Genomic Identification of the TOR Signaling Pathway as a Target of the Plant Alkaloid Antofine in the Phytopathogen Fusarium graminearum

Fusarium head blight caused by the fungal pathogen Fusarium graminearum is a devastating disease of cereal crops worldwide, with limited effective chemical treatments available. Here we show that the natural alkaloid compound antofine can inhibit fusarium head blight in wheat. Using yeast genomic screening, we identified the TOR pathway component RRD2 as a target of antofine that is also required for F. graminearum pathogenicity.

which stimulates angiogenesis through the action of protein kinase B or AKT/mTOR signaling pathways, is inhibited by antofine via an unknown mechanism (5).
Antofine has also been shown to inhibit growth of a variety of microorganisms, including two strains of the phytopathogen Fusarium graminearum (6), which causes Fusarium head blight (FHB) disease in small-grain cereals, resulting in low-yield, lowquality, mycotoxin-contaminated grain, which poses a serious threat to food safety and the economy (7). Due to the ubiquitous global distribution of F. graminearum, most agronomic practices aimed at controlling FHB, including chemical control, offer only moderate control and do not eliminate the proliferation of the disease. Only a few active ingredients have been registered to suppress F. graminearum as a foliar or seed treatment in cereals (8). Most of these compounds belong to the triazole group of fungicides and include tebuconazole, triticonazole, difenoconazole, and ipconazole. The efficacy of these fungicides can vary between Fusarium species, and moreover, emergence of fungicide-resistant strains is compelling stakeholders to develop new strategies to combat FHB disease (9,10).
Although ubiquitous in eukaryotes, only recently has the TOR signaling pathway been documented to play a role in F. graminearum development and pathogenesis (11). Inhibition of TOR signaling by rapamycin, which binds Fkbp12 to inhibit Tor kinase and the downstream Tap42 protein phosphatase complex, reduces both vegetative growth and conidial germination, leading to reduced pathogenicity (11). In addition, two peptidyl-proly cis/trans-isomerases, RRD1 (FGSG_09229) and RRD2 (FGSG_01092), which regulate the activity of type 2A phosphatases of the TOR pathway and confer resistance to rapamycin when mutated (12), have overlapping functions in mycotoxin production and virulence, as well as growth and reproduction (13). However, the severity of growth defects and asexual spore production are more pronounced in the F. graminearum rrd2 (Fgrrd2) mutant than Fgrrd1 (13). In addition, FgRRD2, but not FgRRD1, modulates sensitivity to the phenylpyrrole fungicide fludioxonil and plays a dominant role in regulation of the high-osmolarity glycerol (HOG) pathway in F. graminearum (13).
In this report, we use yeast haploinsufficiency profiling (HIP) to identify potential targets of antofine. We show that RRD2 is a target of antofine in F. graminearum. Additionally, we show that binding of antofine to RRD2 leads to the disruption of the Tap42 phosphatase complex, providing a potential mechanism for disruption of the TOR signaling pathway.

RESULTS AND DISCUSSION
We purified antofine from Vincetoxicum to homogeneity as previously described (see Fig. S1A in the supplemental material) (6). After establishing a standard growth curve based on spore concentrations (Fig. S1B) and a linear relationship between mycelial growth and weight (Fig. S1C), we showed that antofine suppressed F. graminearum germination and growth in a dose-dependent manner with a 50% inhibitory concentration (IC 50 ) of ϳ100 g/ml (see Fig. S2A in the supplemental material). Tylophorine is structurally related to antofine, and both compounds display similar activities, including growth inhibition of many cancer cell lines by blocking S-phase transition and arresting HepG2, HONE-1, and NUCG-3 carcinoma cells at the G 1 phase (14). However, the suppression of F. graminearum germination and growth (as well as yeast growth [ Fig. 1B]) was specific to antofine, and we therefore used tylophorine as a biologically inactive negative control (Fig. 1A) (15). In addition to suppressing in vitro growth, antofine decreased FHB symptoms on wheat heads when coinoculated with F. graminearum spores (Fig. S2B). It should be noted that at the antofine concentrations tested, antofine alone did not produce any observable deleterious effects such as kernel weight (data not shown).
