTP, New England Biolabs, Ipswich, MA, United States), 0.15 μL Dream Taq DNA Polymerase and 0.6 μL 10 mM forward and 0.6 μL 10 mM reverse primer as well as 1 μL template DNA (20 ng/μL for plant extracts and 1 ng/μL for pure culture controls) or a colony lysed in sterile ddH2O. The reaction conditions were as follows: one cycle at 94°C (3 min); 30 cycles at 94°C (30 s), 50°C/60°C (30 s) for 16S rRNA/gyrB, respectively, and 72°C (1 min/2 min for 16S rRNA/gyrB respectively), plus one final cycle at 72°C (6 min).
Amplification with the Phire Hot Start II Polymerase (Thermo Fisher Scientific) was performed in 20 μL reaction mix consisting of 11.6 μL sterile ddH2O, 4 μL 5 x Phire Green Reaction Buffer (1.5 mM MgCl2 final concentration), 0.4 μL dNTP Solution Mix (10 mM of each dNTP), 0.4 μL Phire Hot Start II Polymerase and 1 μL 10 mM forward and 1 μL 10 mM reverse primer as well as 1 μL template DNA (20 ng/μL for plant extracts and 1 ng/μL for controls) or a colony lysed in sterile ddH2O. The reaction conditions were as follows: one cycle at 98°C (2 min); 30 cycles at 98°C (10 s), 48°C/60°C (10 s) for 16S rRNA/gyrB, respectively, and 72°C (20 s/8 s for 16S rRNA/gyrB respectively). Resulting PCR products were purified using a MonarchTM PCR/DNA clean up Kit (New England Biolabs) and Sanger sequenced by Eurofins Genomics (Eurofins Genomics Germany GmbH, Ebersberg, Germany).
Plants were grown in five biological replicates and three leaves per plant were pooled for further analysis. Leaves were divided into two equal parts and one half was surface sterilized, the other half was left untreated. The acumen was always removed and handled individually. Additionally, we collected water that was used to wash the leaf surface from the acumen. DNA quality and quantity were measured via Fragment AnalyzerTM (Advanced Analytical Technologies, Inc., Ankeny, United States). Subsequently, PCR was performed in triplicate using the Phusion Flash High-Fidelity PCR Master Mix (Thermo Fisher Scientific) and primer pair 335F/769R (Dorn-In et al., 2015) to avoid co-amplification of plant and chloroplast DNA in a total volume of 10 μL (10 ng DNA template, 12.5 μL PCR master mix, 10 pmol of each primer). PCR conditions were 10 s at 98°C; 30 cycles of 1 s at 98°C, 5 s at 59°C, 45 s at 72°C; 1 min 72°C. To exclude potential contamination by PCR, a no template sample using water instead of DNA was included in all following steps. PCR products were qualified using gel electrophoresis pooled and purified using Agencourt AMPure® XP beads (Beckman Coulter, Brea, CA, United States). DNA quality and quantity were checked as described above. The subsequent indexing PCR was performed using the Nextera XT Index Kit v2 (Illumina, Inc. San Diego, CA, United States) and the Phusion Flash high-fidelity PCR master mix (Thermo Fisher Scientific) in a total volume of 25 μL (10 ng DNA template, 12.5 μL PCR master mix, 2.5 μL of each index) and the following PCR conditions: 30 s at 98°C; 8 cycles of 10 s at 98°C, 30 s at 55°C, 30 s at 72°C; 5 min 72°C. Indexing PCR products were purified and quantified as described above and pooled in an equimolar ratio of 4 nM. Sequencing was performed using an Illumina Miseq platform (Illumina Inc.) with Reagent Kit v3 (600 cycles).
Sequences were analyzed using the QIIME 2 software package release 2018.8.0 (Caporaso et al., 2010) with default parameters. FASTQ files were trimmed and merged with a minimum read length of 50 and minimum Phred score of 15 using AdapterRemoval (Schubert et al., 2016). The QIIME 2 plugin DADA2 (Callahan et al., 2016) was used for quality control with the following parameters: 10 bp were removed n-terminally, reads were truncated at position 290 (forward) and 220 (reverse), respectively, and expected error was adjusted to 3. The resulting unique amplicon sequence variants (ASVs) are biological sequences discriminated from errors, allowing the detection of single-nucleotide differences over the sequenced gene. The ASV method has demonstrated a better specificity and sensitivity than OTU based methods, which cluster sequencing reads according to a fixed dissimilarity threshold (Callahan et al., 2017). Taxonomic analysis was performed using the SILVA_132_QIIME release 99% as reference database and the classify-consensus-blast option of QIIME 2, setting –p-perc-identity and –p-min-consensus to 0.9 each. PCR negative control showed no ASVs contamination during sample processing. Data was analyzed and visualized using the phyloseq package in R (McMurdie and Holmes, 2013).
Genome Sequencing and Assembly
Library preparation and genome sequencing was conducted by the next generation sequencing (NGS) facility of the Vienna Biocenter Core Facilities GmbH (VBCF, Vienna, Austria) using a PacBio Sequel instrument (Pacific Biosciences of California, Inc., Menlo Park, CA, United States). Subreads were assembled by application of the HGAP4 pipeline (Chin et al., 2013). The quality of the genome assembly was evaluated using QAST v4.4 (Mikheenko et al., 2018). Linear chromosomes and plasmids were circularized using circlator (Hunt et al., 2015).
Genome Annotation and Analysis
Rapid, automated gene prediction was performed using the Prokka software package (Seemann, 2014). Clusters of orthologous groups of proteins (COGs) were assigned using the COGsoft software (Kristensen et al., 2010) running COGtriangles to assign COGs and COGnitor to assign COG function by comparison to the COG database. Macromolecular systems like bacterial protein secretion systems were identified using the MacSyFinder program (Abby et al., 2014) and the sets of models and profiles described by Abby et al. (2016). Additionally, the assembly was uploaded to the web-based MicroScope platform for microbial genome annotation and comparative genomics (Vallenet et al., 20061), where the automatic annotation was manually curated. Pseudogenes were identified and the product description was then curated for all genes considered in detail in this study. All >70% identity matches to a protein with an experimentally verified function were designated with the same product description unless other evidence overruled this annotation. All other product descriptions, except (conserved) hypothetical proteins, were preceded by “putative.” For most coding sequences (CDS) a >90% identity match was found with P. xenovorans strain LB400 with a very well manually curated genome (Chain et al., 2006). Unless new evidence overruled this annotation, it was designated with the same putative function.
Available genomes and phylogenetic marker sequences of Burkholderia, Paraburkholderia and Caballeronia strains were retrieved from GenBank and the Joint Genome Institute’s Integrated Microbial Genomes database (JGI-IMG) as well as the SILVA rRNA database project and the PubMLST db (Jolley et al., 2018). Multiple sequence alignments were created using Mafft (Katoh et al., 2002) and trimmed using BMGE (Criscuolo and Gribaldo, 2010). Trimmed alignments were used to calculate maximum likelihood phylogenomic trees in IQ-Tree (Felsenstein, 1981) displaying ultrafast bootstrap (UF-BS) (Minh et al., 2013) and SH-aLRT (Guindon et al., 2010) values. Trees were manually annotated.
Calculation of ANI Values
ANI values were determined using the JSpeciesWS web server (Richter et al., 2016). The assembly of the Msb3 genome was uploaded to the JSpeciesWS website in FASTA format together with whole genome sequences selected based on tetra-nucleotide usage. ANI analysis was performed with the ANIb algorithm, accessible via the JSpeciesWS web service.2
Plant Growth Promotion Assays
Seeds of tomato (Solanum lycopersicon cv. Moneymaker) were surface sterilized by immersion in 70% (v/v) ethanol for 5 min followed by incubation in 2.8% NaClO for 10 min and subsequently washed with sterile distilled water for 30 min. The treated seeds were placed onto Murashige & Skoog (MS) agar medium including B5 vitamins (Duchefa Biochemie B.V, Haarlem, Netherlands) and germinated in the dark at 22°C. After 10 days seedlings were exposed to light and after 14 days uniform seedlings were selected and inoculated with bacteria. The seedlings were dipped into bacterial suspensions (0.5−5 × 109 CFUs mL–1 in 1 × PBS either live or heat killed via autoclaving) and subsequently transferred to a 300 mL pot containing 60 g of sterilized garden soil (150−600 mg L–1 N, 150−600 mg L–1 P2O5, 200−900 mg L–1 K2O, 150 mg L–1 Mg, pH = 5–6.5) (Franz Kranzinger GmbH). The experiment was performed using nine biological replicates. In a second experiment using only three biological replicates the seedlings were first transferred to pots and after 7 days the soil was inoculated with bacteria. All pots were randomly placed in a growth chamber for 34 days at 22°C, a photoperiod of 16 h (100−130 PPFD, μmol m–2 s–1 at the ground level), and relative humidity of 65%. After 25 days all pots were fertilized once with 20 mL 0.1% WUXAL® Super (Hauert Manna Düngerwerke GmbH) consisting of 8% N (2.3% NO3–, 3.7% NH4+, 2% Urea), 8% P2O5, 6% K2O and trace elements in distilled water (conductivity 0.51 mS). The plants inoculated with autoclave killed bacteria functioned as controls and were grown under the same conditions. The plants were harvested after 34 days. After removal of soil, total biomass fresh weight (FW) and dry weight (DW) as well as partial contributions of shoot and root were determined. Shoot length was measured as distance from its base to the last node of the emergence. Bacteria were re-cultivated from plant roots after homogenization of the tissue in 0.4% NaCl as described above.
For scanning electron microscopic (SEM) analyses cell cultures were first dehydrated with EtOH (in a PBS EtOH mixture starting from 50% stepwise increasing by 10% to a final concentration of 100% EtOH) and subsequently CO2 critical point dried by application of a Leica EM CPD300 (Leica Microsystems GmbH, Wetzlar, Germany) automated critical point dryer. The dried samples were mounted on aluminum stubs and coated with gold for 80 s using a sputter coater (SCD 050; Denton Vacuum LLC). Finally, images were obtained in a JSM-6390 JEOL scanning electron microscope (JEOL Germany GmbH, Freising, Germany).
