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The majority of plant growth promoting rhizobacteria (PGPR) confer plant immunity against a wide range of foliar diseases by activating plant defences that reduce a plant’s susceptibility to pathogen attack. Here we show that Arabidopsis thaliana (Col-0) plants exposed to Bacillus subtilis strain FB17 (hereafter FB17), results in reduced disease severity against Pseudomonas syringae pv. tomato DC3000 (hereafter DC3000) compared to plants without FB17 treatment. Exogenous application of the B. subtilis derived elicitor, acetoin (3-hydroxy-2-butanone), was found to trigger induced systemic resistance (ISR) and protect plants against DC3000 pathogenesis. Moreover, B. subtilis acetoin biosynthetic mutants that emitted reduced levels of acetoin conferred reduced protection to A. thaliana against pathogen infection. Further analysis using FB17 and defense-compromised mutants of A. thaliana indicated that resistance to DC3000 occurs via NPR1 and requires salicylic acid (SA)/ethylene (ET) whereas jasmonic acid (JA) is not essential. This study provides new insight into the role of rhizo-bacterial volatile components as elicitors of defense responses in plants.
Plants are constantly challenged by a plethora of disease causing microorganisms.1,2 To counter the onslaught of infections by microorganisms, plants have evolved a combination of constitutive and inducible defense responses.3,4 Induction of programmed cell death at the site of infection is a mechanism known as hypersensitive response (HR), while induction of defenses triggered throughout the plant is referred to as systemically induced resistance.5 The mechanism of induction for HR is highly sophisticated and occurs as a result of gene for gene interactions between plant encoded resistance (R) genes and corresponding pathogen encoded avirulence (Avr) genes. The induction of SAR leads to enhanced resistance in distal parts of the plant against further attack by the same or a different pathogen.6 This increase in systemic resistance occurs by two common pathways. These two pathways involve mediation by the plant hormones salicylic acid (SA) and JA. SA and JA defense responses are known to reduce the natural bacterial diversity on A. thaliana.7,8 Some of the SA analogs such as BTH (benzo(1,2,3) thiadiazole-7-carbothioic acid S-methyl ester) and INA (dichloroisonicotinic acid) also are known to elicit SAR.9 Further SA is known to signal the expression of a number of pathogenesis related proteins (PRs) like PR-1, PR-2 and PR-5 in Arabidopsis thaliana and Nicotiana tabacum plants.10 Studies involving genome wide transcript analysis of A. thaliana have revealed other genes, in addition to the known PRs likely to function in SAR.11
A number of biocontrol bacteria, also known as plant growth promoting rhizobacteria (PGPR), protect plants from soil-borne pathogens by antagonistic mechanisms.12,13 Such bacteria colonizing on the roots can also induce systemic resistance in aerial plant parts, which are spatially separated from the inducing PGPR. The protection by such a mechanism typically is manifested by reduction in the pathogen growth and is phenotypically similar to the pathogen induced SAR.14 This mechanism of induction of systemic resistance by root colonizing rhizobacteria in aerial plant parts is referred to as induced systemic resistance (ISR).
