- Research article
- Open Access
Jasmonate and ethylene dependent defence gene expression and suppression of fungal virulence factors: two essential mechanisms of Fusarium head blight resistance in wheat?
BMC Genomics volume 13, Article number: 369 (2012)
Fusarium head blight (FHB) caused by Fusarium species like F. graminearum is a devastating disease of wheat (Triticum aestivum) worldwide. Mycotoxins such as deoxynivalenol produced by the fungus affect plant and animal health, and cause significant reductions of grain yield and quality. Resistant varieties are the only effective way to control this disease, but the molecular events leading to FHB resistance are still poorly understood. Transcriptional profiling was conducted for the winter wheat cultivars Dream (moderately resistant) and Lynx (susceptible). The gene expressions at 32 and 72 h after inoculation with Fusarium were used to trace possible defence mechanisms and associated genes. A comparative qPCR was carried out for selected genes to analyse the respective expression patterns in the resistant cultivars Dream and Sumai 3 (Chinese spring wheat).
Among 2,169 differentially expressed genes, two putative main defence mechanisms were found in the FHB-resistant Dream cultivar. Both are defined base on their specific mode of resistance. A non-specific mechanism was based on several defence genes probably induced by jasmonate and ethylene signalling, including lipid-transfer protein, thionin, defensin and GDSL-like lipase genes. Additionally, defence-related genes encoding jasmonate-regulated proteins were up-regulated in response to FHB. Another mechanism based on the targeted suppression of essential Fusarium virulence factors comprising proteases and mycotoxins was found to be an essential, induced defence of general relevance in wheat. Moreover, similar inductions upon fungal infection were frequently observed among FHB-responsive genes of both mechanisms in the cultivars Dream and Sumai 3.
Especially ABC transporter, UDP-glucosyltransferase, protease and protease inhibitor genes associated with the defence mechanism against fungal virulence factors are apparently active in different resistant genetic backgrounds, according to reports on other wheat cultivars and barley. This was further supported in our qPCR experiments on seven genes originating from this mechanism which revealed similar activities in the resistant cultivars Dream and Sumai 3. Finally, the combination of early-stage and steady-state induction was associated with resistance, while transcript induction generally occurred later and temporarily in the susceptible cultivars. The respective mechanisms are attractive for advanced studies aiming at new resistance and toxin management strategies.
Fusarium head blight (FHB) caused e.g. by F. graminearum Schwabe (teleomorph Gibberella zeae (Schwein.) Petch) is one of the most destructive diseases of wheat (T. aestivum L.) worldwide, causing significant reductions in grain yield and quality. The most efficient strategy to control FHB in wheat is the use of resistant cultivars[1, 2]. However, in hexaploid wheat the resistance to FHB is highly complex. Since 1999, over 200 QTL have been reported, whereas only a few QTL were found to be stable in different genetic backgrounds and useful for breeding. The most stable QTL were obtained from the Chinese wheat varieties Sumai 3 and Wangshuibai. However, poor agronomic performance and the frequent occurrence of genetic linkage drag make them less suitable donors of resistant genes. Moreover, the genetic and molecular basis of the quantitative FHB resistance is still poorly understood.
Recent studies on the mode of Fusarium spike colonisation have revealed that the pathogens use a specific arsenal of virulence factors which are essential in nearly all phases of the disease making them interesting targets for novel resistance strategies. Trichothecene toxins, such as deoxynivalenol (DON), and hydrolytic enzymes, such as subtilisin-like and trypsin-like proteases, are two virulence factors that were found to occur during almost the entire course of disease[5, 6]. DON was found to be produced in the fungal infection structures already during the initial penetration of floret tissues[7, 8]. The reason for this early secretion remains unknown, because the initial infection is symptomless and indistinguishable between susceptible and resistant wheat cultivars in all respects; even the trichothecene-deficient Fusarium mutants do not show any restrictions regarding their infectious ability[10–12]. However, already in the second infection phase, DON production gains relevance. It is supposed that the general capacity to prevent protein synthesis makes the toxin an important suppressor of early plant defences[13, 14]. For that purpose, DON seems to enable the fungal hyphae to break through the spike rachis node which is the central bottle-neck for both, the initial spread from infected florets into the spike rachis and the reverse direction from the rachis into uninoculated spikelets[10–12, 15, 16]. During the rachis colonization when hyphae grow vertically, the toxin may inhibit the onset of various cell wall reinforcement processes in the vicinity of invading hyphae. At the same time, fungal proteases are likely to participate in the suppression of plant defences by degrading pathogenesis-related (PR) proteins or defence-signalling compounds according to their property to cause proteolytic protein digestion[19–21]. In the spikes of the resistant landrace Wangshuibai the down-regulation of different housekeeping proteins was reported already 6 to 24 h after F. graminearum inoculation as a consequence of the secretion of fungal hydrolytic enzymes and toxins.