For production of fluorescent micrographs plant samples were fixed in 2% paraformaldehyde in 1 × PBS (pH = 7.2) for 1 h and subsequently washed in PBS, twice. Samples were then treated according to the respective downstream application. To keep as many bacterial cells on the leaf surface as possible we conducted a “minimal-washing” DNA staining experiment: Nucleic acids were stained by immersion of the specimen in 10 x SYBR® < /cps:sup > -Green I (Thermo Fisher Scientific) in 1 × PBS for 10 min. Excess dye was removed through two additional washing steps. Samples could be imaged directly.
For specific identification of bacteria, FISH analysis was conducted as follows: Treatment with lysozyme solution (1 mg mL–1 in PBS) was applied for 10 min at 37°C and subsequently the samples were dehydrated in a stepwise ethanol series (25, 50, 75, and 99.9%; 15 min each step). Double labeling of oligonucleotide probes for FISH (DOPE-FISH) was performed with probes obtained from Microsynth (Microsynth AG, Balgach, Switzerland) labeled at both the 5′ and 3′ end positions with the respective fluorophore. An EUBmix targeting all bacteria consisting of an equimolar mixture of EUB338-I (Amann et al., 1990), EUB338-II, EUB338-III (Daims et al., 1999), coupled with the fluorochrome ATTO-488, and the Burkholderia s.l. specific probe Burkho (Hogardt et al., 2000), coupled with Cy3, were used for detection of the corresponding bacteria. The non-specific probe NON-EUB (Wallner et al., 1993) was used as a control for unspecific binding on separate samples. Hybridization was carried out at 46°C for 2 h or overnight within Eppendorf tubes containing the hybridization solution (20 mM Tris–HCl pH 8.0, 0.01% w/v SDS, 0.9 M NaCl, 10 ng μL–1 of each probe and 20% or 30% formamide for EUBmix and Burkho, respectively) and the respective plant sample. Post-hybridization was conducted at 48°C for 30 min with a pre-warmed post-FISH solution containing 20 mM Tris–HCl pH 8.0, 0.01% SDS, 5 mM EDTA pH 8.0 and NaCl at a concentration corresponding to the formamide concentration (0.215 M and 0.102 M NaCl for EUBmix and Burkho, respectively). When applied together, the probes were hybridized sequentially, starting with the probe requiring the higher formamide concentration. Samples were rinsed with ice cold distilled water before air drying in the dark. The samples were then observed under a confocal microscope.
Images were taken on a confocal laser scanning microscope (CLSM) (Leica DMRE SP5) (Leica Microsystems). A white light laser was used for excitation of fluorescence signals (SYBR® < /cps:sup > -Safe: ex/em 410/520-540 nm; “chlorophyll autofluorescence”: ex/em 550 or 555/674-716 nm; “trichome specific signal”: ex/em 550 or 555/571-655 nm; Atto-488: ex/em 502/520-540 nm; Cy3: ex/em 550/560-590 nm). The scanning speed was 100 Hz and a 20× or 63× glycerol immersion objective was used for all images. Images were taken sequentially to prevent leaching of fluorescent signals into other channels. Stacks of 15 to 25 optical sections per series were recorded to cover a large range and the fluorescence data was combined in maximum projections using the Leica Application Suite (LAS) X (Leica Microsystems) software platform. Postprocessing included separation of dye signals from Cy3 and plant specific signals using the implemented “Channel Dye Separation” tool via signal informed selection of regions of interest. This was done due to the overlapping emission spectra of Cy3 and plant structures (compare Cy3 and trichome specific emission at excitation with 550 nm). Cy3-channel images and chlorophyll autofluorescence images were used as an input and the processed Cy3-channel image was used to generate montages shown in this manuscript. Non-processed images corresponding to the ones shown in the manuscript can be found in Supplementary Figure 3. Adaptation of brightness and contrast of all images to better suit print and screen representation was conducted through ImageJ version 1.52q (Schneider et al., 2012).
We tested for the significance of an inoculation effect on plant biomass and shoot length in the PGP assay in tomato as well as for a sample condition effect on bacterial read counts in the normalized amplicon sequencing dataset by applying Student’s t-tests. Reported P-values are calculated through two-tailed tests that assume a normal distribution of the data points and equal variance. To test for significant differences between means of abundance values in the normalized amplicon sequencing dataset we applied Tukey’s HSD (honestly significant difference) tests, based on the same assumptions. Values generated through analysis of independent biological replicates functioned as single data points used for the calculation. All analyses were performed in the program R (R Core Team, 2019), version 3.5.3.
Principal coordinate analyses were performed using pairwise, normalized, weighted UniFrac distances between all samples on the normalized ASV tables and the first two principal coordinates were visualized. Data was visualized through the R software packages phyloseq (McMurdie and Holmes, 2013) and vegan (Oksanen et al., 2013) using the plugin ggplot2 (Wickham, 2016).
Isolation of Strain Msb3 From D. bulbifera Leaves
We realized the untapped potential of the leaf as a habitat for beneficial microbial interaction partners and conducted a broad screening in several plant families, including Dioscoreaceae, to detect novel forms of interactions in their phyllosphere. We investigated several Dioscorea species through amplification of marker genes using specific primers (Spilker et al., 2009). Sequencing of the PCR products revealed the presence of a highly abundant gyrB gene that clustered with that of free living cultivable Paraburkholderia species in DNA extracts of greenhouse grown D. bulbifera. In an effort to isolate the strain, serial dilutions of NaClO and EtOH surface sterilized leaves and leaf acumens were plated onto tryptic soy agar (TSA) medium and incubated at room temperature for 48 h. We obtained near to pure cultures from every leaf acumen extract in three biological replicates within two sequential experiments. No colonies were obtained on plates incubated with leaf extract, although the bacteria had been detected in the respective DNA extract (Supplementary Figure 1), likely a result of the harsh sterilization treatment. Amplification of 16S rRNA and gyrB-genes of individualized colonies and alignment to sequences amplified previously confirmed the identity of the isolate. The Paraburkholderia strain was designated Msb3.
We could reproduce cultivation of the strain from leaves harvested a second time in 2017 as well as after completion of an entire growth cycle of the perennial vine in 2018 and qualitative amplification of marker genes during that period showed consistent colonization (data not shown). The following results were obtained from mature leaves harvested in 2018.
Strain Msb3 Dominates the D. bulbifera Acumen Surface Microbiome
To obtain a more detailed view of the microbial community in this environment and the role of strain Msb3 we conducted a 16S rRNA gene-based amplicon sequencing approach with general bacterial primers. The following samples were analyzed: leaves (L), surface-sterile leaves (LS), acumens (A), surface-sterile acumens (AS), and surface microbiota (−S). After analysis of raw reads, trimming, filtering and chimera removal (Supplementary Information), we defined a dataset consisting of 1,112 specific amplicon sequence variants (ASVs). ASVs occurring in extraction and PCR control samples as well as unassigned reads and singletons were removed and subsampling with 17,702 reads was performed, reflecting the lowest read number obtained per sample, to relatively compare chloroplast contaminations in different sample types. We defined a core dataset of 993 ASVs distributed across all samples through removal of plant-sequence-derived ASVs as well as ASVs present in less than 5% of all samples and normalized the final dataset by rarefying to 739 reads per sample. Rarefaction analysis indicated diversity coverage of >99% (Supplementary Figure 2A) and consequently an adequate sampling depth for further analysis.
We explored the data in respect to the relative abundance of Msb3 and closely related taxa in different sample types. We compared all samples via principal coordinate analysis (Supplementary Figure 2B) to dissect major differences between location (L vs. A) and sample type (L vs. LS and A vs. AS, respectively). Surface microbiota, largely represented by γ-Proteobacteria (Supplementary Figure 2C), heavily influence community composition in A compared to AS. These differences become apparent in γ-Proteobacteria fractions (Figures 1A,B). It should be mentioned that we follow the taxonomy of the SILVA SSU Ref NR 99 release 132 in which β-Proteobacteria were reclassified as an order within γ-Proteobacteria following the Genome Taxonomy Database3 (Parks et al., 2018) and so, on an order level A is clearly different from other sample types: the Xanthomonadales subset is larger in A than in others (A vs. L: p = 0.0362; A vs. LS: p = 0.0111), but at the same time these are represented by fewer ASVs and Pseudomonadales, rather dominant in LS and AS, largely disappear (A vs. LS: p = 0.0015; A vs. AS: p = 0.0897). Generally, β-Proteobacteriales are almost exclusively made up of Burkholderiaceae (Figure 1C), whose distribution on a genus level (Figure 1D) is another driver for the separation of these samples. While disinfected samples, AS and LS, display a diverse set of evenly distributed genera within the family, both A and L show a less diverse pattern and especially A a higher fraction of Burkholderia s.l. (A vs. LS: p = 0.0498; A vs. AS: p = 0.0272). Here, Burkholderia s.l. make up 82% of Burkholderiaceae on average. In total Burkholderia s.l. species make up more than 25% of bacterial reads in A, constituting a substantial part. This becomes even more significant considering the bacterial load, approximated by relative abundance of bacterial reads compared to plant/chloroplast derived ASVs (Figure 1E). The summed number of reads per sample type is about two times higher than in other leaf derived samples (Figure 1F) and the read number per sample is consistently and significantly higher (A vs. L: p = 0.0052; A vs. LS: p = 0.0019; A vs. AS: p = 0.0345) (Figure 1G).
Figure 1. ASVs defining the leaf acumen microbiome. (A) Histograms showing the distribution of classes present in the 993 ASVs in samples from the D. bulbifera leaf lamina, untreated (L) and surface sterilized (LS), compared with classes present in those of the leaf acumen, (A and AS). The conditions were analyzed in five biological replicates and, per replicate, three leaves were pooled. (B) Distribution of orders present among the ASVs from the class γ-Proteobacteria. (C) Distribution of families present among the order Betaproteobacteriales, and (D) distribution of genera present in the family Burkholderiaceae. Taxonomic classification follows the current phylogenetic framework used by the SILVA database. (E) Bacterial load per sample type approximated through read count of bacterial ASVs compared to those of plant derived ASVs. (F) Histogram of total bacterial read count summed up per sample type and, (G) read count per sample displayed in a box-plot after removal of plant derived ASVs. Significant differences were determined through applying a two-tailed Student’s t-test, that assumes a normal distribution of the data points and equal variance, to read counts per condition in the normalized dataset. (H) Phylogenetic tree of ASVs that belong to the genus Burkholderia (s.l.). Their prevalence and abundance in certain sample types is represented by colored circles on the branch tip as shown in the legend on the right. (I) Sequence identity matrix of ASVs shown in panel (H) and the resulting OTU classification according to a 97% sequence identity threshold.