There are reports describing ISR elicitation by various Gramnegative Pseudomonas spp and Gram positive biocontrol PGPR Bacillus spp.15–21 A. thaliana plants treated with PGPR Serratia marcescens strain 90–166 and B. pumilis strain SE34 showed reduced disease severity and symptom development against Cucumber mosaic virus (CMV).14 B. subtilis, found ubiquitously in the soil, has been reported to promote plant growth and protect plants against fungal infection,14,22–27 apart from inducing ISR.14 The induction of ISR when treated with PGPRs has been shown to be mediated primarily through plant signaling molecules such as JA and ethylene (ET).14,16
In addition to B. subtilis biocontrol against soil borne fungal pathogens, B. subtilis systemically protect A. thaliana against cucumber mosaic virus by SA and NPR1 independent and JA dependent mechanisms.14 However, its biocontrol effect against A. thaliana root infection by P. syringae was attributed to its ability to form biofilms and to produce surfactin.12 Few bacterial volatile components are reported to induce systemic resistance in plants against various pathogens,28 although, it has been observed that bacterial volatile components (acetoin or 3-hydroxy-2-butanone) can serve as agents for triggering growth promotion in A. thaliana.27 Additionally, it was also demonstrated that a volatile compound, 2,3-butanediol which is structurally similar to acetoin produced by Bacillus amyloliquefaciens IN937a and Bacillus subtilis GB03 elicited an ISR in Arabidopsis.27 Plant components containing a six carbon backbone, e.g., (E)-2-hexenal, which is rapidly emitted from damaged plant tissue, has also been shown to induce the expression of defense-related genes in intact plants.29,30 In addition, a defensive role for terpenes as volatile elicitors has been proposed in excised lima bean (Phaseolus lunatus) plants.29 A recent study, from our group, showed that DC3000 infected shoots relay chemical signal(s) underground through root secretions. The root-secreted chemical specifically attracts and enhances FB17 root binding and biofilm formation on the infected seedlings.31 Although various groups have shown the mechanisms of B. subtilis biocontrol of root infections, the studies on the effect of B. subtilis induced ISR on aerial bacterial pathogenic infections are limited. Most of the reports relating to airborne signals inducing ISR are performed in isolation with respect to the biocontrol agent and the aerial pathogen. In this study, we report that root colonized B. subtilis (FB17) triggers acetoin induced ISR in the aerial parts. Further, ISR restricts pathogen multiplication and disease progression through a SA/ET and NPR1 dependent mechanism.
To increase the understanding of the biological significance of FB17 root binding during aerial infection, we examined this symbiotic interaction in actual disease resistance. The FB17 root-colonized plant leaves, inoculated with DC3000, showed a reduced symptom development in terms of formation of water soaked lesions compared to controls with no FB17 root inoculation at 5 days post infection (Fig. 1A). Further, a reduction in pathogen multiplication, as shown by a reduced number of colony forming units (CFU) counts of DC3000 in the inoculated leaves was observed in plants co-treated with FB17 (F(4,25) = 312.6, p < 0.05) compared to plants infected only with DC3000 (Fig. 1B).
We examined whether the elicitation of defense pathways can be mediated by a bacterial volatile organic compound that protects plants from DC3000 infection. In this experiment, we included acetoin in the magenta boxes in which A. thaliana plants were grown. Interestingly, the plants subjected to volatile treatment developed much lower disease symptoms when compared to untreated controls (Fig. 2A). Significantly lower DC3000 CFUs (p < 0.05, t-test) were recorded from the leaves of the plants subjected to acetoin treatment (Fig. 2B). Since DC3000 was not susceptible to direct antimicrobial acetoin (1 ml of 10 mM stock ~88 µg) treatments from broth micro-dilution assays (Suppl. Fig. 1), acetoin appears to be effectively activating plant defenses against aerially infected DC3000.
To further probe the role of acetoin in induction of ISR in A. thaliana against DC3000 infections, we employed B. subtilis strains (BSIP1173 and BSIP1174) impaired in production of acetoin.32 The genotypes of both acetoin nonproducing strains (BSIP1173 and BSIP1174) were trpC2 alsS::alsS-lacZ2 cat and trpC2 alsS::alsS-lacZ cat pta::aphA3 respectively.32 The insertional inactivation of the als operon (BSIP1173) and double mutant (als and pta) (strain BSIP1174), lead to abolishment in acetoin production.32 The mutant and overexpressing strain (BSIP1171) (genotype: trpC2 pta::aphA3) were tested and compared against wild type strains BS168 (parental strain), GB03 and FB17 for their effect on DC3000 infection in A. thaliana. All of the wild type and mutant strains, including the overexpressing strain BSIP1171, showed similar root colonization on aerially infected DC3000 A. thaliana Col-0 plants (Fig. 3A and B) but the acetoin mutant strains (BSIP1173 and BSIP1174) failed to protect the plants from DC3000 infection (Fig. 3A). A significantly higher symptom development (Fig. 3A), percent disease incidence (F(6,43) = 153.1, p < 0.05) (Fig. 3C) and DC3000 CFUs (F(6,43) = 125.3, p < 0.05) (Fig. 3D) were recorded from the plant roots that were inoculated with acetoin biosynthetic mutant strains compared to the plant roots inoculated with wild type B. subtilis strains (Fig. 3A, C and D). In summary, our data shows that acetoin released from the B. subtilis augments plant defense against aerial DC3000 infections. We also show that acetoin is not important for the root binding phenotype as the acetoin mutant biofilms were indistinguishable from the parental wild type strains31,33 (Fig. 3A).
