Original Research ARTICLE
Two New Biocontrol Agents Against Clubroot Caused by Plasmodiophora brassicae
- 1The Key Lab of Plant Pathology of Hubei Province, Huazhong Agricultural University, Wuhan, China
- 2School of Environmental Sciences, University of Guelph, Guelph, ON, Canada
Clubroot disease caused by Plasmodiophora brassicae can lead to serious yield losses in crucifers such as Brassica napus. In this study, 323 bacterial strains were isolated from the rhizosphere of severely diseased B. napus in Dangyang county, Hubei province, China. Antagonistic strains were first identified based on dual culture inhibition zones with Fusarium oxysporum and Magnaporthe oryzae. These were then further screened in germination inhibition and viability assays of resting spores of P. brassicae. Finally, eight of the antagonistic strains were found to significantly reduce the disease severity of clubroot by more than 40% under greenhouse conditions, and two strains, F85 and T113, were found to have efficacy of more than 80%. Root hair infection experiments showed that F85 and T113 can inhibit early infection of root hairs, reduce the differentiation of primary plasmodia of P. brassicae, and inhibit formation of secondary zoosporangia. Based on sequence analysis of 16S rDNA gene, gyrA gene and 22 housekeeping genes as well as carbon source utilization analysis, the F85 was identified as Bacillus velezensis and T113 as Bacillus amyloliquefaciens. Genome analysis, PCR and RT-PCR detection revealed that both F85 and T113 harbor various antibiotic biosynthesis gene clusters required to form peptides with antimicrobial activity. To our knowledge, this is the first report of B. velezensis as a biocontrol agent against clubroot disease.
Clubroot, caused by soil-borne obligate parasite Plasmodiophora brassicae, is a serious disease on Brassica spp., especially oil-seed crops, and causes severe yield losses worldwide (Dixon and Page, 1998). Recently, clubroot disease has been increasing annually in Chongqing, Sichuan, Yunnan, and Hubei provinces and other major rapeseed-producing areas in China (Huang, 2010), and become the main disease on rapeseed. After rapeseed roots become infected, root cells proliferate abnormally, forming tumor-like bulges. The enlarged roots become cracked and then rotten due to infection by other pathogens and saprophytes. Life cycle of the pathogen consists of two key phases: in the initial phase, resting spores penetrate root hairs and epidermal cells and then form primary plasmodia; in the second phase, primary plasmodia release secondary zoospores, which then penetrate the root cortex and form galls. The mature secondary plasmodia of root cortex can form many resting spores that are released into soil (Schwelm et al., 2015).
Biocontrol with microbial antagonists has emerged as a promising alternative treatment with low environmental impact to reduce the use of synthetic fungicides. In recent decades, some antagonistic microorganisms have been identified as biological control agents (BCAs) for clubroot disease, including Trichoderma spp., Bacillus subtilis, Bacillus Amyloliquefaciens, and Lysobacter antibioticus (Cheah et al., 2000; Li et al., 2013; Zhou et al., 2014). Trichoderma can effectively prevent clubroot disease after mixing into an organic fertilizer containing actinomycetes (Joo et al., 2004). Soil-drench application of L. antibioticus cell-free culture filtrate reduced clubroot by 74.6% in greenhouse experiments (Zhou et al., 2014). The strain B. subtilis XF-1 exhibits a good suppression effect on P. brassicae with 76.9% control efficiency, and produces eight homologs of fengycin, seven homologs of dehydroxyfengycin, and six unknown fengycin-type cyclopeptides to destroy the cell wall integrity of the resting spores (Li et al., 2012).
Previous studies indicate that Bacillus spp. could produce many secondary metabolites to inhibit pathogen infection in host (Kilian et al., 2000). Lipopeptide antibiotics are a class of major antagonists produced by Bacillus. Based on chemical structure, lipopeptides have been divided into three major families: iturin, surfactin, and fengycin (Bonmatin et al., 2003). Lipopeptides are also involved in induction of resistance in plant systems (Ongena et al., 2007). Bacilysin, which is produced and excreted by many Bacillus, is a dipeptide antibiotic that resists pathogens, Staphylococcus aureus and Candida albicans (Yazgan et al., 2001). Flagellin produced by Bacillus spp. is a potent elicitor of defense responses in tomato and Arabidopsis (Felix et al., 1999). Bacillus spp. induces systemic resistance (ISR) of plants against a broad spectrum of phytopathogens (Ryu et al., 2004). For example, B. cereus AR156 induces ISR by salicylic acid/ethylene-signaling pathways in an NPR1-dependent manner which involves multiple PAMP-triggered immunity (PTI) components (Nie et al., 2017). Bacillus amyloliquefaciens SQR9 produces multiple elicitors to induce systemic resistance in Arabidopsis against DC3000 and Botrytis cinerea (Wu et al., 2018).
These lipopeptides, polyketides, dipepetide antibiotics, 2,3-butanediol, and exopolysaccharides play major roles in ISR (Wu et al., 2018). Bacillus strains have also been investigated for their capacity to protect plants by stimulating plant growth and forming multicellular structures or biofilms (Gardener, 2010; Chen et al., 2013). Rhizosphere bacteria were frequently found to form biofilm-like structures on plant roots (Morris and Monier, 2003), and biofilms from rhizobacteria play an important role in protecting plants (Timmusk et al., 2005). For example, GltB regulates biofilm formation and influences colonization of B. subtilis 916 on rice stems. Loss of gltb leads to poor efficacy against rice sheath blight (Zhou et al., 2016). Biocontrol effects of Bacillus on P. brassicae mainly include antagonistic activity (Li et al., 2013), induction of host resistance (Lahlali et al., 2013) and changes in microbial communities in the rhizosphere soil (Liu et al., 2018). However, there has been no report about biocontrol by Bacillus velezensis of clubroot.
The objectives of this study were to: (i) isolate effective antagonistic strains from the rhizosphere soil of asymptomatic rapeseed in severely infected fields; (ii) identify and characterize the selected bacterial isolates with antagonistic activities against P. brassicae; (iii) evaluate the efficacy of strains under greenhouse conditions; and (iv) identify main antimicrobial genes involved in antifungal activity in genomes of the Bacillus isolates. The goal was to identify new promising candidates to be used as BCAs against clubroot.
Materials and Methods
Soil Sample, Pathogen Inoculum, and Plant
From 2016 to 2017, soils from 5 to 15 cm deep associated with asymptomatic rapeseed were collected from severely infected fields in Dangyang county, Hubei province, China for isolation of antagonistic strains to P. brassicae and stored at 4°C. Clubroot galls were collected from infested rapeseed, dried at room temperature and stored at −20°C until used. Based on the method of Castlebury et al. (1994), crude resting spores were extracted. Approximately, 5 g of dried galls were soaked in 50 ml sterile deionized water (SDW) and then macerated in a blender at high speed for 2 min. The resulting suspension was filtered through eight layers of cheesecloth. Concentrations of resting spores were estimated with a hemocytometer and spore suspensions were diluted with SDW to 1 × 107 spores ml–1 for soil inoculation.