We also investigated the diversity and occurrence of ASVs classified as Burkholderia s.l. (Figure 1H) to identify Msb3 as well as other Burkholderia s.l. species. In total 31 ASVs were classified within the genus, and formed four distinct clusters (Figure 1I) in a sequence identity matrix as well as in a phylogenetic tree (Figure 1H). These were defined as operational taxonomic units (OTUs) based on a 97% sequence identity threshold for simplification. All sequences from OTU1 and OTU2 were identified as Clade I Paraburkholderia based on BLAST hits against NCBIs non-redundant nucleotide collection and compared to our own phylogenetic reconstructions (see section “Ecological and Phylogenetic Boundaries in Burkholderia s.l.”). OTU3 could not be identified unambiguously based on the 345 bp sequences but seems to be most closely related to some Caballeronia species and OTU4 is affiliated with Clade II Paraburkholderia. The most abundant ASVs (5, 6, and 218), which belong to OTU1, are at least 99.8% identical to the 16S rRNA gene of strain Msb3. In general, ASVs that belong to OTU1 are most abundant in A (but prevalent in all sample types) and are being reduced or disappear completely with surface sterilization, indicating that they are most abundant on the acumen surface.
Burkholderia s.l. Species Aggregate on Secretory Trichomes
To demonstrate that bacteria are indeed quite abundant on the surface of the D. bulbifera leaf acumen we analyzed parts of the leaves by means of confocal microscopy. In order to visualize bacteria, we stained nucleic acids with a SYBR® Green general DNA stain and made use of the plant autofluorescence signature to image various plant structures in the background. In contrast to the leaf lamina the leaf acumen is densely covered with trichomes that emit a characteristic autofluorescence signal between 571 and 655 nm when excited at 550−555 nm (Figure 2A). This signal can nicely be separated from chlorophyll autofluorescence (em 674−716 nm) as well as that of other plant surface specific structures (cuticle etc.), which suggests the presence of certain compounds within the cell wall or the excretions of the trichome causing the signal. We used the specificity of the signal to reduce the plant associated background while still visualizing the trichomes. Bacteria can indeed be observed in exceptionally high numbers (Figure 2). They consistently occur within large clusters on the surface of trichomes (Figures 2B,C). Interestingly, these clusters could already be observed at very early stages in the development of the leaf, in fact, at a stage where the leaf hardly consists of anything but the acumen. Naturally, this led to the question of the identity of the bacteria. To see whether Burkholderia s.l. species were among the trichome associated microbiota we conducted fluorescence in situ hybridization (FISH) experiments using double labeling of oligonucleotide probes (DOPE-FISH) coupled with confocal laser-scanning microscopy (CLSM). Bacteria were labeled with an Atto488 coupled mix of EUB probes (EUBmix) and members of the Burkholderia s.l. species cluster were labeled with the Cy3 tagged probe Burkho. Indeed, we could show that the bacteria that form clusters on or in between secretory trichomes are almost exclusively Burkholderia s.l. spp. (Figures 3A,B). We also observed other bacteria-like structures after coupling of DOPE-FISH using the Burkho probe and SYBR® Green staining (Supplementary Figure 3). However, these were never observed as clusters on trichomes and, even outside of clusters, the vast majority of cells emitted a Cy3 signal, indicating they, too, were Burkholderia s.l. species.
Figure 2. Microscopic analysis of bacteria associated to secretory trichomes on the D. bulbifera leaf acumen. Confocal laser scanning microscopy (CLSM) images of trichomes located on the upper side of the leaf acumen. Trichome autofluorescence could be separated from other channels and can be observed in cyan, chlorophyll autofluorescence in magenta and nucleic acids were stained with SYBR® < /cps:sup > -Green, here depicted in yellow. Excitation (ex.) and emission (em.) wavelengths are indicated above. (A) Trichomes densely cover the surface of the acumen and microorganisms strongly colocalize with trichomes, as can be observed in panel (B) a magnification of two trichomes in panel (A), as well as in panel (C), showing another pair of trichomes densely colonized by microorganisms. Scale bars represent 20 and 10 μm in panels (A) and (B,C), respectively.
Figure 3. Visualization of clusters of Burkholderia sensu lato spp. associated with secretory trichomes on leaf acumens of Dioscorea bulbifera (potato yam) by DOPE-FISH/CLSM microscopy. EUBmix and Burkho probes were applied onto leaf acumens sequentially and the upper surface of the acumen, which is densely covered with secretory trichomes, was visualized (A). Burkholderia s.l. spp. (white arrows), labeled with both EUBmix (green channel) and Burkho probes (yellow channel), can be observed clustering on the sides of, or in between, secretory trichomes (st, orange arrows) emerging from the upper epidermis (ue, green arrows) of the leaf acumen. In panel (B) a high-resolution image of a cluster on the side of a trichome can be seen, all bacterial cells shown are labeled with the Burkholderia s.l. specific probe.
Strain Msb3 Represents a Novel Paraburkholderia Species
To further analyze the role of strain Msb3 in its occupied niche and its phylogenetic affiliation we sequenced and assembled its genome. Average nucleotide identity (ANI) values were calculated for selected genome pairs from a dataset of 15 genomes of closely related taxa (see Supplementary Information), making use of the JSpecies Web Server (Richter et al., 2016; Table 2 and Supplementary Table 1). The closest relative of strain Msb3 is Burkholderia sp. Ch1-1 with an ANIb value of 98.89% and an alignment fraction (AF) of 0.87. According to the 95% threshold for species delineation (Kim et al., 2014) this classifies them as the same species. Strain Ch1-1 has not been described yet and information concerning its lifestyle is scarce (NCBI BioProject: PRJNA224116) nor is it available in public strain collections. P. xenovorans is the closest classified relative of strain Msb3 and its type strain shares an ANIb value of 93.54% with (AF = 0.78) with strain Msb3, indicating that they are distinct species (Kim et al., 2014). The type strains of P. aromaticivorans and P. phytofirmans are also closely related to strain Msb3 but fall far below the threshold with ANIb values of 89% and 87%, respectively. These results indicate that strain Msb3 represents a novel species.
Table 2. ANIb values and percentage of aligned sequences between selected genomes and the genome of strain Msb3.
Genome of Strain Msb3
General Genome Properties
The genome of strain Msb3 has a size of 8.35 Mbp, harboring 8,199 coding sequences (CDS) distributed over five circular replicons – two chromosomes and three plasmids – designated C1 (4.48 Mbp), C2 (3.5 Mbp), P1 (204 Kbp), P2 (94 Kbp), and P3 (64 Kbp) in agreement with the described P. xenovorans strain LB400 (henceforth LB400) replicon structure (Chain et al., 2006). Origins of replication were determined based on the presence of genes involved in DNA replication close to the predicted origin by G + C skew analysis (Figure 4). The total G + C% of the genome of strain Msb3 is 62.52%. Summed genomic properties are usual for Paraburkholderia species, shown in Table 3 and details concerning plasmids as well as a comparison of replicon specific clusters of orthologous groups of proteins (COG) classification patterns and biases toward certain groups can be observed in Figure 4 and are further discussed in Supplementary Information.
Figure 4. Circular Replicons and COG distribution in the Msb3 Genome. (A) Classification of CDS into functional categories based on clusters of orthologous groups of proteins (COGs) on the two chromosomes. (B) Functional distribution over the five replicons, based on the COG classification. Values in panels (A,B) are shown as the percentage of genes on each replicon belonging to each COG. (C) Representation of circular replicons found in the genome of strain Msb3. Each replicon is sorrounded by a black circle, indicating the size of the contig in Mpb but also reflecting its relative size compared to other replicons. The two chromosomes were investigated in more detail. The meaning of each circle, starting from the outside, is as follows: circle 1 displays contig size in Mpb; circle 2 and 3 display CDS on (+) and (–) strand, respectively; circle 4 shows the location of RNAs on each chromosome, rRNAs in red and tRNAs in black; circle 5 carries COG functional classifications of each CDS classified within a COG; circle 6–8 show genomic islands of strain Msb3 when compared to its closest relatives, where circle 6 represents PsJN, circle 7 represents LB400 and circle 8 Ch1-1: a blue box is a genomic island with more than 40% of all CDS within the region absent from the relatives’ genome and a red box an island with 100% of CDS absent from the genome of the close relative. Circle 9 displays a histogram of the G + C content (mol%) calculated per gene, relative to the average of the whole genome (62.55 mol%). Circle 10 shows cumulative G + C skew calculations in steps of 1000 bp, relative to 0.
Strain Msb3 carries a large genome shaped for versatility. A total of 3,378 CDS classified within COGs related to metabolic processes present a large repertoire of genes executing various metabolic functions. Through analysis of carbohydrate metabolism and transport we can infer a heterotrophic or potentially mixotrophic growth mode for strain Msb3. A detailed reconstruction of strain Msb3s primary metabolism can be found in Supplementary Information. Noteworthy is the identification of several putative TRAP-family dicarboxylic acid transporters, suggesting that C4 dicarboxylic acids could be used for energy production through enzymatic carboxylate degradation in the tricarboxylic acid (TCA) cycle. Interestingly, specific TRAP transporters were found among genes shared only by strain Msb3 and P. phytofirmans strain PsJN (henceforth PsJN) but not LB400, indicating that adaptations to specific environmental niches may have reshaped central carbon acquisition strategies. Phenotypic assays were conducted showing aerobic growth on malate and citrate. Dicarboxylic acids are among the preferred substrates for growth and may provide energy and a source of carbon for growth in planta.
Nitrogen metabolism encompasses most features usually found within most relatives of strain Msb3. The presence of an entire nif nitrogen fixation gene cluster located on C2 is worth mentioning as this could enable the strain to perform BNF, a feature that is lacking from the PsJN genome. More information can be retrieved from Supplementary Information and Supplementary Table 2.