In order to identify potential targets of antofine, we used haploinsufficiency profiling (HIP) in yeast (16). HIP exploits drug-induced haploinsufficiency, as measured by growth defects resulting from deletion of one copy of a drug target gene, and has been used to identify the targets of small molecules, including fungicides (16). After establishing a sublethal concentration (2 g/ml) of antofine (see Fig. S3A in the supplemental material), we conducted an HIP screen on ϳ6,000 yeast heterozygous strains and identified three heterozygous strains that were hypersensitive to antofine. While wildtype (WT) yeast growth was inhibited by 2.5% at 2.0 g/ml of antofine (ϳ4 M), the 3 heterozygous mutants YOR375C, YBR095C, and YIL153W displayed 23, 15.5, and 12.5% growth inhibition, respectively (Fig. S3B). The Saccharomyces cerevisiae glutamate dehydrogenase gene (ScGDH1; YOR375C) has a homologue in F. graminearum (FGSG_07174) with 73% identity, and the ScRRD1 gene (resistant to rapamycin deletion 1; YIL153W) has two homologues in F. graminearum, FGSG_09229 (FgRRD1) and FGSG_01092 (FgRRD2), with identities of 38 and 32%, respectively (13). The third target identified in yeast YBR095C showed a weak homology (18% identity) with F. graminearum gene FGSG_08612, and the homology between these proteins was not contiguous. Therefore, we pursued FgGDH1, FgRRD1, and FgRRD2 for further characterization as putative targets of antofine. Note that both Scgdh1 and Scrrd1 mutant strains displayed no hypersensitivity to the negative-control tylophorine (Fig. 1B).
To determine if F. graminearum genes could complement yeast mutants, we ex- Antofine Targets the TOR Pathway in F. graminearum ® pressed FgRRD1 (FGSG_09229) and FgRRD2 (FGSG_01092) in the S. cerevisiae YIL153 mutant strain and expressed FgGDH1 (FGSG_07174) in the S. cerevisiae YOR375C mutant strain. FgGDH1 was able to partially complement the antofine sensitivity of the Scgdh1 mutant strain (Fig. 1C). Interestingly, FgRRD2 (P Ͻ 0.01) but not FgRRD1 was able to partially rescue antofine sensitivity in the Scrrd1 mutant strain and was therefore chosen for further analysis (Fig. 1C). To test if FgGDH1 and FgRRD2 are direct targets of antofine, both genes were cloned and expressed, and the purified protein (see Fig. S4 in the supplemental material) was used in thermal shift assays (TSAs) (17,18). TSA determines a shift in the melting temperature (T m ) of a protein upon binding to a ligand, measured by changes in light scattering or fluorescence. The T m of FgGDH shifted from 61°C to 62.4°C in the presence of 100 g/ml of antofine ( Fig. 1D; ϩA 100 ); however, in the presence of 100 g/ml of tylophorine, the T m did not shift relative to FgGDH alone ( Fig. 1D; T 100 ). The TSA also showed that the T m of purified FgRRD2 shifted from 51°C to 54°C ( Fig. 1D; A 100 ) and similar to FgGDH, the shift with tylophorine was negligible compared to that with the protein alone ( Fig. 1D; T 100 ). The TSA results indicate that antofine binds both FgGDH and FgRRD2 proteins.
Since antofine inhibited FHB symptoms on wheat ( Fig. S2B), we tested whether both antofine targets were associated with fusarium pathogenicity. We deleted GDH1 and RRD2 in F. graminearum and performed pathology tests on the susceptible wheat variety Roblin. The deletion of FgGDH1 did not affect the pathogenicity, suggesting that it is not the antofine target responsible for F. graminearum virulence (see Fig. S5A in the supplemental material). In contrast, targeted deletion of FgRRD2 significantly affected the virulence of F. graminearum (Fig. S5B). After 15 days postinfection (dpi), the entire wheat head was bleached after inoculation with wild-type F. graminearum spores ( Fig. S5B; Fg), while no such effect was visible after inoculation with the mutant strain ( Fig. S5B; Fg rrd2). It is likely that growth defects and its inability to produce the mycotoxin deoxynivalenol significantly contributes to the virulence defects (13). Overexpression of FgRRD2 in the Fgrrd2 mutant strain (Fgrrd1::OEFgRRD2) not only restored F. graminearum virulence ( Fig. S5b; Fg rrd2:OEFg RRD2) but also counteracted the effect of antofine (Fig. 2C). These results suggest that although antofine appears to have multiple targets, FgRRD2 is the target responsible for virulence inhibition in F. graminearum (13).