Interestingly, a precursor of acetoin, 2,3-butanediol did not protect plants against DC3000 infections. We used previously established in vitro infection protocol,59 which relies on the degradation of chlorophyll florescence with the DC3000 inflicted disease progression as well as measuring bacterial growth through determining colony forming units per gram of fresh weigh of the seedlings. The A. thaliana plants treated with 2,3 butanediol and infected with DC3000 showed similar loss of red fluorescence (indicative of chlorophyll loss) compared to the lone DC3000 treatments (Suppl. Fig. 2). The results were interpreted using micrographs correlated well with the pathogen multiplication data set, wherein, plants treated with 2,3 butanediol and infected with DC3000 showed similar trends of pathogen multiplication compared to the lone DC3000 treatments (Suppl. Fig. 2). These results suggest the importance of acetoin but not its precursor 2,3 butanediol, in disease protection in A. thaliana against DC3000 pathogenesis.
To determine the involvement of SA and ET/JA pathways mediated by FB17, we employed a SA deficient A. thaliana line (NahG) and ET/JA (etr1-3, jar1-1) A. thaliana signaling mutants treated with FB17 and infected with DC3000. Little difference was observed between the B. subtilis root inoculated and un-inoculated NahG plants in terms of disease symptom development (Suppl. Fig. 3), and DC3000 CFUs from inoculated leaves (Fig. 4A). In contrast, a JA component mutant jar1-1 showed reduced DC3000 CFU (F(2,19) = 231.2, p < 0.05) and disease symptoms indicative of chlorosis post FB17 treatment (Suppl. Fig. 3; Fig. 4A). The ET pathway compromised mutant, etr1-3 revealed a similar phenotype as shown previously with NahG plants, indicating no enhanced disease resistance post FB17 treatment and DC3000 infection (Suppl. Fig. 3; Fig. 4A). Together, these data suggest that B. subtilis FB17 induced systemic resistance is NPR-1 dependent and requires SA and ET.
Further, to test whether acetoin also requires NPR1, SA and ET components to induce resistance against DC3000, infections were carried out a similar experiment as described earlier for FB17 except that the FB17 was replaced with acetoin treatment. The results presented in Supplementary Figure 3 show that acetoin failed to protect SA deficient NahG and ethylene mutant etr1-3 plants from DC3000 infection, whereas a significant reduction in DC3000 multiplication in terms of CFUs (F(2,29) = 231.2, p < 0.05) was observed with wild type Col-0 and JA mutant jar1-1 (Fig. 4B). These results correlated well with the earlier results with FB17 treatment and indicated that the B. subtilis derived-acetoin functions through NPR1-dependent pathway and required SA and ET components to induce resistance against DC3000 infections.