On C2 we identified a non-ribosomal peptide synthetase (NRPS) consisting of a two-protein core cluster, an “amino acid adenylation enzyme/thioester reductase family protein” as well as a “non-ribosomal peptide synthase/amino acid adenylation enzyme” predicted by antiSMASH, and a border cluster containing an ABC-superfamily cyclic peptide transporter as well as all necessary transport system components. Gene clusters predicted to produce some bacteriocins were detected on both chromosomes, including one responsible for linocin-M18 production.
Terpenoid biosynthesis is also prominently represented by three protein clusters, two of which encode a putative squalene synthase (SQS), responsible for the catalytic reduction of two farnesyl pyrophosphate molecules to squalene through the consumption of NADPH. Squalene is a parent molecule of cyclic triterpenoids. Appropriately, we found a hpn (hopanoid biosynthesis) operon (hpnBCDEN, shc, nifB). It encodes enzymes for hopanoid biosynthesis, structural modifications and transport. Squalene-hopene cyclase (shc) can synthesize cyclic triterpenoids directly from squalene. Resulting hopanoid lipids are thought to provide membrane stability and to mediate stress resistance under low pH and high osmotic pressure (Belin et al., 2018) and, interestingly, many hopanoid-producing bacteria are capable of nitrogen fixation (Berry et al., 1993; Belin et al., 2018) or live in plant-associated environments (Ricci et al., 2014).
Finally, we identified a type I polyketide synthase (T1PKS) cluster on P2. It is part of a larger gene cluster associated with capsule polysaccharide production and export. The synthesis of many complex polyketide antibiotics or immunosuppressants in bacteria is catalyzed by such multimodular PKSs.
Genetic Factors Defining the Specific Niche of Strain Msb3
Macromolecular systems in the genome of Msb3 were predicted using the MacSyFinder tool (Abby et al., 2014) using the models from Abby et al. (2016) for the identification of protein secretion systems and closely related macromolecular systems in bacterial genomes. 15 loci encoding 11 different systems were identified in the genome of strain Msb3. Apart from a complete flagellum and two complete Tad pilus loci it harbors complete T1SS (3x), T2SS, T3SS, T5aSS, T5bSS (3x) and T5cSS (2x). Additionally, an incomplete T6SS was predicted, located on C2, but missing three necessary genes: tssA, tssI and evpJ. Upon closer inspection of the locus, however, a TssA homolog was identified carrying the TssA characteristic N-terminal ImpA domain (PFAM: PF06812) with an unusual C-terminal extension. We also identified two VgrG (=TssI) orthologs, encoded away from the main locus on C1. Furthermore, the functioning of the T6SS is not always dependent on EvpJ as demonstrated in Edwardsiella tarda by Zheng and Leung (2007). Therefore, the T6SS can be considered functional, remaining to be experimentally confirmed. Interestingly, the complete T6SS is among those elements shared between strain Msb3 and PsJN, but absent in LB400 (Supplementary Information and Supplementary Figure 4).
The expression of motility genes is under strict regulation and is mediated through sensing of environmental stimuli (Osterman et al., 2015). The Msb3 genome encodes 37 genes involved in chemotaxis (Che protein response regulators). This, together with quorum sensing mechanisms like luxR-like and N-acyl-homoserine lactone (AHL) based systems found in the genome could enable the strain to sense a set of environmental stimuli and to adapt to them. Motility genes, together with the presence of genes encoding for plant cell wall-degrading enzymes (cellulases and endoglucanases), could help to explain the systemic plant colonization by strain Msb3 in D. bulbifera.
Key adaptations for the colonization of eukaryotic hosts are mechanisms to cope with the consequences of host defense mechanisms. Reactive oxygen species (ROS) detoxification as well as xenobiotic degradation are common strategies of plant endophytes. The Msb3 genome shows a range of detoxification mechanisms including various enzymes necessary to cope with oxidative stress (catalases peroxidases), heavy metal and drug efflux systems and the degradation of organic substances (Supplementary Table 3). Additionally, multiple glutathion-S-transferases (GSTs) (17×) confer defense against both acute and chronic toxicities of electrophiles and reactive oxygen/nitrogen species, which includes processes such as the biodegradation of xenobiotics and antimicrobial drug resistance (Hayes et al., 2005; Allocati et al., 2009).
Genes Involved in Plant Growth Promotion
Activity of the enzyme ACC-deaminase (acdS) has been shown to significantly contribute to plant growth (Shah et al., 1998; Penrose and Glick, 2003) and represents the best way for plant growth promotion (PGP) besides IAA production (Olanrewaju et al., 2017). The presence of both IAA biosynthesis through indole-3-acetonitrile nitrilase, as well as ACC-deaminase (acdS) genes is a strong indication for the important role these genes play in the plant-associated lifestyle strategies of this strain.
Another mechanism by which plant associated bacteria can stimulate plant growth is by supplying nutrients, most notably, nitrogen. As mentioned above strain Msb3 carries a complete nitrogenase gene cluster (nifABZSHDKENXQ) on C2, theoretically enabling the strain to perform BNF. This may contribute directly or indirectly to plant growth and offers a powerful tool for mutualistic plant-microbe interactions. In Figure 5A we present a metabolic reconstruction of strain Msb3, based on its genome sequence, summarizing our findings.
Figure 5. Paraburkholderia sp. strain Msb3. (A) Metabolic reconstruction based on the genome sequence of strain Msb3. Depicted are processes discussed in the main text that are thought to be relevant in the occupation of plants as a specific niche. The cartoon representation includes core metabolisms that are insinuated through dashed boxes and circles. Dashed lines and arrows indicate connectivity of pathways or suggest transport of substances. Full arrows indicate translocation across membranes through transporters. Pathways, transporters, protein complexes and substances are labeled with abbreviations as follows: ACC, 1-aminocyclopropane-1-carboxylic acid; acdS, ACC-deaminase; α-KB, α-ketobutyrate; GS, glutamine synthetase; GOGAT, glutamine oxoglutarate aminotransferase; gltmn, glutamine; gltmt, glutamate; IAA, indole-3-acetic acid; ABC, ATP-binding cassette transporter; PPP, pentose phosphate pathway; G3P, glyceraldehyde 3-phosphate; F6P, fructose 6-phosphate; TCA, tricarboxylic acid cycle; TRAP, tripartite ATP-independent periplasmic transporters; LPS, lipopolysaccharide; T3SS, type III secretion system; T6SS, type VI secretion system; GSH, glutathione; -R, rest; GST, glutathione S-transferases; t1PKS, type I polyketide synthase; PK, polyketide; AAs, amino acids; NRPS, non-ribosomal peptide synthetase; NRP, non-ribosomal peptide; RND, resistance-nodulation-division family transporters; MFS, major facilitator superfamily; MDR, multi-drug resistance ABC transporter; DMT, drug/metabolite transporter superfamily. (B) Scanning electron micrograph of strain Msb3 in pure culture. (C) Growth curves of strain Msb3 at different temperatures in liquid TSB medium, growth rates decline with rising temperature and at 37°C growth is inhibited. OD600 per timepoint and temperature was measured with biological triplicates and every single measurement was performed in technical triplicates. Means of technical triplicates functioned as individual values, which were used to calculate averages and standard deviations (D) CLSM image overlay of a FISH experiment performed on a D. bulbifera leaf acumen, displaying a single secretory trichome on the surface of the acumen. Bacteria have been labeled with EUBmix-ATTO488 (green signal) and Burkholderia s.l. species with Burkho-Cy3 (yellow signal). Plant autofluorescence was visualized in magenta. Burkholderia s.l. species appear bright yellow in the overlay, whereas plant structures appear grayish magenta.
Physico-Chemical Characterization of Strain Msb3
We phenotypically examined strain Msb3 (Figure 5B) in respect to its temperature growth range, its resistance and susceptibility to various antibiotics as well as its preferred carbon sources. The strain grows up to a temperature of 35°C with optimal growth observed between 22°C and 28°C. Growth on rich medium is inhibited between 36°C and 37°C. A clear growth rate reduction was observed at temperatures between 30°C and 35°C (Figure 5C).
The preferred carbon sources of strain Msb3 are simple C4 sugars. The strain can grow in minimal medium that contains glucose as well as malate and citrate as sole carbon sources, respectively. At an equimolar concentration growth on malate is more efficient than growth on glucose.
Strain Msb3 is resistant to several commonly used antibiotics including ampicillin (50−100 μg/mL), cefalexin (10−40 μg/mL), and chloramphenicol (25 μg/mL). It is, however, sensitive to standard inhibitory concentrations of carbenicillin, streptomycin as well as kanamycin.
Strain Msb3 Promotes Plant Growth in Tomato
To experimentally validate our hypotheses concerning the PGP potential of strain Msb3 we monitored the growth of tomato (Solanum lycopersicum L., cv. Moneymaker) seedlings inoculated with the strain. Nine biological replicates of 14-day old seedlings grown from surface disinfected seeds were inoculated with bacteria by dipping into bacterial suspension (OD = 10, 0.5−5 × 109 CFUs) and were subsequently raised in sterilized soil under controlled conditions. Controls were treated with dead bacteria. 34 days post-inoculation (DPI) the plants were harvested and shoot length as well as root- and shoot-biomass were determined. We observed a highly significant effect: seedlings inoculated with live bacteria were significantly taller as well as heavier than their control counterparts (Figure 6). This effect was highly significant for all forms of biomass: Δ total biomass FW (P = 0.00074); Δ shoot biomass FW (P = 0.0073); Δ root biomass FW (P = 0.00067); Δ shoot biomass DW (P = 0.0003); Δ root biomass DW (P = 0.0008); Δ total biomass DW (P = 0.00008). Shoot length was also significantly influenced (P = 0.02253) by the treatment. Root biomass was influenced most heavily with an average increase of 44% (FW) and 87% (DW) compared to the control, followed by shoot biomass with an increase of 14.5% (FW) and 28% (DW), leading to a total difference of roughly 22% (FW) and 40% (DW). We subsequently tried to inoculate just the soil around the seedling and, despite the small number of biological replicates (three), retained a comparable and significant effect: 36% increase (P = 0.033) in root biomass. Re-cultivation of strain Msb3 from roots of inoculated tomato seedlings and plants grown in inoculated soil was successful, indicating that the strain successfully invaded the tomato rhizosphere to promote plant growth.