The intercellular spread through the spike rachis is accompanied by lateral hyphae growth to infect uninoculated spikelets. This secondary colonisation is essentially associated with the secretion of DON and proteases which initiate and facilitate necrotrophic intracellular nutrition. The phase is characterized by dramatic changes in the interaction between pathogen and host concerning the respective transcriptomes, secretomes and metabolomes[7, 17, 23, 24], and is often described as switching point from fungal biotrophy to necrotrophy. Increased DON levels were observed 26 to 96 h after infection (hai). In addition, between 48 and 72 hai F. graminearum transcripts were found to encode especially degrading enzymes such as proteases. These accumulations were typically linked to increased levels of systemic fungal development and collapsed host cells. Both virulence factors are probably essential for the penetration and mortification of host cells, as Fusarium pathogens use cell wall digestion to enter living host cells and DON, in particular, is known to activate plant programmed cell death[31, 32]. In summary, DON and proteases have a significant impact on cell wall digestion, protein matrix reduction and damage to starch granules, typically seen in Fusarium-infected wheat kernels rendering grain yield unsuitable and unsafe for food, feed or malting purposes[19, 33–36].
In order to characterise the transcriptional changes in the resistant cv. Dream compared with the susceptible cv. Lynx, we performed gene expression profiling using the GeneChip® Wheat Genome Array. GeneChip expression data obtained 32 and 72 h after inoculation with F. graminearum or, respectively, mock have revealed indications for the presence of two main defence mechanisms in cv. Dream, reflecting a biphasic strategy against FHB disease. One mechanism comprised jasmonate- and ethylene-mediated defence reactions directed against fungal growth and sporulation, while the second mechanism was specifically directed towards fungal mycotoxins and proteases. Quantitative real-time PCR (qPCR) time-course study was applied to analyse the expressions of seven selected anti-virulence gene candidates in the cultivar pairs Dream/Lynx and Sumai 3 (resistant)/Florence-Aurore (susceptible). Observed similarities between the resistant cultivars Dream and Sumai 3 in terms of FHB-responsive up-regulated genes from both described defence mechanisms will be reported.
Results and discussion
Identification of FHB-responsive genes in the resistant wheat cultivar Dream
Transcript abundances in the F. graminearum (FHB)-inoculated and mock-inoculated wheat cultivars Dream (resistant) and Lynx (susceptible) were measured and compared using the Affymetrix GeneChip® Wheat Genome Array. The general disease progression was examined on single-floret inoculated samples that were collected 32 and 72 hours after inoculation (hai). All measurements were performed with three biological replicates. For each timepoint the four GeneChip datasets were compared to identify differentially expressed genes involved in the different aspects of the inoculation response. Table1 lists all comparisons with the respective numbers of differentially expressed genes.
A gene set enrichment analysis (GSEA) of the comparisons was conducted to identify relevant functional classes associated to incompatible cv. Dream-F. graminearum interactions. Table2 provides an overview of the nine Gene Ontology (GO) terms that were enriched in those genes found to be significantly up-regulated in the resistant cv. Dream at 32 and 72 h after Fusarium inoculation compared with the Fusarium inoculated susceptible cv. Lynx. All terms were found to be associated to the disease as the respective represented gene products were neither enriched in the analogous cultivar comparison after mock inoculation nor in the comparison ‘cv. Lynx Fusarium inoculated versus cv. Lynx mock inoculated’. No GO terms were enriched in the significantly down-regulated genes at 32 hai while 20 enriched terms were observed at the later timepoint (Table3). For enrichments at 72 hai associations to the infection with F. graminearum were restricted and, thus, were only possible if a GO term was also enriched also at 32 hai.
The GSEA provided insides into defence mechanisms that were induced during incompatible interactions (Table2). At 32 hai an exclusive enrichment was observed for the terms ‘lipoxygenase activity’ (GO:0016165), ‘oxylipin biosynthetic process’ (GO:0031408) and ‘lipid biosynthetic process’ (GO:0008610) including genes, such as lipoxygenases, involved in the plant oxylipin metabolism. Additionally, lipoxygenases genes were also frequent in the term ‘response to wounding’ (GO:0009611). Putative cysteine-rich proteins, such as thionins, were detected in the GO term ‘pathogenesis’ (GO:0009405). Phyto-oxylipins comprising antimicrobial peptides and defence-signalling molecules such as jasmonates, together with cysteine-rich pathogenesis-related (PR) genes indicate an induced antifungal defence mechanism.