The haploid yeast rrd1 mutant and mutants of the two homologues in the F. graminearum strain PH1, Fgrrd1 and Fgrrd2, have been shown to be resistant to the inhibitory effects of rapamycin (12,13). We confirmed this phenotype for the Fgrrd2 mutant in our F. graminearum strain (DAOM 233423 [ Fig. 2]). Wild-type F. graminearum spores pretreated with rapamycin at 10 and 20 ng/ml decreased in growth by 50 and 80%, respectively, relative to untreated spores ( Fig. 2A; Fg Wt). However, no such growth inhibition was observed with the Fgrrd2 mutant strain exposed to rapamycin ( Fig. 2A; Fg rrd2). We therefore hypothesized that if antofine antagonizes RRD2, it should chemically phenocopy the rapamycin insensitivity of the Fgrrd2 mutant. In support of this, growth of wild-type F. graminearum spores was monitored in the presence of sublethal doses of antofine (50 and 100 g/ml [A 50 and A 100 , respectively]) and inhibitory concentrations of rapamycin (20 and 50 ng/ml [R 20 and R 50 , respectively]) (Fig. 2B). We observed that the inhibitory effects of rapamycin at both doses were suppressed by antofine at 50 g/ml (Fig. 2B). Antofine at 100 g/ml suppressed the inhibitory effect of rapamycin at the lower concentration (20 ng/ml) but not at the higher concentration (50 ng/ml), likely due to synergism between antofine and rapamycin toxicity at higher concentrations. Altogether, the results strongly support RRD2 as a direct target of antofine.
RRD is a component of the target of the rapamycin signaling pathway, which is evolutionarily conserved and important for cell growth in eukaryotes (19). In yeast, the rapamycin-sensitive Tor complex 1 (TORC1), in addition to promoting anabolic processes, leads to suppression of stress response pathways (20). This dual role makes this pathway an extremely important subject area of study since its disruption either through mutation or through chemical inhibition can influence numerous diseases, including cancer and diabetes (21). TORC1 mediates these pathways through regula-tion of a set of serine/threonine protein phosphatases, including Sit4, protein phosphatase 2A (PP2A), and Ppg1, which together form the phosphatase-associating protein Tap42 protein complex in a nutrient-and Tor-dependent manner (22). The current model suggests that TORC1 is associated with the Tap42-phosphatase complexes, and upon nutrient stress or rapamycin treatment, the Tap42-phosphatase complex is released from TORC1 (22). This event disassembles the Tap42-phosphatase complex, leading to the activation of the phosphatases and inhibition of Tor activity (19). Therefore, as a positive regulator of phosphatases, Tap42 represents an important regulator of the TOR signaling pathway.
In summary, we have identified targets of antofine in F. graminearum, one of which (RRD2) is crucial for pathogenicity in wheat. Our finding that the plant-derived compound antofine directly impacts the action of TOR signaling provides an additional tool to dissect this complex signaling pathway and a potential lead compound for integrative pest management programs in crop protection. In addition to rapamycin, other and FgPpg1 has been demonstrated previously and was used as a positive control (11). Shown is a representative of three independent biological replicates, each with three technical replicates.
inhibitors of the TOR pathway such as PP242, which acts as a competitive inhibitor for the ATP binding site of mammalian TOR, have been proposed for therapeutic use (24). More recently, PP242 was also used to inhibit the plant Tor kinase and reduce F. graminearum disease development in Arabidopsis (25). A similar increase in resistance to pathogens was observed when signaling from the TOR pathway was attenuated in Arabidopsis with a mutation in the Raptor gene, a direct target of the Tor kinase (26). However, the same study showed that manipulation of the TOR pathway could have unintended negative effects on plant growth, which presents an obvious hurdle to targeting this pathway for crop protection.