Figure 6. Box-plots of growth promotion assays in tomato using strain Msb3 as an inoculant. Individual tomato plants (n = 9) were inoculated with either live (green boxes) or heat killed (yellow boxes) cells of strain Msb3 and plant growth was compared after 34 DPI. Depicted here are comparisons between total biomass FW and DW as well as the respective contribution of shoot and root (in DW). Additionally, the shoot length was compared. Statistical significance was tested via two tailed Student’s t-tests.
Ecological and Phylogenetic Boundaries in Burkholderia s.l.
We realized there were discrepancies between views concerning generic as well as ecological boundaries in Burkholderia s.l. In order to derive useful information concerning the lifestyle of strain Msb3 in respect to dangers associated to its application we set out to review current hypotheses concerning the prevalence of opportunism and pathogenicity within different clades affiliated with Burkholderia s.l. We generated a robust phylogenetic tree (Figure 7) using 54 concatenated ribosomal proteins containing all strains within Burkholderia s.l. that were available for PubMLST in the BIGSdb (Jolley et al., 2018) and extracted the sequences from a set of selected other Burkholderiaceae. In an extensive literature review we retrieved information about all strains, including isolation source, details about the isolation as well as information about strains not represented in the tree, but with relevant isolation sources, differing from the represented strains’ source (Supplementary Table 4). We inferred whether a species, represented by all its strains, could be considered opportunistic/pathogenic or not. Our analysis shows that the proposed ecological boundaries within Burkholderia s.l. are not supported: the plant-beneficial and environmental (PBE) Burkholderia species cluster is now comprised of five distinct genera: Paraburkholderia s.s.; Caballeronia; Robbsia; Trinickia and Mycetohabitans. Every single one of these genera harbors at least one species that can act as an opportunistic pathogen to either plants or humans (Figure 7) and in total we have identified at least six species within the group with connections to disease and clinical environments. Paraburkholderia s.s. forms two large clusters in our reconstruction, henceforth referred to as Clade I and Clade II Paraburkholderia s.s. Strain Msb3 branches within Clade I Paraburkholderia s.s., which contains the opportunistic human colonizer P. fungorum.
Figure 7. Ecological data concerning Burkholderia sensu lato species within a robust phylogenetic framework. A phylogenetic tree for the genus Burkholderia sensu lato based on the concatenated alignment of 54 ribosomal proteins. Species and strain names represent those used in the Bacterial Isolate Genome Sequence Database (BIGSdb), except for strain Msb3, which is marked in pink and carries the species name proposed in this study. The most recent genus names validly published for specific groups, distinguished through gray and white shading, are shown outside of the first circle. The first circle indicates whether one or more pathogenic strains (plant or animal) were found within a bacterial species. If there was evidence, all strains carrying the same species name were marked yellow. The second circle shows the primary isolation source of every strain included in the analysis, using a color code explained in the legend. Annotations on the tree include small circles on branch tips, showing additional details about the primary isolation source or the isolation source of strains from the same species not included in the analysis. Octagons on nodes display values for ultrafast (UF) bootstrap and approximate likelihood ratio test (aLRT) calculations with the non-parametric SH correction (SH-aLRT) in the spirit of the Shimodaira–Hasegawa (SH) algorithm. Branch length is given as amino-acid substitutions per site. Ralstonia picketti strain 12J was used as an outgroup to set the root of the tree.
As the plant phyllosphere is an underrepresented target of microbiological studies we set out to discover novel forms of associations between Burkholderia s.l. species and their plant hosts in this habitat. Inspired by the occurrence of the “leaf nodule symbiosis” in Dioscorea sansibarensis (Carlier et al., 2017; Pinto-Carbo et al., 2018; De Meyer et al., 2019) we investigated the prevalence of Burkholderia s.l. species in the plant family Dioscoreaceae. Indeed, we detected and isolated the novel Paraburkholderia strain Msb3 from leaf acumens of Dioscorea bulbifera. In our efforts to describe the strain, its ecology and its potential, we conducted several targeted experiments to gain insights into (a) its role on its host plant D. bulbifera, (b) its genetic and metabolic repertoire, (c) its potential for agricultural application in promoting plant growth and (d) its phylogenetic position and the potential of it and its close relatives for pathogenicity.
Paraburkholderia spp. generally display an array of desirable properties that could be exploited for uses in agriculture that are matched by few other groups of bacteria. To illustrate: P. xenovorans strain LB400 can fix nitrogen and has the ability to degrade polychlorinated biphenyl (PCB) and could be used for bioremediation of contaminated soils. P. phytofirmans strain PsJN is an endophytic plant growth promoting organism with an extraordinary host range (Frommel et al., 1991; Sessitsch et al., 2005; Da et al., 2012; Mitter et al., 2013) and could be used for large scale production of biofertilizers. Some Paraburkholderia spp. have the ability to nodulate legumes and symbiotically fix nitrogen, unusual among Betaproteobacteria, therefore called “β-rhizobia” (Moulin et al., 2001; Chen et al., 2003). The tendency of Paraburkholderia to engage in facultative symbiotic relationships with plants is unequivocal and, unlike leaf nodulating Caballeronia species, the degree of loose-intimacy allows us to culture and study them and to potentially transfer these traits to non-original host plants. To our best knowledge, this is the first report of a Paraburkholderia strain flourishing in the phyllosphere of its host plant and it is also the first implication of a strain of the genus in a facultative symbiotic relationship with a yam family plant. It should be noted that here the broad definition of symbiosis is used, as the outcome of the interaction for both parties is not fully elucidated. This definition includes mutualistic, as well as commensal and parasitic associations and generally refers to any type of a close, prolonged interaction between two different organisms.
We consistently detected the strains molecular signature in plant DNA extracts of D. bulbifera over a period of 3 years, representing three complete growth cycles of the perennial vine. We also retrieved high numbers of cells from crude leaf acumen extracts in two independent cultivation trials, a year apart, from the same plant individual and detected the strains 16S rDNA in several individuals that had been reproduced clonally through underground tubers. We hypothesized about the role of strain Msb3 among the leaf microbiota on D. bulbifera and about the actual abundance and position on the plant. Using the described amplicon sequencing approach, we were able to show that strain Msb3 indeed localizes at leaf acumens. Since surface sterilization of the acumen lead to a significant reduction of bacterial reads, heavily influencing the relative abundance of strain Msb3, the organism does not seem to reside inside the plant but rather dwells on the acumen surface instead. Indeed, microscopic analysis showed that bacteria are associated to trichomes on the acumen (Figures 2, 3, 5D). Further visual exploration of secretory trichomes on the leaf acumen via FISH using a genus specific probe lead to the identification of clusters of bacteria affiliated with Burkholderia s.l., colonizing the sides of trichomes (Figure 3), further supporting our hypothesis. We generally found few other bacteria. This may be an artifact due to weak signal intensity compared to the plant background and fast bleaching of Atto488, yet, these findings were supported by other experiments using a general DNA stain instead of the EUBmix (Supplementary Figure 3). Together with the community profiling data these results provide strong evidence that strain Msb3 plays a key role in its niche, as it clearly dominates this bacterial community.
The observed association could offer an intriguing perspective on the evolution of the “leaf nodule symbiosis” in Dioscoreaceae. D. sansibarensis is considered the only species of the monocot family, in which nodule formation occurs (Carlier et al., 2017; Pinto-Carbo et al., 2018; De Meyer et al., 2019), however, the genomic similarity between our strain and O. dioscoreae (Carlier et al., 2017), their position and abundance on the leaf and the role of secretory trichomes (Miller and Reporter, 1987; Pinto-Carbo et al., 2018) as well as the close phylogenetic relationship of both hosts (Viruel et al., 2018) and microbes (Carlier et al., 2017) are indicative for conserved structures mediating these associations. Both symbionts are bona fide epiphytes for at least part of their life (Carlier et al., 2017) and form clusters on secretory trichomes on the leaf acumen (Miller and Reporter, 1987) of their true yam host plant. In light of the absence of nodules in D. bulbifera our findings could be interpreted as an early stage in the development of such a structure. As we have not actually elucidated the mechanics of the interaction, or the transmission of the symbiont, we refrain from defining it as the discovery of a novel form of the leaf symbiosis. Nevertheless, we believe there are striking parallels between this association and the leaf symbiosis in D. sansibarensis. The herein described genomic properties resemble many of those found and upregulated in planta in O. dioscoreae (De Meyer et al., 2019): a complete T6SS, a NRPS, polyketide synthesis, prominent organic acid and TCA intermediate metabolism, ammonia assimilation and a functional GS/GOGAT pathway, ROS detoxification mechanisms and an ACC deaminase.
Strain Msb3 thereby displays most properties associated with plant associated and endophytic lifestyles and offers some intriguing strategies for PGP and interaction with various hosts. The gene repertoire associated with host colonization, in particular the abundance of macromolecular systems, is indicative of a large host range, comparable to that of PsJN. Indeed, the T6SS is absent in most close relatives of strain Msb3, but conserved in both this strain and PsJN, underlining its potential importance in successful plant colonization. PGP mechanisms include plant hormone regulation strategies, i.e., ACC deamination and IAA synthesis. Growth promotion through PsJN is thought to be mediated this way (Sessitsch et al., 2005) and the genes are absent in soil dwelling LB400. The combination of these genes with a nitrogenase gene cluster is remarkable. Although nitrogenase enzymes are extremely sensitive to oxygen (Gallon, 1992) in vitro diazotrophy has been shown in many plant-associated, non-legume-nodulating Paraburkholderia species, including P. unamae, P. tropica, P. silvatlantica, P. xenovorans, P. vietnamiensis and P. kururiensis (Martinez-Aguilar et al., 2008; Suarez-Moreno et al., 2012). The rare consolidation of these features, BNF and plant hormone regulation, constitutes a powerful tool for the production of potent biofertilizers.
The exact role of strain Msb3 in the association to D. bulbifera remains unclear. Secondary metabolism may well play an important role. It does in the association of O. dioscoreae to D. sansibarensis (De Meyer et al., 2019) and similarly, strain Msb3 carries gene clusters for the production of a non-ribosomal peptide and a polyketide hitherto unknown. So far, we were not able to produce axenic D. bulbifera plants, stalling our efforts to further investigate it and low bacterial biomass compared to plant biomass exacerbates applications such as analysis of the leaf meta-transcriptome. We do know, however, that strain Msb3 strongly promotes plant growth in another plant, i.e., tomato. We tested its potential for PGP under semi-sterile conditions and observed a strong and highly significant effect on plant biomass upon inoculation of seedlings or soil. Here, growth promotion is most likely mediated through colonization of the tomato rhizosphere. The fact that strain Msb3 confers PGP to hosts beside D. bulbifera suggests a large host range and shows its ability to quickly adapt to various ecological niches. These traits make it an ideal candidate for investigation in respect to agricultural applications. This is underlined by the fact that it lacks the ability to survive at temperatures higher than 36°C, making colonization of mammalian hosts unlikely.