For measuring germination inhibition and viability assay of the resting spores of P. brassicae, the crude resting spore suspension described above was purified. It was first centrifuged at 500 RPM for 10 min. The supernatant was then centrifuged at 3100 RPM for 15 min. Pellet was re-suspended in 30 ml of SDW and centrifuged for three times. The pellet was suspended again in 5 ml of 50% sucrose and centrifuged again. Then, supernatant was centrifuged under the same conditions again. Finally, the pellet was re-suspended in 5 ml of SDW and the purified suspension was stored in a refrigerator at 4°C for 1 week.
The susceptible oilseed rape cv. Huabu-9 was used for P. brassicae inoculation in greenhouse experiments. Seeds were sterilized in 1% sodium hypochlorite for 5 min and washed three times with sterile water. The disinfected seeds were placed into Petri dishes on moist filter paper at 25°C for germination. After 4 days, seedlings were transplanted into plastic pots (10 cm × 10 cm × 15 cm) filled with soil (five seedlings per pot). On the 10th day after transplanting, the plants were inoculated with P. brassicae.
Isolation and Screening of Antagonistic Strains Against P. brassicae
Approximately 10 g of rhizosphere soil was placed in 100 ml SDW, and then shaken for 30 min at 180 RPM. Suspensions were then diluted with SDW to 10–3, 10–4, 10–5 and 10–6, and 200 μl of each diluent was plated on Martin Medium (Wang et al., 2011). The plates were incubated at 28°C and colony morphology was observed every day. The isolates were purified on Martin Medium and stored at 4°C (Lai et al., 2012).
Since cell walls of P. brassicae are similar to that of Fusarium oxysporum and Magnaporthe oryzae (Moxham and Buczacki, 1983; Liu Y. et al., 2014), these two phytopathogens (F. oxysporum strain F685 and M. oryzae strain P131) were chosen as indicator fungi to screen antagonistic strains against P. brassicae. A hyphal plug of the pathogen was placed in center of each fresh 9-cm-diam PDA plates. A colony from a freshly prepared bacterial culture was streaked around fungal plug at a distance of 3 cm using a sterile toothpick. Culture media streaked around fungal plug served as a control. Each treatment was repeated on four plates. The plates were incubated at 28°C and inhibition zones were measured after 3 days.
Germination Inhibition and Viability Assay of Resting Spores of P. brassicae
Root exudates stimulate germination of resting spores of P. brassicae (Rashid et al., 2013). Five-day-old rapeseed seedlings were transplanted individually onto a 50-ml beaker containing Hoagland’s nutrient solution and incubated at 24°C for 7 days. Root exudates were collected, filtered through a 0.22-μm cellulose nitrate filter and stored at 4°C until use. Single colonies of bacterial antagonistic strains were incubated on Luria-Bertani (LB) liquid medium at 30°C for 3 days at 180 RPM to prepare bacterial fermentation. The fermentation filtrate of bacterial isolates was centrifuged at 8000 RPM for 15 min and the supernatant was filtered through 0.22-μm cellulose nitrate filter.
Shallow liquid cultures in 50 ml flasks were used for germination inhibition assays of resting spores (Lahlali and Peng, 2014). Resting spore suspensions were diluted to 1 × 107 spores ml–1 with root exudates and pH was adjusted to 6.3 with 2M HCl. Then, 4.5 ml resting spore suspension and 0.5 ml bacterial fermentation filtrate were placed in the 50 ml flask. As a control, resting spore suspension with LB medium was incubated at the same time. All treatments were allowed to incubate under dark conditions at 25°C. After 7 days, 10 μl of suspension was placed onto a glass slide. After slight heat drying over an alcohol lamp, 50 μl of 1% orcein was added to each slide and allowed to stain for 2–3 min, and then rinsed with 95% alcohol. After drying, 10% sterilized glycerol was added and the resting spores were observed under at BS203 optical microscope. Uncolored resting spores were considered germinated (Lahlali et al., 2011). Approximately, 200 spores were examined for each treatment, with three replications. The corrected germination rate of resting spores was equal to the spore germination rate after treatment minus the rate before treatment. Germination inhibition rates of resting spores were calculated using the formula n = [(a-b)/a] ×100, where n is germination inhibition rate of resting spores, a is resting spore germination rate of the control, and b is that of the treatment.
To test viability, 0.5 ml of a suspension of resting spores (4 × 107 spores ml–1) was mixed with 0.5 ml of bacterial fermentation filtrate in a sterile tube, and incubated at room temperature. After 2 days, each treatment was mixed with an equal volume of phosphate buffer at pH 7.4 and added to 1 ml of Evans blue solution (vital stain). After mixing, it was allowed to stand for 30 min at room temperature, washed four times with distilled water, and resting spores were observed at BS203 microscope. Resting spores with dark blue color were considered as inactive. Sterile LB medium was used as control. Each experiment was repeated three times. At least 200 spores were examined from each treatment, with three repetitions. The corrected frequency for non-viable resting spores was equal to frequency of non-viable spores after treatment minus that before treatment.
In order to screen effective biocontrol strains against clubroot, soil-drench application of bacterial fermentations of all the antagonistic strains previously selected was done in the greenhouse. Each pot (10 cm × 10 cm) was inoculated with 10 ml of each bacterial fermentation described above, and each pot was inoculated with 10 ml resting spore suspension at the same time. Pots were treated with 20 ml water as the negative control and the fungicide Fluazinam was used as a positive control. Three pots were used for each treatment with three independent replicates. The treated plants were kept in a growth chamber at 25°C (16-h photoperiod, 90% RH) for 4 weeks. Clubroot severity was rated using a slightly improved grading standard (Peng et al., 2011) which included 0–3 scales: 0 = normal root growth without galling, 1 = galls on main roots or a few small galls formed on <1/3 lateral roots, 2 = galling on main root or on 1/3–2/3 lateral roots, and 3 = larger galls were formed on 2/3 of main root and lateral roots. Disease severity index (DSI) was calculated following Lahlali et al. (2013) and based on the grade standard.
Effect of Antagonistic Strains on Early Infection of P. brassicae in Root Hairs
Sandy soil was used to cultivate seedlings for observation of root hair infection. A 50-ml beaker was filled with washed and sterilized sandy soil, and wrapped with black paper to create a dark environment for germination and infestation by resting spores. Three 7-day-old rapeseed seedlings were transplanted into each beaker. Three days after transplanting, the seedlings were inoculated with 1 ml of fermentation filtrate of biocontrol strain F85 or T113 and 1 × 107 resting spores. The control was resting spore suspension alone. Each treatment was repeated three times. After inoculation, root hairs were monitored for 15 days, with nine seedlings observed for each treatment every day. Roots were washed with water, immersed in fixative solution (1:1; 95% acetic acid: 95% ethanol) for 10 min, stained in 125 ppm aniline-blue (dissolved in 50% acetic acid) for 1 min, and then rinsed with tap water for 1 min (Sharma et al., 2011). Root hairs of 1 cm in length of lower sections of hypocotyls was microscopically observed for infection.