Large-scale fungicide use in agriculture is leading to emergence of multidrug resistance (MDR) in fungal strains, characterized by partial to complete resistance to fungicides (10). In this context, combinatorial drug application is one approach that can be used to combat MDR pathogens in agriculture. Such an approach is common in treating human diseases such as HIV and malaria and is also a strategy to combat deadly human fungal pathogens, such as Candida, Aspergillus, and Cryptococcus, and block the emergence of resistance (27,28). The latter study showed that the small molecule beauvericin increased efficacy of azole-derived compounds through the inhibition of a multidrug efflux pump and the TOR signaling pathway (28). Similarly, a checkerboard analysis between antofine and existing fungicides could reveal concentrations of antofine that are benign to humans but can increase the efficacy of other commonly used azole-derived fungicides used in agriculture (29).

MATERIALS AND METHODS
Purification and confirmation by NMR of antofine. Root tissues of Vincetoxium rossicum were harvested, vacuum desiccated, and crushed in EtOAc. The crude extract was filtered, concentrated by rotary evaporator, and dissolved in 0.01 M HCl. The pH was reduced to 2.0 with 1 M HCl and the solution partitioned with EtOAc. The organic fraction was concentrated by rotary evaporator and dried for storage. The pH of the aqueous fraction was increased to 10 with 1 M NH 4 OH and partitioned with EtOAc. The alkaline fraction containing antofine was concentrated by rotary evaporator, dissolved in pure acetonitrile (ACN), and injected into a 250-by 10-mm 5-m 120-Å C 18 reverse-phase semipreparatory column (ACE-121-2510; Advanced Chromatography Technologies). The column was preequilibrated in a gradient (5% ACN in water to 75% ACN in water) over 20 min at 10 ml/min. Antofine was eluted in 75% ACN-distilled water (dH 2 O) in 10-ml fractions for 20 min. An aliquot of 2 ml from each sample was dried using a SpeedVac (SVC-100H; Savant) and suspended in 200 l methanol (MeOH). A 10-l aliquot was spotted onto a sterile 6-mm filter disc. The discs were placed amended side down on petri dishes containing 2% YPD (yeast extract-peptone-dextrose) agar evenly spread with ϳ1.0 ϫ 10 6 CFU of S. cerevisiae BY4741 and incubated at 30°C overnight. The fractions that demonstrated an inhibition zone were pooled and dried using a rotary evaporator. The pellet was suspended in MeOH and spotted onto a glass-backed silica thin-layer chromatography (TLC) plate (5715-7; EMD Chemicals). Compounds were separated by TLC with two consecutive migrations of 60:40 EtOAc-MeOH and traced by illumination under shortwave (254-nm) UV light. Each band was scraped from the silica plate and recovered using MeOH. The MeOH was removed by rotary evaporator, and the recovered compounds were solubilized in CHCl 3 and tested for activity as described before. Purified antofine was subjected to 1 H nuclear magnetic resonance (NMR) for confirmation. The NMR spectrum was recorded on a Bruker Avance 400-MHz NMR spectrometer. The sample was recorded using CDCl 3 as the solvent, purchased from Cambridge Isotope Laboratories, Inc. The reference peak was set using the known residual solvent peak of CDCl 3 at 7.26 ppm. The NMR spectrum was compared to the known spectrum of antofine (30).
Identification of antofine targets in yeast by haploinsufficiency profiling. The Yeast Heterozygous Knock-Out collection (Open Biosystems; GE Healthcare, USA), along with the diploid wild-type strain (BY4743), was copied to solid 2% YPD agar amended with 150 g/ml G418, contained in an Omniwell plate (Nunc catalog no. 242811), using a 96-pin replicator (Nunc catalog no. 250520) and the OmniTray copier (Nunc catalog no. 250555) and incubated overnight at 30°C. The initial screen was initiated with antofine (0.75 g/ml) and incubated for 24 h at 30°C. The plates were scanned as a grayscale image (Epson Perfection V750 Pro) and processed with the Epson Scan version 3.24A scanning software at a 300-dpi resolution. The initial screen was repeated 6 times at antofine concentrations of 2.75, 2.5, 2.0, and 1.25 g/ml, with a final concentration of methanol at 0.01%. The results of the initial screens were analyzed together using the Screen Mill analysis package, and all mutants that received a P value of Ͻ0.05 were selected for further analysis (31).