Nevertheless, the application of PGPB and bioagents in the environment is connected to several risks that need to be understood and eliminated before administration. The possibility of releasing pathogens (to humans but also other vertebrates and plants) into the environment and possibly into the food chain must be averted at all cost. Paraburkholderia are often viewed as unproblematic and even beneficial, as their phylogenetic difference from pathogenic and opportunistic Burkholderia s.s. is undisputed and its isolates almost exclusively come from environmental samples, usually from soil and plants (Suarez-Moreno et al., 2012; Angus et al., 2014; Sawana et al., 2014; Estrada-de los Santos et al., 2015). However, this is subject to a controversial debate within the community (Estrada-de los Santos et al., 2015; Eberl and Vandamme, 2016; Vandamme et al., 2017; Dobritsa and Samadpour, 2019). To clear out misconceptions and to tackle safety concerns we reevaluated phylogenetic relationships within Burkholderia s.l. in a refined phylogeny using data from almost 280 different isolates and mapped ecological data points, retrieved from extensive literature review, onto our robust phylogenetic framework. Our strain level analysis clearly shows that the ecological characterization along phylogenetic boundaries within Burkholderia s.l. is by no means an accurate way to classify environmental strains as unproblematic. The five genera originating from the PBE Burkholderia species cluster contain opportunists: (1) Caballeronia (Dobritsa and Samadpour, 2016) contains two species that are potentially opportunistic human colonizers: Caballeronia turbans and Caballeronia concitans were both isolated from human clinical samples, i.e., blood, pleural fluid and lung tissue (Peeters et al., 2016). (2) Robbsia (Lopes-Santos et al., 2017; Oren and Garrity, 2017) is represented by a single species, Robbsia andropogonis, which was isolated from stripe disease in sorghum (Smith, 1911) and causes leaf spots, streaks, or stripes in a wide host range. The plant pathogen is, however, no longer considered part of the Burkholderia s.l. species complex (Lopes-Santos et al., 2017) and has therefore not been included in our tree. (3) Trinickia (Estrada-de Los Santos et al., 2018; Oren and Garrity, 2018) contains the known phytopathogen T. caryophylli, which is the causative agent of bacterial wilt and root rot of carnations (Burkholder, 1942). (4) Mycetohabitans is comprised of two species, M. endofungorum and M. rhizoxinica (Partida-Martinez et al., 2007). While Estrada-de Los Santos et al. (2018) claim that these species are not likely to be pathogenic a study by Gee et al. (2011) shows that strains of both species could be isolated from clinical samples, including human blood and wounds. Although strong statements about their actual pathogenicity are inappropriate, due to a lack of information about the clinical background of these isolates, these species should be carefully investigated and opportunistic behavior should be assumed. (5) A similar case can be observed in the emended genus Paraburkholderia (here s.s.). Some isolates of P. fungorum originated from human or mice clinical samples (Coenye et al., 2001), including cystic fibrosis patients (Coenye et al., 2002) and a case of bacteremia with P. fungorum with clinical features of septic arthritis has been observed (Gerrits et al., 2005). Additionally, P. tropica, a well-studied free-living nitrogen fixing plant-associated bacterium (Reis et al., 2004), has been found to colonize immunocompromised patients. The patient developed septicemia due to P. tropica infection of the blood (Deris et al., 2010). 16S rRNA analysis of the blood culture gave a 100% identity match to that of P. tropica, unambiguously demonstrating that at least one strain of this species can be considered an opportunist in immunocompromised patients.
It ought to be mentioned that most of the cases described above have been limited to very few occurrences, usually only in immunocompromised patients, suggesting that the risks they pose to healthy individuals is rather small. Nevertheless, classification of any novel isolate as unproblematic should be conducted with great care. We therefore emphasize that such classification of any species or strain within the genera investigated here, including that of Msb3, must be made on a case-by-case basis, only after careful molecular and phenotypic characterization. The need for a consensus within the community, outlining the procedures for their characterization (e.g., growth at 37°C, suitable multispecies infection scenarios, mammalian hosts, etc.) is certainly necessary.
Finally, we believe that detailed analysis of whole genomes, on a strain level rather than species level, using explicit ecological data (e.g., host range, isolation source) may help to elucidate genomic adaptations to opportunism and pathogenicity in plants or animals previously gone unnoticed. Providing genomic as well as ecological data with every description of novel strains may facilitate this process. Paraburkholderia sp. strain Msb3 certainly presents a promising model to study the genetic prerequisites for the development of facultative symbiotic interactions within Burkholderia s.l. as well as a resourceful candidate to investigate and generate biofertilizers with a broad host range.
Data Availability Statement
Genome data from Paraburkholderia sp. strain Msb3 has been submitted to ENA in BioProject PRJEB33427. The whole genome sequence is available under accession numbers LR699553-LR699557. The nucleotide sequence data obtained through 16S rRNA amplicon sequencing have been submitted to the Sequence Read Archive of NCBI under BioProject number PRJNA562285.
WW and JH conceived and designed the research. JH and FS performed the bacteria isolation and the growth promotion experiments. JH performed the molecular biology experiments, genome annotation, analysis of amplicon sequencing data, and phylogenetic analyses, and wrote the manuscript with contribution from WW. SK, SG, BF, and MS performed the amplicon sequencing experiments and data preparation. JH and MB provided the microbiological and pysico-chemical data. JH, BD, and AB provided the microscopy images and performed fluorescence in situ hybridization experiments. JH, FS, and LF identified and collected the samples. JH, MK, and WW analyzed and interpreted the results. All authors discussed and revised the manuscript.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
We thank Prof. Dr. Christa Schleper for her constructive criticism regarding the presented data and for reading and correcting the manuscript. Also, thankfully acknowledged is the hard work of our gardeners, Andreas Schröfl and Thomas Joch. The LABGeM (CEA/Genoscope & CNRS UMR8030), the France Génomique and French Bioinformatics Institute national infrastructures (funded as part of Investissement d’Avenir program managed by the Agence Nationale pour la Recherche, contracts ANR-10-INBS-09 and ANR-11-INBS-0013) are acknowledged for support within the MicroScope annotation platform. The Vienna Biocenter Core Facility (VBCF) and the Cell Imaging & Ultrastructure Research (CIUS) core facility (University of Vienna) are acknowledged for providing essential services for the generation of the presented data.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2020.00581/full#supplementary-material
- ^ http://www.genoscope.cns.fr/agc/microscope/home/index.php
- ^ http://jspecies.ribohost.com/jspeciesws/#home
- ^ https://gtdb.ecogenomic.org/
Abby, S. S., Neron, B., Menager, H., Touchon, M., and Rocha, E. P. (2014). MacSyFinder: a program to mine genomes for molecular systems with an application to CRISPR-Cas systems. PLoS One 9:e110726. doi: 10.1371/journal.pone.0110726
Amann, R. I., Krumholz, L., and Stahl, D. A. (1990). Fluorescent-oligonucleotide probing of whole cells for determinative, phylogenetic, and environmental studies in microbiology. J. Bacteriol. 172, 762–770. doi: 10.1128/jb.172.2.762-770.1990
Angus, A. A., Agapakis, C. M., Fong, S., Yerrapragada, S., Estrada-de los Santos, P., Yang, P., et al. (2014). Plant-associated symbiotic Burkholderia species lack hallmark strategies required in mammalian pathogenesis. PLoS One 9:e83779. doi: 10.1371/journal.pone.0083779
Belin, B. J., Busset, N., Giraud, E., Molinaro, A., Silipo, A., and Newman, D. K. (2018). Hopanoid lipids: from membranes to plant–bacteria interactions. Nat. Rev. Microbiol. 16:304. doi: 10.1038/nrmicro.2017.173
Berry, A. M., Harriott, O. T., Moreau, R. A., Osman, S. F., Benson, D. R., and Jones, A. D. (1993). Hopanoid lipids compose the Frankia vesicle envelope, presumptive barrier of oxygen diffusion to nitrogenase. Pro. Natl. Acad. Sci. U.S.A. 90, 6091–6094. doi: 10.1073/pnas.90.13.6091
Burkholder, W. H. (1942). Three bacterial plant pathogens: Phytomonas earyophylli sp.n., Phytomonas alliicola sp.n., and Phytomonas manihotis (Arthaud-Berthet et Sondar). Viégas. Phytopathol. 32, 141–149.