Identification and Characterization of T113 and F85
Morphological and physiological properties and molecular characteristics of isolates F85 and T113, which were identified as having high biocontrol efficacy in greenhouse experiments were tested. To observe colony morphology, a LB medium plate was streaked and incubated at 30°C for 24 h. Gram reaction was determined by using bioMe’rieux Gram stain kit (Sooyeon et al., 2014) according to the manufacturer’s instructions. The two strains were tested for their utilization patterns of carbon sources using the BIOLOG GEN III system (El-Liethy et al., 2018) based on the manufactures’ protocols. MicroPlates were read automatically by BIOLOG GEN III system and supplied database was used to characterize the strains.
Bacterial samples were first identified based on analysis of their 16S rDNA sequence. Genomic DNA of the strains was extracted using Bacterial Genomic DNA Extraction kit (TIANamp). The 16S rDNA was amplified using universal primers 27F (5′-AGAGTTTGATCCTGGCTCAG-3′) and 1492R (5′-GGTTACCTTGTTACGACTT-3′). Each PCR reaction was carried out in a final volume of 25 μl, containing 12.5 μl 2× PCR Mix, 1 μl of each primer, 1 μl genomic DNA and 9.5 μl ddH2O. The sample was subjected to the following temperature cycling profile: 94°C for 5 min, followed by 35 cycles of 94°C for 30 s, 50°C for 30 s, 72°C for 1.5 min, with a final extension step of 10 min at 72°C. PCR products were detected by 1% agarose gel electrophoresis and sequenced by the TSINGKE Biological Technology Company (Beijing, China). The 16S rDNA sequences were compared with GenBank databases1 using the BLAST search program. Second, to confirm the BLAST results, gyrA sequences were amplified with primers gyrA-f (5′-CAGTCAGGAAATGCGTACGTCCTT-3′) and gyrA-r (5′-CAAGGTAATGCTCCAGGCATTGCT-3′) (Chen et al., 2016) to construct a phylogenetic tree. The determined gyrA sequences were compared with GenBank databases and aligned with CLUSTALX (Jeanmougin et al., 1998). MEGA 7.0 software (Tamura et al., 2007) was used to conduct phylogenetic analyses using Maximum-likelihood method with 1000 bootstrap tests.
To further confirm the species identities of T113 and F85, 22 housekeeping genes, including dnaG, frr, infC, nusA, pgk, pyrG, rplA, rplB, rplC, rplD, rplE, rplF, rplK, rplL, rplP, rplT, rpmA, rpoB, rpsB, rpsM, smpB, and tsf, were extracted from the assembled genomes of F85 and T113, and chosen to splice sequences for analyze the phylogenetic relationship in Bacillus species using Maximum-likelihood method as described above.
Genomic Sequencing and Annotation
Genomic DNA of T113 and F85 was extracted using Wizard® Genomic DNA Purification Kit (Promega) according to the manufacturer’s protocol. For Illumina sequencing, at least 1 μg genomic DNA was used for each strain in sequencing library construction. DNA samples were sheared into 400–500 bp fragments using a Covaris M220 Focused Acoustic Shearer following the manufacture’s protocol. Illumina sequencing libraries were prepared from sheared fragments using NEXTflexTM Rapid DNA-Seq Kit. Prepared libraries were then used for paired-end Illumina sequencing (2 bp × 150 bp) on an Illumina HiSeq X Ten platform (Majorbio Bio-pharm Technology, Shanghai, China).
Data generated were used for bioinformatic analysis using I-Sanger Cloud Platform2 from Shanghai Majorbio, using procedures as follows. Original image data were transferred into sequence data via base calling, which were defined as raw data or raw reads and saved as FASTQ files. Those FASTQ files were the original data provided for users, which included detailed read sequences and read quality information. Statistical analysis of quality information was performed for quality trimming, which removed low quality data could be removed to leave a clean data. An assembly of clean reads was performed using SOAPdenovo2.
Glimmer v3.023 was used for coding sequence (CDS) prediction, tRNA-scan-SE v2.0.54 was used for tRNA prediction, and Barrnap5 was used for rRNA prediction (Guo et al., 2012; Dunlap et al., 2013). The predicted CDSs were annotated from NR, Swiss-Prot, Pfam, GO, COG, and KEGG database using sequence alignment tools such as BLAST, Diamond and HMMER. Briefly, each set of query proteins were aligned with the databases, and annotations of best-matched subjects (e-value < 10–5) were obtained for gene annotation.
Identification and Expression of Antimicrobial Biosynthesis Genes
PCR detection was performed to detect antimicrobial peptide biosynthetic genes with pre-existing primers (Mora et al., 2011; Yang et al., 2015; Sajitha et al., 2016). Amplification of 15 antimicrobial biosynthesis genes was performed using specific primers (Table 1). PCR amplifications were conducted in 25 μL of reaction mixtures containing 12.5 μl 2× PCR Mix, 1 μl PCR primer, 1 μl genomic DNA and 9.5 μl ddH2O. The sample was subjected to the following temperature cycling profile: 94°C for 5 min; followed by 35 cycles of 94°C for 30 s, 50°C for 30 s, 72°C for 1.5 min, with a final extension of 10 min at 72°C. PCR products were detected using 1% agarose gel electrophoresis.
Expression of antimicrobial biosynthesis genes was analyzed using reverse transcription PCR (RT-PCR). Samples were collected from bacteria grown for 1 day in liquid LB. Total RNA was extracted with the OMEGA Bio-tek Bacterial RNA Kit (OMEGA, Guangzhou, China). Reverse transcription assays were performed using TransScriptTM One-Step Gdna Removal and cDNA Synthesis SuperMix Kit (TransGen, Beijing, China). RT-PCR mixtures were composed of 12.5 μL of 2× HieffTM PCR Master Mix (YeSen, Shanghai, China), 1 μL of cDNA, 1 μL of each primer, and 9.5 μL nuclease-free water. The experiment was repeated three times.
To further determine whether antimicrobial biosynthesis genes were expressed upon interaction with P. brassicae, resting spores were treated with F85 or T113 bacterial cells for germination inhibition assays as described above. Total RNA was extracted from suspensions at 0, 12, 14, and 16 h after treatment. The F85 or T113 bacterial suspension treated with root exudates served as a control. RT-PCR manipulation was conducted as described above.
Data were subjected to analyses of variance (ANOVA) using SPSS 13.0 software (SPSS, Inc., Chicago, IL, United States). Mean comparisons were conducted using a least significant difference (LSD) test (P = 0.05).