Our previous studies showed a higher PR1::GUS expression in plants that were root inoculated with FB17 compared to control untreated plants.31 The PR1::GUS expression was higher in the aerial parts compared to the root system in the FB17 treated plants. A. thaliana leaves sprayed with SA also showed higher PR1 expression while the root treated plants showed much less PR1 expression.31 As our results show that acetoin treated A. thaliana plants displayed enhanced resistance against DC3000, we examined whether acetoin induced expression of key defense genes. Further, PR1::GUS plants with acetoin showed enhanced PR1 expression compared to the untreated plants. Acetoin treated A. thaliana plants also revealed PR1 expression patterns similar to FB17 treatments (data not shown). Our data with the disease compromised mutants showed that FB17 mediated ISR, against DC3000, is NPR1-dependent and requires ET/SA. Further, we estimated the free SA levels, and our results showed significantly (F(8,55) = 175.2, p = 0.05) higher SA levels in the leaves of the plants that were root inoculated with FB17 compared to the control untreated plants (Suppl. Fig. 4A). Negative controls such as plant roots treated with other rhizobacteria P. aeruginosa (PAO1) and Pfo-1 showed no induction in free SA levels (Suppl. Fig. 4A). Interestingly, acetoin treatment also enhances the total free SA level (F(2,19) = 131.2, p < 0.05) in A. thaliana plants (Suppl. Fig. 4B).
To further confirm that a FB17 component, acetoin, mediates this response, we analyzed the defense genes PDF1.2 and Jin1 whose expression depends on functional ET and JA pathways. Our RT-PCR data shows that acetoin and FB17 treated A. thaliana plants express more PDF1.2 and PR1 transcripts but not Jin1 in leaves compared to the mock inoculated plants (Fig. 5A and B). Surprisingly, our results negated PDF1.2 and PR1 transcript expression in roots under FB17 treatments (Fig. 5). Further, co-inoculations of DC3000 with B. subtilis acetoin biosynthetic mutants (BSIP1173 and BSIP1174) also showed similar results confirming the role of NPR-1 (Suppl. Fig. 5). These results establish the involvement of this FB17 derived volatile component in mediating defense responses against DC3000 through NPR1 and ET dependent pathways by triggering PR1 and PDF1.2 expressions.
Different rhizobacterial strains including B. subtilis have been previously reported to protect plants against a number of pathogens including viruses.14,20,27,34–38 Our recent results showed that A. thaliana plants specifically recruit B. subtilis when experiencing an aerial pathogen attack from DC3000.31 These results revealed for the first time that the inducible plant responses triggered by DC3000 pathogenesis include the induction of root secretions that effectively recruit B. subtilis in the rhizosphere.31 In this study, root inoculation of A. thaliana with B. subtilis FB17 strain was found to stimulate plant defense pathways, though the elicitation profile of the genes involved was different from that previously reported using other rhizobacteria and biocontrol agents. It has been reported that B. subtilis root colonization protects plants against cucumber mosaic virus by a SA and NPR1 independent mechanism.14,27 Our analysis using FB17 and defense-compromised mutants of A. thaliana indicated that the resistance to DC3000 occurred via NPR1 and required SA/ET, whereas the Jar-1 was not essential. Although there are numerous examples of microorganisms interacting to trigger salubrious plant responses or a deleterious outcome, few reports have probed the role microbial VOCs may play in triggering biochemical changes of either primary or secondary plant metabolism. Results presented here indicate that a volatile bacterial component has the potential to induce systemic resistance in A. thaliana against DC3000 pathogenesis.
An important hallmark of the induction of systemic resistance is PR gene expression and the induction is signaled by the elevated levels of SA accumulated in the tissue showing systemic resistance.39 Exogenous application of SA has been reported to induce systemic resistance and PR gene expression.39–41 Our results with the defense compromised mutants show that resistance to DC3000 mediated by FB17, occurred primarily through the NPR1 pathway and required SA and ET components. Both npr1-1 and NahG plants treated with FB17 negated any enhanced resistance against DC3000 pathogenesis. NahG mutants are unable to accumulate SA because the incorporated gene product salicylate hydroxylase converts SA to the inactive form catechol and, therefore, are unable to induce PR-1.41 Similar results were obtained with the ET compromised mutant, etr1-3, which also showed no disease resistance against DC3000 post FB17 treatment. Interestingly, FB17 treatment of wild type A. thaliana plants induced accumulation of SA along with PR1 expression. Although our results indicate that resistance against DC3000 mediated by FB17 is NPR1 dependent and requires SA. Other PGPR strains such as P. fluorescens WCS417r reduced both the growth and symptom development by P. syringae in the leaves of A. thaliana upon root inoculation.42 However, in this case the ISR was independent of SA accumulation and PR gene expression,43 indicating that the mechanism to induce ISR is pathogen and PGPR strain specific. A recent study shows that a mixed inoculum treatment of B. subtilis and B. amyloliquefaciens triggers ISR through a SA dependent pathway against DC3000.43 Further, understanding of the mechanisms of translation of ISR by B. subtilis into a real benefit for plants in terms of disease resistance could be an interesting aspect.