Callahan, B. J., McMurdie, P. J., and Holmes, S. P. (2017). Exact sequence variants should replace operational taxonomic units in marker-gene data analysis. ISME J. 11:2639. doi: 10.1038/ismej.2017.119
Callahan, B. J., McMurdie, P. J., Rosen, M. J., Han, A. W., Johnson, A. J. A., and Holmes, S. P. (2016). DADA2: high-resolution sample inference from Illumina amplicon data. Nat. Methods 13, 581–583. doi: 10.1038/nmeth.3869
Caporaso, J. G., Kuczynski, J., Stombaugh, J., Bittinger, K., Bushman, F. D., Costello, E. K., et al. (2010). QIIME allows analysis of high-throughput community sequencing data. Nat. Methods 7, 335–336. doi: 10.1038/nmeth.f.303
Carlier, A., Cnockaert, M., Fehr, L., Vandamme, P., and Eberl, L. (2017). Draft genome and description of Orrella dioscoreae gen. nov. sp. nov., a new species of Alcaligenaceae isolated from leaf acumens of Dioscorea sansibarensis. Syst. Appl. Microbiol. 40, 11–21. doi: 10.1016/j.syapm.2016.10.002
Carlier, A., Fehr, L., Pinto-Carbo, M., Schaberle, T., Reher, R., Dessein, S., et al. (2016). The genome analysis of Candidatus Burkholderia crenata reveals that secondary metabolism may be a key function of the Ardisia crenata leaf nodule symbiosis. Environ. Microbiol. 18, 2507–2522. doi: 10.1111/1462-2920.13184
Carlier, A. L., and Eberl, L. (2012). The eroded genome of a Psychotria leaf symbiont: hypotheses about lifestyle and interactions with its plant host. Environ. Microbiol. 14, 2757–2769. doi: 10.1111/j.1462-2920.2012.02763.x
Chain, P. S., Denef, V. J., Konstantinidis, K. T., Vergez, L. M., Agullo, L., Reyes, V. L., et al. (2006). Burkholderia xenovorans LB400 harbors a multi-replicon, 9.73-Mbp genome shaped for versatility. Proc. Natl Acad. Sci. U.S.A. 103, 15280–15287. doi: 10.1073/pnas.0606924103
Chen, W. M., Moulin, L., Bontemps, C., Vandamme, P., Bena, G., and Boivin-Masson, C. (2003). Legume symbiotic nitrogen fixation by β-Proteobacteria is widespread in nature. J. Bacteriol. 185, 7266–7272. doi: 10.1128/jb.185.24.7266-7272.2003
Chin, C.-S., Alexander, D. H., Marks, P., Klammer, A. A., Drake, J., Heiner, C., et al. (2013). Nonhybrid, finished microbial genome assemblies from long-read SMRT sequencing data. Nat. Methods 10:563. doi: 10.1038/nmeth.2474
Coenye, T., Goris, J., Spilker, T., Vandamme, P., and LiPuma, J. J. (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
Coenye, T., Laevens, S., Willems, A., Ohlen, M., Hannant, W., Govan, J. R., et al. (2001). Burkholderia fungorum sp. nov. and Burkholderia caledonica sp. nov., two new species isolated from the environment, animals and human clinical samples. Int. J. Syst. Evol. Microbiol. 51(Pt 3), 1099–1107. doi: 10.1099/00207713-51-3-1099
Compant, S., Nowak, J., Coenye, T., Clement, C., and Ait Barka, E. (2008). Diversity and occurrence of Burkholderia spp. in the natural environment. FEMS Microbiol. Rev. 32, 607–626. doi: 10.1111/j.1574-6976.2008.00113.x
Criscuolo, A., and Gribaldo, S. (2010). BMGE (Block Mapping and Gathering with Entropy): a new software for selection of phylogenetic informative regions from multiple sequence alignments. BMC Evo. Biol. 10:210. doi: 10.1186/1471-2148-10-210
Da, K., Nowak, J., and Flinn, B. (2012). Potato cytosine methylation and gene expression changes induced by a beneficial bacterial endophyte, Burkholderia phytofirmans strain PsJN. Plant Physiol. Biochem. 50, 24–34. doi: 10.1016/j.plaphy.2011.09.013
Daims, H., Brühl, A., Amann, R., Schleifer, K.-H., and Wagner, M. (1999). The domain-specific probe EUB338 is insufficient for the detection of all bacteria: development and evaluation of a more comprehensive probe set. Syst. Appl. Microbiol. 22, 434–444. doi: 10.1016/S0723-2020(99)80053-8
De Meyer, F., Danneels, B., Acar, T., Rasolomampianina, R., Rajaonah, M. T., Jeannoda, V., et al. (2019). Adaptations and evolution of a heritable leaf nodule symbiosis between Dioscorea sansibarensis and Orrella dioscoreae. ISME J. 13, 1831–1844. doi: 10.1038/s41396-019-0398-8
Deris, Z. Z., Van Rostenberghe, H., Habsah, H., Noraida, R., Tan, G. C., Chan, Y. Y., et al. (2010). First isolation of Burkholderia tropica from a neonatal patient successfully treated with imipenem. Int. J. Infect. Dis. 14, e73–e74. doi: 10.1016/j.ijid.2009.03.005
Dobritsa, A. P., and Samadpour, M. (2016). Transfer of eleven species of the genus Burkholderia to the genus Paraburkholderia and proposal of Caballeronia gen. nov. to accommodate twelve species of the genera Burkholderia and Paraburkholderia. Int. J. Syst. Evol. Microbiol. 66, 2836–2846. doi: 10.1099/ijsem.0.001065
Dobritsa, A. P., and Samadpour, M. (2019). Reclassification of Burkholderia insecticola as Caballeronia insecticola comb. nov. and reliability of conserved signature indels as molecular synapomorphies. Int. J. Syst. Evol. Microbiol. 69, 2057–2063. doi: 10.1099/ijsem.0.003431
Dorn-In, S., Bassitta, R., Schwaiger, K., Bauer, J., and Holzel, C. S. (2015). Specific amplification of bacterial DNA by optimized so-called universal bacterial primers in samples rich of plant DNA. J. Microbiol. Methods 113, 50–56. doi: 10.1016/j.mimet.2015.04.001
Estrada-De Los Santos, P., Bustillos-Cristales, R., and Caballero-Mellado, J. (2001). Burkholderia, a genus rich in plant-associated nitrogen fixers with wide environmental and geographic distribution. Appl. Environ. Microbiol. 67, 2790–2798. doi: 10.1128/AEM.67.6.2790-2798.2001
Estrada-de Los Santos, P., Palmer, M., Chavez-Ramirez, B., Beukes, C., Steenkamp, E. T., Briscoe, L., et al. (2018). Whole genome analyses suggests that burkholderia sensu lato contains two additional novel genera (Mycetohabitans gen. nov., and Trinickia gen. nov.): implications for the evolution of diazotrophy and nodulation in the burkholderiaceae. Genes 9:E389. doi: 10.3390/genes9080389
Estrada-de los Santos, P., Rojas-Rojas, F. U., Tapia-García, E. Y., Vásquez-Murrieta, M. S., and Hirsch, A. M. (2015). To split or not to split: an opinion on dividing the genus Burkholderia. Ann. Microbiol. 66, 1303–1314. doi: 10.1007/s13213-015-1183-1
Frank, J. A., Reich, C. I., Sharma, S., Weisbaum, J. S., Wilson, B. A., and Olsen, G. J. (2008). Critical evaluation of two primers commonly used for amplification of bacterial 16S rRNA genes. Appl. Environ. Microbiol. 74, 2461–2470. doi: 10.1128/aem.02272-07
Frommel, M. I., Nowak, J., and Lazarovits, G. (1991). Growth enhancement and developmental modifications of in Vitro grown potato (Solanum tuberosum spp. tuberosum) as affected by a nonfluorescent pseudomonas sp. Plant Physiol. 96, 928–936. doi: 10.1104/pp.96.3.928
Gee, J. E., Glass, M. B., Lackner, G., Helsel, L. O., Daneshvar, M., Hollis, D. G., et al. (2011). Characterization of Burkholderia rhizoxinica and B. endofungorum isolated from clinical specimens. PLoS One 6:e15731. doi: 10.1371/journal.pone.0015731
Guindon, S., Dufayard, J.-F., Lefort, V., Anisimova, M., Hordijk, W., and Gascuel, O. (2010). New algorithms and methods to estimate maximum-likelihood phylogenies: assessing the performance of PhyML 3.0. Syst. Biol. 59, 307–321. doi: 10.1093/sysbio/syq010
Hogardt, M., Trebesius, K., Geiger, A. M., Hornef, M., Rosenecker, J., and Heesemann, J. (2000). Specific and rapid detection by fluorescent in situ hybridization of bacteria in clinical samples obtained from cystic fibrosis patients. J. Clin. Microbiol. 38, 818–825. doi: 10.1128/jcm.38.2.818-825.2000
Hunt, M., Silva, N. D., Otto, T. D., Parkhill, J., Keane, J. A., and Harris, S. R. (2015). Circlator: automated circularization of genome assemblies using long sequencing reads. Genome Biol. 16:294. doi: 10.1186/s13059-015-0849-0
Jolley, K. A., Bray, J. E., and Maiden, M. C. J. (2018). Open-access bacterial population genomics: BIGSdb software, the PubMLST.org website and their applications. Wellcome Open Res. 3:124. doi: 10.12688/wellcomeopenres.14826.1
Kasajima, I., Sasaki, K., Tanaka, Y., Terakawa, T., and Ohtsubo, N. (2013). Large-scale extraction of pure DNA from mature leaves of Cyclamen persicum Mill. and other recalcitrant plants with alkaline polyvinylpolypyrrolidone (PVPP). Sci. Horticult. 164, 65–72. doi: 10.1016/j.scienta.2013.09.011
Katoh, K., Misawa, K., Kuma, K. I., and Miyata, T. (2002). MAFFT: a novel method for rapid multiple sequence alignment based on fast Fourier transform. Nucleic Acids Res. 30, 3059–3066. doi: 10.1093/nar/gkf436
Kim, M., Oh, H. S., Park, S. C., and Chun, J. (2014). Towards a taxonomic coherence between average nucleotide identity and 16S rRNA gene sequence similarity for species demarcation of prokaryotes. Int. J. Syst. Evol. Microbiol. 64(Pt 2), 346–351. doi: 10.1099/ijs.0.059774-0
Kristensen, D. M., Kannan, L., Coleman, M. K., Wolf, Y. I., Sorokin, A., Koonin, E. V., et al. (2010). A low-polynomial algorithm for assembling clusters of orthologous groups from intergenomic symmetric best matches. Bioinformatics 26, 1481–1487. doi: 10.1093/bioinformatics/btq229
Lee, C. J., Lee, J. T., Kwor, J., Kim, B., and Park, W. (2005). Occurrence of bacterial soft rot of onion plants caused by Burkholderia gladioli pv. alliicola in Korea. Australasian Plant Pathol. 34, 287–292.