Our initial screen yielded 873 potential candidates. To further narrow the list of candidates, we employed a liquid-based analysis. Briefly, each mutant was grown to an absorbance at 600 nm (ABS 600 ) of ϳ5.0, and 10 l of this new cell suspension was transferred to a new 96-well plate containing 190 l of YPD and bringing the cell density equivalent to an ABS 600 reading of 0.25 (ϳ5.0 ϫ 10 6 CFU/ml), supplemented with 0.20 g/ml of Antofine. The plate was then loaded into a BioTek Powerwave plate reader, for incubation at 30°C, and then the growth was assessed by ABS 600 every 10 min over the course of 48 h. The growth for each mutant (with antofine) was then compared to the average growth calculated for the WT (with antofine), by subtracting the calculated percentage of WT growth from the calculated percentage of growth for the mutant, where a positive result signified the mutant grew better than the WT under experimental conditions, and a negative result signified the mutant grew poorer than the WT when antofine was present. We used 10% as the cutoff for growth differences. This analysis yielded 16 mutants sensitive to antofine.
To confirm the observed effect of antofine, 16 antofine-sensitive mutants were further screened with three concentrations of antofine (2.5, 2, and 1.5 g/ml) in triplicate. This was repeated three times. After analysis, three yeast mutants (YBR095C, YOR375C, and YIL153W) showed a consistent sensitive phenotype to antofine.
ScreenMill analysis. The differences in colony growth were assessed by the ScreenMill growth measurement and analysis software suite (31). Briefly, each plate is scanned and then analyzed using the colony measurement engine, which detects each colony and assigns each a numerical value based upon its circularity and size. The file output is then input into the data review engine. A web-based application normalizes raw screen data and provides the user with an opportunity to manually select data for exclusion from analysis. The normalized data are used to calculate P values by t test for parametric data or the Mann-Whitney test for nonparametric data.
Construction of F. graminearum Fggdh1 and Fgrrd2 mutant strains and the Fgrrd2::OEFgRRD2 overexpression strain. F. graminearum wild-type strain DAOM 233423 (NRRL29169) was provided by C. Babcock of the Canadian Collection of Fungal Cultures (CCFC/DAOM), Agriculture and Agri-Food Canada, Ottawa. Macroconidia were used as the inoculum for all experiments and were produced in a liquid carboxymethyl cellulose medium (32). All of the plasmids were constructed by the USER (uracil-specific excision reagent) technique and outlined (see Fig. S7 in the supplemental material) (33). The deletion of FgGDH (FGSG_07174) and FgRRD2 (FGSG_01092) was performed by PCR amplification of the two homologous recombination sequences (HRSs) for each gene. HRS1 for FGSG_07174 was obtained with primer sets Fg 07174 USER Up-F/R, and HRS1 for FGSG_01092 was obtained with Fg 01092 USER Up-F/R. HRS2 for FGSG_07174 was obtained with primer sets Fg 07174 USER Dn-F/R, and HRS2 for FGSG_01092 was obtained with Fg 01092 USER Dn-F/R. PCR products HRS1 and HRS2 were introduced into the pRF-HU2 vector with hygromycin (Hyg) as the selection marker. The Fgrrd2::OEFgRRD2 overexpression strain was constructed by introducing FGSG_01092 cDNA into the pRF-GUE vector with Geneticin as the selection marker (Gen). The cDNA was amplified by the primer set Fg 01092 GUE_F/R. The F. graminearum mutants were screened for the presence and absence of FGSG_07174 and FGSG_01092 with primer sets Fg 07174 Orf F/R and Fg 01092 Orf F/R, respectively. The presence of the gpdA promoter in the Fgrrd1::OEFg RRD1strain was confirmed by the primer set Gpd Pro F and Fg 01092 Orf R. The sequences of the primers are listed in Table S1 in the supplemental material. Touchdown PCR conditions were used to confirm F. graminearum transgenic strains: 100 ng of genomic DNA for 8 cycles at 63 to 55°C and for 22 cycles at 55°C. We verified the copy number in the mutant strains by quantitative real-time PCR (qRT-PCR) analyses (Fig. S7G). Briefly, the analyses were performed with the primer set Fg 01092 qPCR F/R for FGSG_01092 and the primer set Fg 07174 F/R for FGSG_07174 and normalized with a known single-copy gene coding for glyceraldehyde-3-phosphate dehydrogenase, GAPDH (FGSG_16627), using the primer set Fg 16627 F/R (Table S1) (34). All samples were assessed in triplicate using the QuantStu-dio3 (Applied Biosystems, USA).