Screening of Antagonistic Bacterial Strains Against P. brassicae
A total of 323 bacterial strains were isolated from the rhizosphere of asymptomatic oilseed rape plants in severely diseased fields. Among these bacterial strains, 54 were found to have potential antagonistic activities in dual culture streak plates, as their average inhibition of the two indicator fungi was greater than 3 mm (Figures 1A,B). Notably, 17 strains (F2, T91, F85, T115, T71, F10, F11, T73, C12, T111, T48, D13, T55, T84, T113, T70, and F3) had inhibition zones greater than 10 mm (Figure 1A). These 54 bacterial strains with potential antagonistic activities were selected for further testing.
Figure 1. Streak plate method to screen antagonistic strains by using indicator fungi, Fusarium oxysporum and Magnaporthe oryzae. (A) Average size of inhibition zones of the two indicator fungi. Each experiment was repeated three times. (B) Inhibition zones of biocontrol strains against the two fungi. The red line indicated the inhibition zones greater than 10 mm as the cut-off value. Data are presented as mean ± SD. Different letters indicate significant differences between treatments according to LSD test (P < 0.05). Capped lines represent standard errors.
Inhibitory Effects of Antagonistic Strains on Germination and Viability of Resting Spores
The 54 bacterial strains with inhibition zone greater than 3 mm were tested for their inhibitory effects on germination and viability of resting spores. After staining with orcein dye, 20 strains, including T84, F30, F85, F3, F11, A46, T67, T111, T117, D16, E66, C12, F10, T115, D14, F2, T73, D13, T71 and T113, were found to have large inhibitory effects on the germination rate of resting spores (36–49 vs. 71% in the control) (Figure 2A). Particularly, strain T113 produced the lowest resting spore germination rate at 36%.
Figure 2. Inhibitory effect of antagonistic strains on the germination and viability of resting spores. (A) Resting spore germination rate of Plasmodiophora brassicae after treatment with biocontrol strains. Each experiment was repeated three times. Data are presented as mean ± SD. Capped lines represent standard errors. (B) Deactivation rate of resting spores of P. brassicae.
All 54 bacterial strains were also tested for their inhibitory effects on viability of resting spores based on vital staining with Evan’s blue. Thirteen strains, C12, F2, T113, A46, T91, F85, T73, D14, D13, T115, E66, F10 and D16, showed high deactivation effects on resting spores (45–55 vs. 12% in the control) (Figure 2B), particularly C12, which resulted in a maximum deactivation rate (54.7%) of resting spores.
Biocontrol Effects of Antagonistic Strains on Clubroot Disease Under Greenhouse Conditions
To investigate the suppressive effects of antagonistic bacteria on clubroot, strains E66, A46, D14, C12, T73, F2, T71, T115, D13, D16, F85, and T113 with potent inhibitory effects on germination and viability of resting spores were tested under greenhouse conditions. The positive control, fungicide Fluazinam, effectively suppressed clubroot resulting in a disease index of 10.9. Disease index of rapeseeds inoculated with P. brassicae alone was 95.6, whereas treatment with different antagonistic bacterial strains reduced the disease index to 10–80. Among these strains, F85 showed significant suppression activities on P. brassicae with a disease index value of 15.9 and T113 was 13.2 (Figure 3).
Figure 3. Control efficiency of the biocontrol bacterial strains against P. brassicae in greenhouse. (A) Morphology of rapeseed roots of each bacterial treatment. (B) Disease incidence of clubroot treated with bacterial suspensions. Each experiment was repeated three times. Different letters indicate significant differences between different treatments according to LSD test (P < 0.05). Capped lines represent standard errors.
Effect of Antagonistic Strains on Early Infection of P. brassicae
Strains F85 and T113, which produced the best disease suppression effect, were selected for root hair infection experiments. In blank control treatment, zoospores infected the root hairs at 2 days after inoculation (DAI) and primary plasmodia were formed at 3 DAI. Secondary zoosporangia developed in root hairs at 6 DAI and secondary zoospores infected the root cortex to result in secondary infection at 9 DAI (Figure 4A). Inoculation with F85 or T113, delayed and suppressed zoospore infection. Primary plasmodia were formed at 5 DAI and secondary zoosporangia in root hairs were observed at 7 DAI. Secondary zoospores infected cortex of root hairs to cause secondary infection at 13 DAI (Figures 4B,C). Compared with the control, the F85 or T113 treatment effectively inhibited root hair infection as well as formation of primary plasmodia and secondary zoosporangia (Figures 4D–F). Hence, both F85 and T113 could effectively suppress root hair infection of P. brassicae.
Figure 4. Inhibition of the infection process of P. brassicae on rapeseed root hairs by F85 and T113. (A) Root hair infection process of untreated control. The zoospores infected root hairs in 2 DAI, formed primary plasmodia in 3 DAI, secondary zoosporangia in 6 DAI and started secondary infection in 9 DAI. RS, resting spore; PP, primary plasmodia; SZ, secondary zoosporangia; SI, secondary infection. (B) Root hair infection process of T113 treatment. The zoospores infected root hairs in 3 DAI, formed primary plasmodia in 5 DAI, secondary zoosporangia in 7 DAI, and started secondary infection in 15 DAI. (C) Root hair infection process of F85 treatment. The zoospores infected root hairs in 3 DAI, formed primary plasmodia in 5 DAI, secondary zoosporangia in 7 DAI and started secondary infection in 15 DAI. (D) Percentage of root hair infection (%) after treated with F85 or T113. (E) Percentage of primary plasmodium formation (%). (F) Percentage of second zoosporangia formation (%). CK: water. Different letters indicate significant differences between treatments according to LSD test (P < 0.05). Capped lines represent standard errors.
Identification and Molecular Characterization of F85 and T113
Analysis of morphological, biochemical, physiological, and molecular characteristics of F85 and T113 were used for taxonomic identification. Both strains were found to be Gram-positive, rod-shaped bacteria (Figure 5). Characteristics detected by BIOLOG GEN III MicroPlate are shown in Supplementary Table S1. Based on these characteristics, F85 and T113 were automatically classified as Bacillus spp. which was also confirmed by sequence analysis of 16S rDNA gene.
Figure 5. Colony morphology and gram staining of the F85 and T113. Both strains strained purpled, identifying them as Gram-positive bacteria. The cells were rod-shaped. The F85 colonies were khaki, the edges were clearcut, and the surface was dry and opaque. The colony of T113 had a dull color and a smooth, translucent surface.
Analysis of a partial gyrA sequence demonstrated that F85 was matched B. velezensis SCGB 1CP023320.1 at 99%, while T113 was matched B. amyloliquefaciens UCMB5036 at 99%.
Sequence analysis of gyrA was carried out to assess its taxonomic position in the phylogenetic tree. The results indicated that F85 and B. velezensis were clustered in one group while T113 and B. amyloliquefaciens were clustered in another group, which were distinctly separated from other species of Bacillus (Figure 6A). To confirm the identification, we also constructed a phylogenetic tree based on 22 housekeeping genes from bacterial genomes. The phylogenetic analysis was consistent with previous results (Figure 6B).