Our in vivo pathogenicity assay results showed a significantly reduced disease incidence, symptom development and DC3000 multiplication in the leaves of B. subtilis root colonized plants. The data mainly indicated that this protection is brought about by the reduced proliferation of the pathogen in the inoculated leaves of the B. subtilis root inoculated plants. This was supported by the significantly lower DC3000 CFUs per gram fresh weight of the inoculated leaves in the case of B. subtilis treated plants. However, like previous studies42,43–48 and our study, the introduction of B. subtilis and challenging plants with P. syringae are spatially separated. This ruled out the possibility of direct effect of acetoin on DC3000 by contact, and demonstrated that the effect was plant mediated. Additionally, exposing the plants uniformly with acetoin also ensured that the effect was systemic and not local. Although, previous studies showed a successful protection of plants from root fungal infections49,50 and aerial feeding by beetles46 no effort has been made to study the effect of B. subtilis induced ISR on the aerial bacterial infections in A. thaliana.
Previously, it was shown by Ryu et al.14 that a volatile blend from B. subtilis GB03 and B. amyloliquefaciens IN937a was able to induce ISR in A. thaliana and reduce the disease severity of Pectobacterium carotovorum (formerly called as Erwinia carotovora subsp. Carotovora). The involvement of the B. subtilis volatile metabolite, acetoin, in the induction of systemic resistance was again confirmed in our study by treating the plants with acetoin. Interestingly, acetoin treatment triggered PR1 expressions and SA accumulation in A. thaliana plants. Acetoin treated A. thaliana plants revealed increased expressions for PDF1.2, suggesting that this compound targets SAR and ET pathways to upregulate defense responses in A. thaliana. These results also overlap with our defense compromised mutants study, wherein etr1-3, npr1-1 and NahG plants revealed no difference in disease symptoms and DC3000 CFUs between FB17 treated and untreated samples. Other metabolites such as surfactin and fengycin lipopeptides produced by B. subtilis strains induced systemic resistance in bean and tomato plants apart from activating the key enzymes of the lipoxygenase pathway in the resistant plants.48 However the results with B. subtilis acetoin biosynthetic mutant strains which did not induce ISR compared to the control wild type strains, confirmed the involvement of acetoin in inducing ISR against DC3000. Higher bacterial multiplication and symptom development was observed in the case of the plants treated with acetoin biosynthetic mutants compared to plants treated with wild type strains FB17, GB03 and parental strain of the mutants BS168. However, the higher efficiency of FB17 observed in terms of ISR induction also indicates that there are might be additional mechanisms specific to FB17 compared to other strains such as GB03. These observations conclusively established the involvement of an exometabolite volatile (acetoin) in mediating disease protection in plants against P. syringae. However, the question related to involvement of a plant component that triggers acetoin biosynthesis in B. subtilis remains unanswered. There is a tempting possibility that root secretions may play a definite role in chemotaxis and elicitation of acetoin biosynthesis in B. subtilis. Our future line of studies in this direction will investigate the role of root exudates on induction of acetoin metabolism in B. subtilis. Some of the common plant metabolites such as organic acids, especially oxaloacetate, trigger the alsSD operon, required for acetoin production.53
Although our results strongly suggest that the acetoin induced ISR restricts pathogen multiplication and disease development, the obvious question is whether this response was specific to B. subtilis? We addressed this question by employing another PGPR strain P. fluorescens (Pf01).42 Interestingly, Pf01 root inoculated plants failed to show protection against DC3000 infection. In contrast, previous studies have reported that other P. fluorescens strains such as WCS417r induce ISR against P. syringae in A. thaliana.42 These results suggest that few strains of P. fluorescens induce ISR against P. syringae also suggesting that the plant protection inflicted by this bacterial species is strain specific in nature.