RNA extraction and cDNA library from F. graminearum. F. graminearum strains were grown in a mixture of 56 mM NH 4 Cl, 8.1 mM MgSO 4 ·7H 2 O, 0.23 mM FeSO 4 ·7H 2 O, 14.7 mM KH 2 PO 4 , 2 g/liter peptone, 2 g/liter yeast extract, 2 g/liter malt extract, and 111 mM glucose for 24 h, and total RNA was extracted from mycelia using TRIzol reagent (Invitrogen), purified using the InviTrap Spin cell RNA minikit (Stratec, Germany), and then converted into cDNA (1 g) using the Applied Biosystems high-capacity cDNA reverse transcription kit. RT-PCRs were similar to the touchdown PCR conditions mentioned before.
Growth curve assays with inhibitors. One thousand spores from F. graminearum wild-type (Wt), ΔFGSG 07174 and ΔFGSG 01092 mutant strains, and the Fgrrd2::OEFgRRD2strain were inoculated in 200 l GYEP medium (0.1% KH 2 PO 4 , 0.05% MgSO 4 ·7H 2 0, 0.05% KCl, 0.02% [vol/vol] trace element solution, and 0.01% sucrose). The spore germination assay was set up in 96-well microtiter plates (Corning 3632), and growth was monitored over a 48-h period at 600 nm using the FLUOstar Optima plate reader (BMG Labtech, USA) in a final volume of 200 l. We assessed the germination and growth of various numbers of spores (250, 500, and 1,000) by absorbance ( ϭ 600 nm) and visualization at numerous time points with a Zeiss AxioImager M2 microscope (Carl Zeiss Canada, Toronto, Ontario) (Fig. S1B). An absorbance reading of ϳ0.5 was the same for all the spore concentrations at 48 h. Therefore, we used 48 h as the endpoint measurement for all of the fusarium spore germination/growth assays. All yeast strains were grown overnight in YPD (yeast extract-peptone-dextrose) at 30°C with shaking at 200 rpm overnight. Cells were diluted to an ABS 600 of 0.5 and used in growth curve assays. The growth was monitored over a 24-h period at 600 nm using the FLUOstar Optima plate reader as described before. The inhibitors were dissolved in 100% methanol and were used at the indicated concentrations in a 1% final concentration of methanol in all of the liquid assays.
Purification of FgGDH (FGSG_07174) and FgRRD1 (FGSG_01092) from yeast. Both FGSG_07174 and FGSG_01092 were cloned into the pYES-DEST 52 Gateway destination plasmid vector by LR clonase reaction (Life Technology, USA). Plasmids were transformed into yeast knockout strains YOR375C and YIL153W, respectively. The complemented yeast was grown in 5 ml of Sabouraud dextrose (SD) medium lacking uracil in the presence of 2% glucose and antibiotic selection with G418 (Sigma) overnight at 30°C. Yeast cells were transferred in a 1:100 ratio to 30 ml of inducing medium with 2% galactose, 1% raffinose, and G418 overnight at 30°C. Yeast cells then were harvested by centrifugation at 2,700 ϫ g for 10 min. The resulting yeast pellet was processed for protein extraction. The His-tagged proteins were purified using the Clontech His-tagged purification miniprep kit. Yeast pellet containing the His-tagged protein was thawed in 1 ml X-tractor buffer, 100 l Zymolyase (5 U/l; G Biosciences), 40 l of 25ϫ Roche Complete mini-protease inhibitor cocktail, 10 l RNase A (20 mg/ml; Sigma), and 5 l DNase I (10 U/l; Agilent). The lysate was incubated at 37°C for 1 h and purified according to the manufacturer's instructions with modifications. Briefly, the total lysates were centrifuged at 15,000 rpm to get rid of the cellular debris, and the supernatant was loaded onto the affinity column. After washes with buffer (20 mM Tris [pH 8.0], 30 mM NaCl, 2 mM dithiothreitol [DTT], and protease inhibitor cocktail) containing 20 and 50 mM imidazole, proteins were eluted with buffer containing 500 mM imidazole. Eluates were dialyzed with buffer overnight at 4°C. Glycerol was added to a final concentration of 20%, and the mixture was stored at Ϫ20°C until use.