Figure 6. Phylogenetic trees based on the partial nucleotide sequence of gyrA (A) and 22 housekeeping genes (B). A Maximum-likelihood phylogenetic tree of F85 and T113 was constructed using MEGA 7.0. The numbers at nodes indicate levels of bootstrap support (%) based on a Maximum-likelihood analysis of 1000 re-sampled datasets; only values greater than 50% are provided.
Based on morphological, physiological and biochemical characteristics and the results of sequence analysis, F85 was identified as B. velezensis and T113 as B. amyloliquefaciens.
Genomic Features and Antibiotic Biosynthesis Analysis of B. velezensis F85 and B. amyloliquefaciens T113
To investigate biosynthesis features of antibiotics in F85 and T113, two libraries were generated to investigate antibiotic biosynthesis genes. In general, both samples showed high quality, with >99% of base reads at Q20 (rate of bases with quality >20) and 96% of base reads >Q30 (rate of bases with quality >30) (Table 2). The distribution of base composition and quality on the clean reads are shown in Supplementary Figures S1, S2. The whole genomes of F85 and T113 were sequenced, revealing a complete circular genome 4,080,442 bp in length and a GC content of 45.98%, while the T113 genome was a complete circular genome 3,988,935 bp in length with a GC content of 46.31% (Table 3). The major features of F85 and T113 genomes are shown in Figures 7A, 8A as circular graphs.
Figure 7. Circular genome visualization, and GO annotation and KEGG pathway analysis of F85. (A) Circular representation of the F85 genome. From outside to inside, circle 1: scale; circles 2 and 3: predicted CDSs color-coded according to their functions; circle 4: rRNA and tRNA; circle 5: GC content; circle 6: GC skew (G+C/G-C). (B) GO annotation of F85, mainly including three major categories: ‘biological processes,’ ‘cellular component,’ and ‘molecular function.’ (C) KEGG pathway analysis of F85. KEGG pathway can be divided into seven categories: Metabolism, Genetic Information Processing, Environmental Information Processing, Cellular Processes, Organismal Systems, Human Diseases, and Drug Development.
Figure 8. Circular genome visualization, and GO and KEGG pathway analysis of T113. (A) Circular representation of T113 genome. (B) GO annotation of T113. (C) KEGG pathway analysis of T113.
Functional distributions of genes and their genetic relationships were assessed by Gene Ontology (GO) annotation and Kyoto Encyclopedia of Genes and Genomes (KEGG) pathway analysis. Annotation of F85 and T113 genomes revealed that main GO categories were ‘biological processes,’ ‘cellular component,’ and ‘molecular function’ (Figures 7B, 8B). A total of 2425 genes were annotated in the GO classification of F85 (Supplementary Table S2), and the most enriched terms for ‘biological processes’ were metabolic process (1338 genes), cellular process (1119 genes) and single-organism process (899 genes). The most enriched terms for the ‘cellular component’ were membrane (780 genes) and membrane part (738 genes). In the ‘molecular function,’ there were the largest numbers of genes in catalytic activity (1382 genes) and binding (948 genes). Almost 2500 genes were annotated in the GO classification of T113 (Supplementary Table S3). The most enriched terms for ‘biological processes’ were metabolic process (1361 genes), cellular process (1132 genes) and single-organism process (940 genes). The most enriched terms for the ‘cellular component’ were membrane (794 genes) and membrane part (757 genes). In the ‘molecular function,’ there were the largest numbers of genes in catalytic activity (1409 genes) and binding (973 genes).
A total of 2024 genes were annotated in the KEGG pathway of F85 (Supplementary Table S4). Representative pathways were ‘cellular processes’ (160 genes), ‘metabolism’ (1287 genes), ‘human diseases’ (85 genes), ‘genetic information processing’ (174 genes), ‘organismal systems’ (35 genes) and ‘environmental information processing’ (283 genes) (Figure 7C). For T113, 2027 genes were annotated in the KEGG pathway (Supplementary Table S2). The representative pathways were ‘cellular processes’ (163 genes), ‘metabolism’ (1287 genes), ‘human diseases’ (87 genes), ‘genetic information processing’ (169 genes), ‘organismal systems’ (35 genes) and ‘environmental information processing’ (286 genes) (Figure 8C).
Subsequently, antibiotic biosynthesis genes were detected from the enriched categories of GO annotation and KEGG pathway. Antibacterial metabolites could be grouped into two separate classes: ribosome-synthesized peptides such as bacteriocin, and small microbial peptides enzymatically synthesized by non-ribosomal pathways, mainly cyclic lipopeptides (Finking and Marahiel, 2004; Romero et al., 2007; Baruzzi et al., 2011). The F85 and T113 genomes contained antibiotic biosynthesis gene clusters associated with both ribosomal and non-ribosomal synthesized peptides (Tables 4, 5). In F85 and T113, these gene clusters comprised genes that encode non-ribosomal peptide synthetases mainly including lipopeptides, peptides, polyketide and terpenoids, and ribosomal peptide synthetases including bacteriocin and antibacterial proteins. The other secondary metabolites related to antibiotic synthesis were identified from the pathway database, including ansamycins, carbapenem, streptomycin, monobactam, phenylpropanoid, penicillin, and cephalosporin. The substances encoded by these genes might be involved in synthesis of these antibiotics.
The antibiotic biosynthesis genes in B. velezensis F85 and B. amyloliquefaciens T113 were amplified to confirm presence of the genes in these genomes. PCR detection showed that all selected antibiotic biosynthesis genes were amplified in F85 and only mycB was not detected in T113 genomic DNA (Figures 9A,B). PCR products were finally confirmed by sequencing.
Figure 9. Identification and expression of antimicrobial biosynthesis genes. PCR amplification of lipopeptide biosynthetic genes from F85 (A) and T113 (B). RT-PCR amplification of lipopeptide biosynthetic genes from F85 (C) and T113 (D). Lane 1: srfAA; Lane 2: fenB; Lane 3: fend; Lane 4: ITUDI; Lane 5: ituD; Lane 6: ituA; Lane 7: ituC; Lane 8: mycB; Lane 9: bmyB; Lane 10: bmyD; Lane 11: BACD; Lane 12: BACAB; Lane 13: BAC; Lane 14: hag; Lane 15: tasA. Marker: TaKaRa DL5000 (TaKaRa, Dalian, China).
Expression levels of the 15 antibiotic biosynthesis genes in bacterial cells were further evaluated using RT-PCR, and the results showed that 12 genes (srfAA, fenB, fend, ITUDI, ituC, mycB, bmyD, BACD, BACAB, BAC, hag and tasA) were expressed in F85 while eight genes (srfAA, ITUDI, bmyB, bmyD, BACD, BACAB, BAC, and tasA) were expressed in T113 (Figures 9C,D). Then, other three non-expressed genes from F85 and seven non-expressed genes from T113 were all chosen to determine whether these antimicrobial biosynthesis genes were expressed upon interaction with P. brassicae. However, all selected genes were still not expressed. Hence, many antimicrobial biosynthesis genes were identified in F85 and T113, and expression of these genes could lead to the synthesis of antibiotic compounds.