Lemaire, B., Janssens, S., Smets, E., and Dessein, S. (2012a). Endosymbiont transmission mode in bacterial leaf nodulation as revealed by a population genetic study of Psychotria leptophylla. Appl. Environ. Microbiol. 78, 284–287. doi: 10.1128/AEM.06130-11
Lemaire, B., Lachenaud, O., Persson, C., Smets, E., and Dessein, S. (2012b). Screening for leaf-associated endophytes in the genus Psychotria (Rubiaceae). FEMS Microbiol. Ecol. 81, 364–372. doi: 10.1111/j.1574-6941.2012.01356.x
Lemaire, B., Vandamme, P., Merckx, V., Smets, E., and Dessein, S. (2011). Bacterial leaf symbiosis in angiosperms: host specificity without co-speciation. PLoS One 6:e24430. doi: 10.1371/journal.pone.0024430
Lopes-Santos, L., Castro, D. B. A., Ferreira-Tonin, M., Corrêa, D. B. A., Weir, B. S., Park, D., et al. (2017). Reassessment of the taxonomic position of Burkholderia andropogonis and description of Robbsia andropogonis gen. nov., comb. nov. Antonie van Leeuwenhoek 110, 727–736. doi: 10.1007/s10482-017-0842-6
Martinez-Aguilar, L., Diaz, R., Pena-Cabriales, J. J., Estrada-de Los Santos, P., Dunn, M. F., and Caballero-Mellado, J. (2008). Multichromosomal genome structure and confirmation of diazotrophy in novel plant-associated Burkholderia species. Appl. Environ. Microbiol. 74, 4574–4579. doi: 10.1128/AEM.00201-08
Miller, I. M., and Reporter, M. (1987). Bacterial leaf symbiosis in Dioscorea sansibarensis: morphology and ultrastructure of the acuminate leaf glands∗. Plant Cell Environ. 10, 413–424. doi: 10.1111/1365-3040.ep11603654
Mitter, B., Petric, A., Shin, M. W., Chain, P. S., Hauberg-Lotte, L., Reinhold-Hurek, B., 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. 4:120. doi: 10.3389/fpls.2013.00120
Oren, A., and Garrity, G. M. (2017). List of new names and new combinations previously effectively, but not validly, published. Int. J. Syst. Evol. Microbiol. 67, 3140–3143. doi: 10.1099/ijsem.0.002278
Oren, A., and Garrity, G. M. (2018). List of new names and new combinations previously effectively, but not validly, published. Int. J. Syst. Evol. Microbiol. 68, 3379–3393. doi: 10.1099/ijsem.0.003071
Osterman, I. A., Dikhtyar, Y. Y., Bogdanov, A. A., Dontsova, O. A., and Sergiev, P. V. (2015). Regulation of flagellar gene expression in Bacteria. Biochemistry 80, 1447–1456. doi: 10.1134/s000629791511005x
Parks, D. H., Chuvochina, M., Waite, D. W., Rinke, C., Skarshewski, A., Chaumeil, P.-A., et al. (2018). A standardized bacterial taxonomy based on genome phylogeny substantially revises the tree of life. Nat. Biotechnol. 36, 996. doi: 10.1038/nbt.4229
Partida-Martinez, L. P., Groth, I., Schmitt, I., Richter, W., Roth, M., and Hertweck, C. (2007). Burkholderia rhizoxinica sp. nov. and Burkholderia endofungorum sp. nov., bacterial endosymbionts of the plant-pathogenic fungus Rhizopus microsporus. Int. J. Syst. Evol. Microbiol. 57(Pt 11), 2583–2590. doi: 10.1099/ijs.0.64660-0
Peeters, C., Meier-Kolthoff, J. P., Verheyde, B., De Brandt, E., Cooper, V. S., and Vandamme, P. (2016). Phylogenomic Study of Burkholderia glathei-like organisms, proposal of 13 Novel Burkholderia Species and emended descriptions of Burkholderia sordidicola, Burkholderia zhejiangensis, and Burkholderia grimmiae. Front. Microbiol. 7:877. doi: 10.3389/fmicb.2016.00877
Penrose, D. M., and Glick, B. R. (2003). Methods for isolating and characterizing ACC deaminase-containing plant growth-promoting rhizobacteria. Physiol. Plant. 118, 10–15. doi: 10.1034/j.1399-3054.2003.00086.x
Philippot, L., Raaijmakers, J. M., Lemanceau, P., and van der Putten, W. H. (2013). Going back to the roots: the microbial ecology of the rhizosphere. Nat. Rev. Microbiol. 11, 789–799. doi: 10.1038/nrmicro3109
Pinto-Carbo, M., Gademann, K., Eberl, L., and Carlier, A. (2018). Leaf nodule symbiosis: function and transmission of obligate bacterial endophytes. Curr. Opin. Plant Biol. 44, 23–31. doi: 10.1016/j.pbi.2018.01.001
Pinto-Carbo, M., Sieber, S., Dessein, S., Wicker, T., Verstraete, B., Gademann, K., et al. (2016). Evidence of horizontal gene transfer between obligate leaf nodule symbionts. ISME J. 10, 2092–2105. doi: 10.1038/ismej.2016.27
R Core Team (2019). R: A Language and Environment for Statistical Computing. Vienna: R Foundation for Statistical Computing. Available online at: https://www.R-project.org/
Reis, V. M., Estrada-de los Santos, P., Tenorio-Salgado, S., Vogel, J., Stoffels, M., Guyon, S., et al. (2004). Burkholderia tropica sp. nov., a novel nitrogen-fixing, plant-associated bacterium. Int. J. Syst. Evol. Microbiol. 54(Pt 6), 2155–2162. doi: 10.1099/ijs.0.02879-0
Ricci, J. N., Coleman, M. L., Welander, P. V., Sessions, A. L., Summons, R. E., Spear, J. R., et al. (2014). Diverse capacity for 2-methylhopanoid production correlates with a specific ecological niche. Isme J. 8, 675–684. doi: 10.1038/ismej.2013.191
Richter, M., Rossello-Mora, R., Oliver Glockner, F., and Peplies, J. (2016). JSpeciesWS: a web server for prokaryotic species circumscription based on pairwise genome comparison. Bioinformatics 32, 929–931. doi: 10.1093/bioinformatics/btv681
Sawana, A., Adeolu, M., and Gupta, R. S. (2014). Molecular signatures and phylogenomic analysis of the genus Burkholderia: proposal for division of this genus into the emended genus Burkholderia containing pathogenic organisms and a new genus Paraburkholderia gen. nov. harboring environmental species. Front. Genet. 5:429. doi: 10.3389/fgene.2014.00429
Sessitsch, A., Coenye, T., Sturz, A. V., Vandamme, P., Barka, E. A., Salles, J. F., et al. (2005). Burkholderia phytofirmans sp. nov., a novel plant-associated bacterium with plant-beneficial properties. Int. J Syst. Evol. Microbiol. 55(Pt 3), 1187–1192. doi: 10.1099/ijs.0.63149-0
Shah, S., Li, J., Moffatt, B. A., and Glick, B. R. (1998). Isolation and characterization of ACC deaminase genes from two different plant growth-promoting rhizobacteria. Can. J. Microbiol. 44, 833–843. doi: 10.1139/w98-074
Sieber, S., Carlier, A., Neuburger, M., Grabenweger, G., Eberl, L., and Gademann, K. (2015). Isolation and total synthesis of kirkamide, an aminocyclitol from an obligate leaf nodule symbiont. Angew Chem. Int. Ed. Eng.l 54, 7968–7970. doi: 10.1002/anie.201502696
Spilker, T., Baldwin, A., Bumford, A., Dowson, C. G., Mahenthiralingam, E., and LiPuma, J. J. (2009). Expanded multilocus sequence typing for Burkholderia species. J. Clin. Microbiol. 47, 2607–2610. doi: 10.1128/JCM.00770-09
Suarez-Moreno, Z. R., Caballero-Mellado, J., Coutinho, B. G., Mendonca-Previato, L., James, E. K., and Venturi, V. (2012). Common features of environmental and potentially beneficial plant-associated Burkholderia. Microb. Ecol. 63, 249–266. doi: 10.1007/s00248-011-9929-1
Vallenet, D., Labarre, L., Rouy, Z., Barbe, V., Bocs, S., Cruveiller, S., et al. (2006). MaGe: a microbial genome annotation system supported by synteny results. Nucleic Acids Res. 34, 53–65. doi: 10.1093/nar/gkj406
Van Oevelen, S. (2002). Identification of the bacterial endosymbionts in leaf galls of Psychotria (Rubiaceae, angiosperms) and proposal of ‘Candidatus Burkholderia kirkii’ sp. nov. Int. J. Syst. Evol. Microbiol. 52, 2023–2027. doi: 10.1099/ijs.0.02103-0
Vandamme, P., Peeters, C., De Smet, B., Price, E. P., Sarovich, D. S., Henry, D. A., et al. (2017). Comparative genomics of Burkholderia singularis sp. nov., a Low G+C Content, free-living bacterium that defies taxonomic dissection of the genus burkholderia.. Front. Microbiol. 8, 1679. doi: 10.3389/fmicb.2017.01679
Viruel, J., Forest, F., Paun, O., Chase, M. W., Devey, D., Couto, R. S., et al. (2018). A nuclear Xdh phylogenetic analysis of yams (Dioscorea: Dioscoreaceae) congruent with plastid trees reveals a new Neotropical lineage. Bot. J. Linnean Soc. 187, 232–246. doi: 10.1093/botlinnean/boy013
Wallner, G., Amann, R., and Beisker, W. (1993). Optimizing fluorescent in situ hybridization with rRNA-targeted oligonucleotide probes for flow cytometric identification of microorganisms. Cytometry 14, 136–143. doi: 10.1002/cyto.990140205
Keywords: Paraburkholderia, Dioscorea, plant-growth-promotion, phyllosphere, yams, acumen, plant-microbe-interaction, epiphyte
Citation: Herpell JB, Schindler F, Bejtović M, Fragner L, Diallo B, Bellaire A, Kublik S, Foesel BU, Gschwendtner S, Kerou M, Schloter M and Weckwerth W (2020) The Potato Yam Phyllosphere Ectosymbiont Paraburkholderia sp. Msb3 Is a Potent Growth Promotor in Tomato. Front. Microbiol. 11:581. doi: 10.3389/fmicb.2020.00581
Received: 10 January 2020; Accepted: 17 March 2020;
Published: 21 April 2020.
Edited by:Michele Perazzolli, University of Trento, Italy
Reviewed by:Stéphane Compant, Austrian Institute of Technology (AIT), Austria
Lionel Moulin, Institut de Recherche Pour le Développement (IRD), France
Copyright © 2020 Herpell, Schindler, Bejtović, Fragner, Diallo, Bellaire, Kublik, Foesel, Gschwendtner, Kerou, Schloter and Weckwerth. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Wolfram Weckwerth, firstname.lastname@example.org