In conclusion, our data show that protection of A. thaliana against DC3000 by a plant growth-promoting rhizobacterium follows a pathway that is dependent on NPR1 and requires SA and ET components but is independent of JA. Further confirmation was provided that FB17 derived VOC acetoin, induces the PDF1.2 and PR1 genes as a component of ET and SA signaling pathways, respectively. Evidence for SA-dependent but NPR1-independent pathways for regulation of PR1 gene expression and resistance to bacterial pathogens have been reported previously51–55 and we conclude that in our system a resistance, involving NPR1-SA dependent pathway is operational with the FB17 association. Although it was shown previously that the B. subtilis volatiles trigger an ISR response in A. thaliana through an ET dependent pathway against Erwinia pathogenesis,14 the involvement of SA and ET pathways together to trigger ISR is not very commonly seen in plants. The ability to prime the plant for an augmented response to pathogen attack is expected to confer a fitness advantage56 to the rhizobacterial-treated plants. This capacity to induce disease resistance in a versatile manner is expected to work in concert with their proven antibiotic effects and their colonization efficiency, making these rhizobacteria excellent candidates for effective biocontrol agents.
A. thaliana wild type cultivar Columbia (Col-0) seeds were procured from Lehle Seeds (Round Rock, TX, and USA). The A. thaliana lines npr1-1, etr1-3, jar1-1 and NahG plants were obtained from Arabidopsis Biological Resource Center (ABRC), Ohio State University, Columbus, OH 43210 USA. Acetoin was obtained from Sigma-Aldrich, USA. Seeds were washed in double distilled water three times and surface sterilized using 50% commercial bleach (sodium hypochlorite) for 3–5 min followed by 3–4 washes in sterile distilled water. Seeds were cultured on Murashige and Skoog’s57 (MS) solid medium with 3% sucrose and, allowed to germinate for 3–4 days at 23 ± 2°C 16 hr light/8 hr dark photoperiod until the roots and shoots emerged. The plates were illuminated with cool white fluorescent light with an intensity of 24 µmol m−2 s−1.
The strains of PGPR B. subtilis FB17 (obtained from Dr. Ray Fall, University of Colorado, Boulder), BS168, GBO3, BSIP1171, BSIP1173, BSIP1174 (from Dr. Paul Paré, Department of Chemistry and Biochemistry, Texas Tech University, Lubbock, TX 79409) were maintained on LB plates and P. fluorescens Pf01 and P. aeruginosa (PAO1) (obtained from Dr. George O’Toole, Department of Microbiology and Immunology Dartmouth Medical School, Hanover, NH 03755-3842). P. syringae DC3000 and E. coli (OP50) (obtained from Dr. Jorge M. Vivanco, Colorado State University, Fort Collins, CO 80523-1173) were maintained on LB plates with 50 µg ml−1 rifampicin. A single colony from a freshly streaked plate with or without antibiotic selection of each of the cultures was used to grow overnight cultures from which approximately OD600 = 0.02–0.05 culture was prepared and used in all the experiments. For routine plant based studies, cells were grown in LB medium at 37°C with shaking set at 220 rpm.