In this study, isolation and screening of biocontrol bacteria from the rhizosphere of healthy plants in severely diseased fields were carried out. The assumption was that, if no symptoms had developed for plants growing in clubroot-infested soil, an antagonist may have prevented infection by P. brassicae. P. brassicae is an obligate parasite that cannot be cultured in vitro, which presents a bottleneck for the large-scale screening of biocontrol bacteria against P. brassicae (Bi et al., 2016). For screening of biocontrol bacteria against clubroot, a variety of pathogenic fungi could be used as indicator fungi for antagonistic test, particularly the pathogenic fungus F. oxysporum. The cell wall of P. brassicae is similar to that of F. oxysporum and M. oryzae (Moxham and Buczacki, 1983; Liu Y. et al., 2014). Fifty-four strains of biocontrol bacteria with apparent inhibition zones in dual plate cultures with the test pathogens were then screened in resting spore germination and viability assays, which are more precise and comprehensive than previous research methods. Two potential biocontrol strains, F85 and T113 both exhibited good inhibitory effects on germination and viability of resting spores (Supplementary Figure S3), and produced greater than 80% disease suppression in greenhouse experiments. The efficacy of these two strains is better than that of previously reported biocontrol strains (Jäschke et al., 2010; Lahlali et al., 2013; Zhou et al., 2014). In order to improve the efficiency of the biocontrol agents under high disease pressure, it will be necessary to examine the combined effect of F85 and T113 against P. brassicae in the future. BIOLOG analysis is always used to identify species of bacteria. However, it is really hard to distinguish characteristics of carbon source utilization between different species of Bacillus. In this case, the gyrA sequence provides a firm framework for the rapid and accurate classification and identification of B. subtilis and related taxa (Chun and Bae, 2000). In this study, F85 and T113 could be easily identified as B. velezensis and B. amyloliquefaciens, respectively, by the single gene gyrA. The results were consistent with identification using 22 housekeeping genes in phylogenetic analysis. Liu X. et al. (2014) reported that B. amyloliquefaciens strain HB-26 showed approximately 60% inhibition activity against P. brassicae in Chinese cabbage pot experiment (Liu X. et al., 2014). Noticeably, the B. amyloliquefaciens strain T113 used in this study exhibited higher suppressive effect on clubroot. Moreover, the present study reports the first description of the biological potential of F85, a B. velezensis strain, to reduce clubroot. However, further work is needed to explore mechanisms of these Bacillus strains to suppress infection of P. brassicae.
The lipopeptide antibiotics produced by Bacillus spp. have been generally assumed to have antifungal activity. Strains of B. amyloliquefaciens produce various antimicrobial lipopeptides including iturins, surfactins and fengycins against phytopathogens (Kim et al., 2010; Pathak and Keharia, 2014). Bacillus subtilis XF-1 is highly protective against P. brassicae. It was predicted to produce cyclic lipopeptide (CLP) antibiotics by genomic analysis, and the CLP were identified by LC/ESI-MS and LC/ESI-MS/MS as fengycin B, fengycin C, fengycin D, and fengycin S (Li et al., 2013). Most Bacillus species produce two to four antimicrobial peptides (AMPs) with bacteriostatic effects and structural stability (Mora et al., 2011). Bacillus subtilis YB-05 has at least four antifungal genes (fenB, ituA, hag, and tas) (Yang et al., 2015). Bacillus subtilis strain A1/3 showed exceptionally diverse antibiotic capacities compared with other B. subtilis strains. It has six AMP (antimicrobial peptides) genes, including srf (surfactin), bacA (bacylisin), fenD (fengycin), bmyB (bacyllomicin), spaS (bubtilin), and ituC (iturin) (Hofemeister et al., 2004). Compared with previous studies, the two highly protective strains F85 and T113 in this work contain more than 10 antibiotic biosynthesis genes, belonging to multiple types of antibiotics including non-ribosomal peptide synthetase and ribosomal peptide synthetase. Hence, F85 and T113 could produce a variety of antibiotics, and both have great potential in biocontrol research in the future.
In summary, two new potential biocontrol strains against clubroot, B. velezensis F85 and B. amyloliquefaciens T113, were identified from Brassica napus rhizosphere. To our knowledge, this is the first report of a B. velezensis strain as a promising biocontrol agent against this disease. Future studies to elucidate biocontrol mechanism and field control efficacy of F85 and T113 are needed, and such information may lead to development of novel strategies to manage clubroot caused by P. brassicae.
Data Avalability Statement
The original genome sequence data of strains F85 and T113 are available in GenBank (Accession SRR9925238 and SRR9925239).
LZ designed the experiments. MZ, YH, YL, TR, and HL performed the experimental work. MZ, LZ, JH, DJ, and TH analyzed the data. MZ, LZ, and TH wrote the manuscript.
This work was supported by the National Key Research and Development Program of China (2018YFD0200902 and 2018YFD0200904) and the China Agriculture Research System (CARS13).
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.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2019.03099/full#supplementary-material
FIGURE S1 | Distribution of base composition on clean reads of F85 and T113 genomic data. (A) Distribution of base composition on clean reads in F85. (B) Distribution of base composition on clean reads in T113. X axis represents base position along reads. Y axis represents base content percentage. Different bases are represented by different colors. As to high quality sequencing reads, A (adenine base) curve should be strictly overlapped with T (thymine base) curve, and G (guanine bsase) curve should be overlapped with C (cytosine base) curve according to the principle of complementary base pairing.
FIGURE S2 | Distribution of base quality on clean reads of F85 and T113 genomic data. (A) Distribution of base quality on clean reads in F85. (B) Distribution of base quality on clean reads in T113. X axis represents base positions along reads. Y axis represents base quality value. The first half is Q-value distribution of reads at the first end of the double-end sequencing sequence, and Q-value distribution of the sequencing reads at the other end.
FIGURE S3 | Inhibitory effect of F85 and T113 on the germination and viability of P. brassicae resting spores. (A) Germination of resting spore was inhibited by F85 or T113. After staining with orcein dye, resting spores without color were considered to be germinating whereas colored spores were considered to be non-germinated ones. G, germinated resting spores; N, non-germinated resting spores. Bar = 50 μm. (B) Viability of resting spores were reduced by F85 or T113. Colorless resting spores were active and dark blue resting spores were inactive. V, viable resting spores; I, inactive resting spores. Bar = 50 μm. Each experiment was repeated three times.
TABLE S1 | Carbon source utilization pattern of F85 and T113 using BIOLOG GEN III system.
TABLE S2 | Number of genes of F85 in category of GO annotation.
TABLE S3 | Number of genes of T113 in category of GO annotation.
TABLE S4 | Number of genes in category of KEGG pathway.