TSAs. Thermal shift assays (TSAs) were performed with purified FgGDH and FgRRD2 proteins. The TSA was performed in Quant Studio 3 (Applied Biosystems) with the Applied Biosystems protein thermal shift dye kit (4461146) in a 20-l reaction volume containing 1 mg/ml of each protein with or without antofine or tylophorine (Santa Cruz Biotechnologies, USA) at 100 g/ml (0.1% methanol). The PCR conditions were used according to the manufacturer's instructions, and data were analyzed with Protein Thermal Shift software version 1.3 (Thermo Fisher Scientific). Melting temperature (T m ) data were generated using the Boltzmann method. ΔT m was calculated by comparing the T m values for each protein without the inhibitors to those with the inhibitors. Data were collected at 1°C intervals from 25°C through 99°C and are shown in the replicate result plot view of the Protein Thermal Shift software.
Fusarium infection assay. Each strain was assessed for the ability to infect susceptible Triticum aestivum (cv. Roblin). Wheat heads (10 heads per strain) were point inoculated at mid-anthesis with each strain at 100,000 spores/ml in a volume of 10 l (1,000 spores). Spores were inoculated between the palea and lemma of a single wheat spikelet. Plants were grown at 25°C for 16-h days with misting every hour for 30 s. After 48 h, misting was reduced to a duration of 30 s every 4 h. Infection was scored by counting the number of visibly infected spikelets at days 5, 10, and 15 (32).
Yeast two-hybrid and ONPG assays. The coding sequences of FgTap42, FgRRD2, FgTip41, FgPp2A, and FgPpg1 from F. graminearum were synthesized and cloned into the pDONR vector (General Biosystems, Morrisville, NC). The genes were subcloned into the yeast vectors pJG4-5 (activation domain B42) and pEG202 (DNA binding domain LexA) by Gateway LR Clonase II reaction (Thermo Fisher Scientific). Yeast two-hybrid plasmid pairs were transformed into S. cerevisiae strains RFY206 and EGY48, before mating and selection on synthetic medium lacking histidine, uracil, and tryptophan. Two independent yeast colonies containing both pJG4-5 and pEG202 for each gene pair were selected for interaction, and the interaction was quantified by a ␤-galactosidase activity assay with ONPG (23). Interaction was monitored in the presence of either antofine or tylophorine (0, 0.1, and 1 g/ml). Three independent experiments were performed, using corresponding empty vectors as negative controls. All the yeast strains were grown as described before in the purification of FgGDH1 and FgRRD1, except the induction with galactose was limited to 1 h. To ensure that expressed proteins were not affected by antofine, extracts from noninduced and induced cultures (Ϯantofine or tylophorine) were subjected to Western blot analyses. Proteins were extracted by 2 M LiAc and 0.4 M NaOH followed by boiling in Laemmli buffer. Twenty micrograms of protein from each sample was separated on a 10% SDS-PAGE gel, and the blots were probed with LexA antibodies for detection of FgTap42 (Millipore Sigma, USA) and hemagglutinin (HA) antibodies (Roche, Germany) to detect both FgRRD2 and FgPpg1 proteins. Proteins were detected by the ECL enhanced chemiluminescence substrate (Lumigen ECL Ultra; TMA-6).