A. thaliana Col-0 plants grown on peat pellets in a growth chamber set for a photoperiod of 16 hr light and 8 hr dark at 23 ± 2°C and illuminated with cool white fluorescent light with an intensity of 24 µmol m−2 s−1 for a twenty day period. The plants were root inoculated with FB17 (OD600 = 0.5) by drenching with 10 ml of the culture in water. Fully expanded leaves were pressure inoculated with 100 µl of OD600 = 0.02 culture of P. syringae the next day. Different treatments included control (without DC3000 infiltration), control root inoculated with FB17, mock (leaf inoculated with sterile water), DC3000 (only leaf infiltration), DC3000 + FB17 (DC3000 leaf infiltration of FB17 root inoculated plants). The plants were transferred to magenta boxes and incubated in the growth chamber for an additional four days. The experiment was terminated after four days and the observations such as disease incidence (percentage of chlorotic leaves per plant), number of colony forming units per gram fresh weight of the leaf were recorded. Leaf samples were also collected and fixed for imaging the bacterial multiplication. Further, the co-cultivated roots were collected and fixed in 4% para-formaldehyde to image for B. subtilis binding and biofilm formation. Similar experiments using disease compromised A. thaliana mutants were carried out for FB17 treatment and DC3000 infections. Each treatment had at least 6 biological replicates and the experiment was repeated at two independent occasions.
Free SA content, in the leaves of plant roots inoculated with or without FB17 and also with or without leaf infiltration with DC3000, was estimated by following a modified protocol from Scott et al.58 Briefly, leaf tissues (up to 0.1 g) were finely ground in liquid N2 and extracted overnight at 4°C in 5 ml 80% methanol. Samples were air dried at 25°C and re-dissolved in 10 ml of 0.2 M sodium acetate buffer (pH 4.5) and centrifuged (13,000 rpm, 5 min). After sample centrifugation, the supernatant was collected and the pH was adjusted to pH 2.0 with 0.1 M HCl and extracted with equal volume of ethyl acetate. The organic phase was back-washed against H2O and evaporated to dryness at 25°C. Samples were re-dissolved in 500 µl of methanol. The samples were analyzed by injecting 30 µl of the extract in to a Dynex Acclaim®, Polar Advantage II, C18 column (5 µm, 120 A°, 4.6 × 150 mm) and separated using a 0% to 100% gradient of methanol in 2 mM formic acid over 60 min. at a flow rate of 1 ml min−1 on a Dynex liquid chromatograph. The total free salicylic acid level was calculated by comparing the peak area from a known concentration of standard SA and the unknown sample. Final data was calculated and expressed as µM of SA per gram fresh weight. Free SA was also estimated with other bacterial root treatments such as Pf0-1, PAO1 and OP50 similar to the above-mentioned protocol. Free SA estimation of acetoin treated plants was performed post-exposure of plants to acetoin (1 ml of 10 mM stock). Each treatment had at least 6 biological replicates and the experiment was repeated at two independent occasions.
All of the conditions for this experiment were similar to the above described, except that the additional treatments of root inoculation of Col-0 plants with wild type B. subtilis strains GBO3, FB17, BS168 and acetoin mutants BSIP1173 and BSIP 1174 were included. A separate set of treatments with acetoin as a volatile was generated by placing acetoin (1 ml of 10 mM stock) in a vial in the corner of the magenta box (Dimensions: 3 × 3 × 4″, growing area of 6.125 sq. inches Plantmedia Co.,) containing the plants with or without leaf infiltration by P. syringae was also set up and made airtight by sealing the cap with four coats of parafilm. All of the observations that were recorded for the earlier experiment were also recorded for this experiment. Each treatment had at least 6 biological replicates and the experiment was repeated at two independent occasions.
We used a previously established protocol59 to analyze the effect of 2,3 butanediol in inflicting resistance against DC3000 in A. thaliana seedlings. The assays were performed in liquid media, wherein surface-sterilized A. thaliana (Col-0) seedlings (5 days old) were suspended in 24 well plates containing MS (1%) media supplemented with 2.5 mm 2-(N-morpholino) ethanesulfonic acid (MES), pH 5.8 (Sigma-Aldrich). Five-day-old seedlings were inoculated with P. syringae DC3000 at a final concentration of 1 × 107 CFU ml−1 (OD600 = 0.02). A total volume of 1 ml of 10 mM 2,3 butanediol was then added to the last column of a 96 well plate where the plants were placed in the first four columns for volatile treated plates (1 ml of ddH2O was added to control plates). Plates were continuously stirred at 80 rpm under continuous light at 22–25°C in a controlled environment room. Seedling phenotypes were assessed at 1–4 days post-inoculation using stereo microscope (Zeiss Axioskop-2), wherein, chlorophyll degradation with loss of red fluorescence was used as an indicator of DC3000 disease progression. To enumerate bacterial populations in inoculated seedlings in the liquid assay, seedlings were removed, rinsed for 20 seconds in 70% ethanol and were homogenized in 100 µl of ddH2O. After homogenization, tube volume was brought to 1 ml and bacteria were quantified by serial dilution plating.