- ^ http://www.ncbi.nlm.nih.gov
- ^ www.i-sanger.com
- ^ http://ccb.jhu.edu/software/glimmer/index.shtml
- ^ http://lowelab.ucsc.edu/tRNAscan-SE/
- ^ http://www.vicbioinformatics.com/software.barrnap.shtml
Baruzzi, F., Quintieri, L., Morea, M., and Caputo, L. (2011). “Antimicrobial compounds produced by Bacillus spp. and applications in food,” in Science Against Microbial Pathogens: Communicating Current Research and Technological Advances, Vol. 2, ed. Méndez-Vilas (Badajoz: Formatex Research Centre), 1102–1111.
Bonmatin, J. M., Laprevote, O., and Peypoux, F. (2003). Diversity among microbial cyclic lipopeptides: iturins and surfactins. Activity-structure relationships to design new bioactive agents. Comb. Chem. High Throughput Screen 6, 541–556. doi: 10.2174/138620703106298716
Castlebury, L. A., Maddox, J. V., and Glawe, D. A. (1994). A technique for the extraction and purification of viable Plasmodiophora brassicae resting spores from host root tissue. Mycologia 86, 458–460. doi: 10.2307/3760580
Chen, X., Zhang, Y., Fu, X., Li, Y., and Wang, Q. (2016). Isolation and characterization of Bacillus amyloliquefaciens PG12 for the biological control of apple ring rot. Postharvest Biol. Technol. 115, 113–121. doi: 10.1016/j.postharvbio.2015.12.021
Chen, Y., Yan, F., Chai, Y., Liu, H., Kolter, R., Losick, R., et al. (2013). Biocontrol of tomato wilt disease by Bacillus subtilis isolates from natural environments depends on conserved genes mediating biofilm formation. Environ. Microbiol. 15, 848–864. doi: 10.1111/j.1462-2920.2012.02860.x
Dixon, G. R., and Page, L. V. (1998). Calcium and nitrogen eliciting alterations to growth and reproduction of Plasmodiophora brassicae (clubroot). Acta Hortic. 459, 343–349. doi: 10.17660/ActaHortic.1998.459.40
Dunlap, C. A., Bowman, M. J., and Schisler, D. A. (2013). Genomic analysis and secondary metabolite production in Bacillus amyloliquefaciens as 43.3: a biocontrol antagonist of Fusarium head blight. Biol. Control 64, 166–175. doi: 10.1016/j.biocontrol.2012.11.002
El-Liethy, M. A., Hemdan, B. A., and El-Taweel, G. E. (2018). Phenotyping using semi-automated BIOLOG and conventional PCR for identification of Bacillus isolated from biofilm of sink drainage pipes. Acta Ecol. Sin. 38, 334–338. doi: 10.1016/j.chnaes.2018.01.011
Felix, G., Duran, J. D., Volko, S., and Boller, T. (1999). Plants have a sensitive perception system for the most conserved domain of bacterial flagellin. Plant J. 18, 265–276. doi: 10.1046/j.1365-313x.1999.00265.x
Guo, Y., Wang, H., Li, Y., Song, Y., Chen, C., and Liao, Y. (2012). Genome of Helicobacter pylori strain xz274, an isolate from a tibetan patient with gastric cancer in China. J. Bacteriol. 194, 4146–4147. doi: 10.1128/JB.00804-12
Hofemeister, J., Conrad, B., Adler, B., Hofemeister, B., Feesche, J., Kucheryava, N., et al. (2004). Genetic analysis of the biosynthesis of non-ribosomal peptideand polyketide-like antibiotics, iron uptake and biofilm formation by Bacillus subtilis A1/3. Mol. Genet. Genomics 272, 363–378. doi: 10.1007/s00438-004-1056-y
Jäschke, D., Dugassa-Gobena, D., Karlovsky, P., Vidal, S., and Ludwig-Müller, J. (2010). Suppression of clubroot (Plasmodiophora brassicae) development in Arabidopsis thaliana by the endophytic fungus Acremonium alternatum. Plant Pathol. 59, 100–111. doi: 10.1111/j.1365-3059.2009.02199.x
Joo, G. J., Kim, Y. M., Kim, J. W., Kim, W. C., Rhee, I. K., Choi, Y. H., et al. (2004). Biocontrol of cabbage clubroot by the organic fertilizer using Streptomyces sp. AC-3. K. J. Microbiol. Biotechnol. 32, 172–178.
Kilian, M., Steiner, U., Krebs, B., Junge, H., Schmiedeknecht, G., and Hain, R. (2000). FZB24® Bacillus subtilis–mode of action of a microbial agent enhancing plant vitality. Pflanzenschutz Nachr. Bayer 1, 72–93.
Kim, P. I., Ryu, J., Kim, Y. H., and Chi, Y. T. (2010). Production of biosurfactant lipopeptides iturin A, fengycin and surfactin A from Bacillus subtilis CMB32 for control of Colletotrichum gloeosporioides. J. Microbiol. Biotechnol. 20, 138–145. doi: 10.4014/jmb.0905.05007
Lahlali, R., Peng, G., Gossen, B. D., Mcgregor, L., Yu, F. Q., Hynes, R. K., et al. (2013). Evidence that the biofungicide serenade (Bacillus subtilis) suppresses clubroot on canola via antibiosis and induced host resistance. Phytopathology 103, 245–254. doi: 10.1094/PHYTO-06-12-0123-R
Lahlali, R., Peng, G., McGregor, L., Gossen, B. D., Hwang, S. F., and McDonald, M. (2011). Mechanisms of the biofungicide Serenade (Bacillus subtilis QST713) in suppressing clubroot. Biocontrol Sci. Technol. 21, 1351–1362. doi: 10.1080/09583157.2011.618263
Lai, K., Chen, S., Hu, M., Hu, Q., Geng, P., Weng, Q., et al. (2012). Control of postharvest green mold of citrus fruit by application of endophytic Paenibacillus polymyxa strain SG-6. Postharvest Biol. Technol. 69, 40–48. doi: 10.1016/j.postharvbio.2012.03.001
Li, X. Y., Mao, Z. C., Wang, Y. H., Wu, Y. X., He, Y. Q., and Long, C. L. (2012). ESI LC-MS and MS/MS characterization of antifungal cyclic lipopeptides produced by Bacillus subtilis XF-1. J. Mol. Microb. Biotech. 22, 83–93. doi: 10.1159/000338530
Li, X. Y., Mao, Z. C., Wang, Y. H., Wu, Y. X., He, Y. Q., and Long, C. L. (2013). Diversity and active mechanism of fengycin-type cyclopeptides from Bacillus subtilis XF-1 against Plasmodiophora brassicae. J. Microbiol. Biotechnol. 23, 313–321. doi: 10.4014/jmb.1208.08065
Liu, C., Yang, Z., He, P., Munir, S., Wu, Y., Ho, H., et al. (2018). Deciphering the bacterial and fungal communities in clubroot-affected cabbage rhizosphere treated with Bacillus Subtilis XF-1. Agric. Ecosyst. Environ. 256, 12–22. doi: 10.1016/j.agee.2018.01.001
Liu, X., Zhang, W., Min, Y., Zhang, Y., Zhang, Z., and Jiang, A. (2014). Separation and characterization of Bacillus amyloliquefaciens active substances against Plasmodiophora brassicae. Amino Acids Biotic Resour. 36, 39–43. doi: 10.14188/j.ajsh.2014.01.009
Liu, Y., Du, Y., Qiao, J., Liang, X., Wang, S., and Li, J. (2014). Screening, identification and evaluation of antagonistic bacteria against Plasmodiophora brassicae. J. Nanjing Agric. Univ. 37, 83–90.