The effect of acetoin on P. syringae was studied by microdilution assay plates where 100 µl culture (OD600 = 0.02) was included into each well in alternative rows and every alternative row contained 100 µl acetoin (10 mM). The control plate received a similar quantity of culture and alternate rows received 100 µl of sterile water. The plates were incubated at 30°C on a rotary shaker. The OD600 was recorded in a plate reader at regular intervals up to 24 h. Each treatment had at least 6 biological replicates and the experiment was repeated at two independent occasions.
All of the conditions for this experiment were the same as the experiments described above except that the plants were root inoculated with P. fluorescens Pf01 (OD600 = 0.5) by drenching with 10 ml of the culture in water. All the observations that were recorded for the earlier experiment were also recorded for this experiment. Each treatment had at least 6 biological replicates and the experiment was repeated at two independent occasions.
Total RNA was extracted from leaves and roots of wild type plants after 12 h with or without FB17 treatment using RNeasy Plant Mini Kit (Qiagen, USA) according to the manufacturer’s instructions. cDNAs were synthesized from 300 ng of total RNA by using oligo dT primer (Ambion, Austin, TX) and Omniscript kit (Qiagen) according to manufacturer’s instruction. PCR amplification was carried out using oligonucleotide primers specific to A. thaliana Actin-2 (obtained from Sigma, USA Cat # C3615- 1SET) and PR1 (F = 5′ AGG TGC TCT TGT TCT TCC CTC GAA 3′; Reverse = 5′ TAC ACC TCA CTT TGG CAC ATC CGA 3′), PDF1.2 (F = 5′ GCT GCT CTT GTT CTC TTT GCT GCT 3′ Reverse = 5′ GGG ACG TAA CAG ATA CAC TTG TGT GC 3′) and Jin1 (F = 5′ ATG ACC CGA TTG GAA CAC CTG GAT 3′ Reverse = 5′ TGT CTC TCT GCT TCG ACG TGG TTT 3′) respectively. The PCR program used is as follows: denature at 95°C for 30 sec, anneal at 55°C for 20 sec, with an extension at 72°C for 1 min and a final extension at 72°C for 5 min.
In order to view adherent FB17 cells and biofilm on the root surface by laser scanning confocal microscopy, the roots were stained with SYTO®13 (Invitrogen, Molecular Probes, Eugene, OR). Images were captured with a 10X Plan-Apochromat objective (numerical aperture 0.45) or 40X C-Apochromat objective (numerical aperture 1.2) on a Zeiss LSM 510 NLO attached to an Axiovert 200M with Zeiss AIM software (Rel. 3.2). Images were acquired with the 488 nm line excitation of an Argon laser using a 505 nm long pass emission filter. Experiments were performed 24 hours post-inoculation and post-treatment with FB17 (5 µl culture of OD600 = 0.02) to 10 day old plants grown in 4 ml liquid MS medium with 1% sucrose. All experiments were repeated twice with three replicates each.
All of the data were averaged from two separate experiments unless mentioned otherwise and further analyzed for variance followed by a Student’s t test and ANOVA with the Benjamini-Hochberg correction60 for multiple testing when necessary using a statistical package JMP®7.0. The data means were considered significantly different at the probability of p ≤ 0.05.
H.P.B. acknowledges the support from University of Delaware Research Foundation (UDRF) and NSF Award IOS-0814477. P.W.P. acknowledges the partial financial support from Welch Foundation (Grant D-1478).
Previously published online: www.landesbioscience.com/journals/cib/article/10584