Morris, C. E., and Monier, J. M. (2003). The ecological significance of biofilm formation by plant-associated bacteria. Annu. Rev. Phytopathol. 41, 429–453. doi: 10.1146/annurev.phyto.41.022103.134521
Nie, P., Li, X., Wang, S., Guo, J., Zhao, H., and Niu, D. (2017). Induced systemic resistance against Botrytis cinerea by Bacillus cereus AR156 through a JA/ET-and NPR1-dependent signaling pathway and activates PAMP-triggered immunity in Arabidopsis. Front. Plant Sci. 8:238. doi: 10.3389/fpls.2017.00238
Ongena, M., Jourdan, E., Adam, A., Paquot, M., Brans, A., and Joris, B. (2007). Surfactin and fengycin lipopeptides of Bacillus subtilis as elicitors of induced systemic resistance in plants. Environ. Microbiol. 9, 1084–1090. doi: 10.1111/j.1462-2920.2006.01202.x
Peng, G., McGregor, L., Lahlali, R., Gossen, B. D., Hwang, S. F., Adhikari, K. K., et al. (2011). Potential biological control of clubroot on canola and crucifer vegetable crops. Plant Pathol. 60, 566–574. doi: 10.1111/j.1365-3059.2010.02400.x
Rashid, A., Ahmed, H. U., Xiao, Q., Hwang, S. F., and Strelkov, S. E. (2013). Effects of root exudates and pH on Plasmodiophora brassicae resting spore germination and infection of canola (Brassica napus L.) root hairs. Crop Prot. 48, 16–23. doi: 10.1016/j.cropro.2012.11.025
Romero, D., Vicente, A. D., Rakotoaly, R. H., Dufour, S. E., Veening, J. W., Arrebola, E., et al. (2007). The iturin and fengycin families of lipopeptides are key factors in antagonism of Bacillus subtilis toward Podosphaera fusca. Mol. Plant Microbe Interact. 20, 430–440. doi: 10.1094/MPMI-20-4-0430
Ryu, C. M., Farag, M. A., Hu, C. H., Reddy, M. S., Kloepper, J. W., and Paré, P. W. (2004). Bacterial volatiles induce systemic resistance in Arabidopsis. Plant Physiol. 134, 1017–1026. doi: 10.1104/pp.103.026583
Sajitha, K. L., Dev, S. A., and Florence, E. M. (2016). Identification and characterization of lipopeptides from Bacillus subtilis B1 against sapstain fungus of rubberwood through MALDI-TOF-MS and RT-PCR. Curr. Microbiol. 73, 46–53. doi: 10.1007/s00284-016-1025-9
Schwelm, A., Fogelqvist, J., Knaust, A., Jülke Sabine Lilja, T., and Bonilla-Rosso, G. (2015). The Plasmodiophora brassicae genome reveals insights in its life cycle and ancestry of chitin synthases. Sci. Rep. 5:11153. doi: 10.1038/srep11153
Sharma, K., Gossen, B. D., and McDonald, M. R. (2011). Effect of temperature on primary infection by Plasmodiophora brassicae and initiation of clubroot symptoms. Plant Pathol. 60, 830–838. doi: 10.1111/j.1365-3059.2011.02458.x
Sooyeon, P., Doo-Sang, P., Kyung Sook, B., and Jung-Hoon, Y. (2014). Phaeobacter aquaemixtae sp. nov., isolated from the junction between the ocean and a freshwater spring. Neurosci. Lett. 283, 109–112. doi: 10.1016/S0304-3940(00)00917-4
Timmusk, S., Grantcharova, N., and Wagner, E. G. H. (2005). Paenibacillus polymyxa invades plant roots and forms biofilms. Appl. Environ. Microbiol. 71, 7292–7300. doi: 10.1128/AEM.71.11.7292-7300.2005
Wu, G., Liu, Y., Xu, Y., Zhang, G., Shen, Q., and Zhang, R. (2018). Exploring elicitors of the beneficial rhizobacterium Bacillus amyloliquefaciens SQR9 to induce plant systemic resistance and their interactions with plant signaling pathways. Mol. Plant Microbe Interact. 31, 560–567. doi: 10.1094/MPMI-11-17-0273-R
Yang, L., Quan, X., Xue, B., Goodwin, P. H., Lu, S., and Wang, J. (2015). Isolation and identification of Bacillus subtilis strain yb-05 and its antifungal substances showing antagonism against Gaeumannomyces graminis var. tritici. Biol. Control 85, 52–58. doi: 10.1016/j.biocontrol.2014.12.010
Yazgan, A., Özcengiz, G., Özcengiz, E., Kılınç, K., Marahiel, M. A., and Alaeddinoğlu, N. G. (2001). Bacilysin biosynthesis by a partially-purified enzyme fraction from Bacillus subtilis. Enzyme Microb. Technol. 29, 400–406. doi: 10.1016/s0141-0229(01)00401-x
Zhou, H., Luo, C., Fang, X., Xiang, Y., Wang, X., Zhang, R., et al. (2016). Loss of gltb inhibits biofilm formation and biocontrol efficiency of Bacillus subtilis Bs916 by altering the production of γ-polyglutamate and three lipopeptides. PLoS One 11:e0156247. doi: 10.1371/journal.pone.0156247
Keywords: Bacillus amyloliquefaciens, Bacillus velezensism, biocontrol, Plasmodiophora brassicae, rapeseed
Citation: Zhu M, He Y, Li Y, Ren T, Liu H, Huang J, Jiang D, Hsiang T and Zheng L (2020) Two New Biocontrol Agents Against Clubroot Caused by Plasmodiophora brassicae. Front. Microbiol. 10:3099. doi: 10.3389/fmicb.2019.03099
Received: 24 September 2019; Accepted: 20 December 2019;
Published: 21 January 2020.
Edited by:Calum Rae Wilson, University of Tasmania, Australia
Reviewed by:Georgios Tzelepis, Swedish University of Agricultural Sciences, Sweden
Bruce D. Gossen, Agriculture and Agri-Food Canada (AAFC), Canada
Copyright © 2020 Zhu, He, Li, Ren, Liu, Huang, Jiang, Hsiang and Zheng. 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: Lu Zheng, email@example.com