Plant serine-protease inhibitors were enriched in the GO terms ‘serine-type endopeptidase inhibitor activity’ GO:0004867 and ‘peptidase activity’ GO:0008233, and represented the second class of genes enriched in the term ‘response to wounding’ (GO:0009611). Serine-protease inhibitors as well as genes encoding serine-proteases identified by the term ‘serine-type carboxypeptidase activity’ (GO:0004185) were enriched at both timepoints. These enriched terms represent an induced defence mechanism against pathogen-released proteases which as virulence factors are secreted to modify host proteins[6, 39]. On the basis of testing, this defence mechanism as well as the antifungal defence mechanism were found to be central and therefore, will be discussed in more detail later on.
Finally, genes encoding for peptidyl-prolyl cis-trans isomerase (PPIase) proteins (GO:0003755) belonging to the immunophilin superfamily were found to be accumulated. PPIase proteins have general functions in protein folding and protein degradation, and several proteins have shown antifungal properties, similar to PR-genes[40, 41].
In the down-regulated genes (Table3) three GO terms were noticeable with regard to the pathogen presence, while associations to the disease were rather unclear for the other terms. The detected GO terms ‘chitin catabolic process’ (GO:0006032) and ‘chitinase activity’ (GO:0004568) demonstrate the down-regulation of genes which typically facilitate the breakdown of fungal cell walls. Chitinase genes have shown to exhibit an enhanced resistance against F. graminearum, in barley while in the grains of Emmer wheat (T. dicoccum), a progenitor of bread wheat (T. aestivum), a similar down-regulation of chitinase genes was observed and discussed as a direct impact of F. graminearum signals. Finally, the term ‘mycelium development’ (GO:0043581) comprises 10 F. graminearum genes, belonging to a set of 69 Fusarium genes which were previously found to be present on the Affymetrix Wheat GeneChip®. As these genes are putatively associated to the progression of the fungal mycelium, their enrichment amongst down-regulated genes might reflect traces of an impaired fungal growth in the resistant Dream cultivar.
A comparison was performed between the ‘cv. Dream Fusarium inoculated versus cv. Lynx Fusarium inoculated’ expression data and the analogous expression data from the mock inoculation (Table1), in order to address expression changes in the resistant cv. Dream associated with the fungal attack. At 32 hai, the genes differentially expressed in cv. Dream could be separated into genes that were differentially expressed to higher levels or were only present after pathogen attack (Figure1 section A), after both treatments (Figure1 section B), and only after control treatment (Figure1 section C). The genes only present in response to FHB were categorised as ‘FHB-responsive genes’. Especially, up-regulated transcripts are likely to represent defences, such as trigger mechanisms or direct antimicrobial activities. Genes with similar expression profiles after both treatments were categorised as ‘genotype-specific genes’ because they were differentially expressed to lower levels or absent in the cv. Lynx spike samples. Up-regulated genes were hereafter discussed as members of a basal defence if their induction has been demonstrated in previous related resistance studies. Finally, a comparison of the genes differentially expressed in cv. Dream at 32 and 72 h after Fusarium inoculation was performed to separate expression changes which have been maintained (Figure1 section E) from those that were exclusive for one of the two timepoints (Figure1 section D and section F). Genes that are only differentially expressed at 72 hai (Figure1 section F) were categorised as ‘72 hai-specific genes’. A mapping into one of the two categories ‘FHB-responsive genes’ and ‘genotype-specific genes’ could not be done, due to the low quality of the microarrays obtained from mock treated cv. Lynx samples at this timepoint (Table1).
The revised dataset contained a total of 2,169 differentially expressed genes after the transcripts likely to represent general cellular processes in cv. Dream were removed. In total 374 of those genes could be assigned to 11 different defence-related classes. The gene classes and assignments were made based on the GSEA results and on information obtained from FHB-related literature. Table4 gives an overview of the respective number of individual genes which have been assigned to the three categories and the 11 defence-related gene classes. Detailed information on genes that were identified as putative defence-related is provided in Additional files1,2 and3. The GSEA results were contributing to the formation of the functional classes: (i) ‘jasmonic acid (JA) and ethylene (ET) related genes’; (ii) ‘cysteine-rich antimicrobial peptides (AMPs)’ including serine-protease inhibitors; (iii) ‘jasmonate-regulated proteins (JRP)’ comprising a set of strictly FHB inducible genes; (iv) ‘GDSL-lipases’; and (v) ‘proteolysis’ including serine proteases. Based on literature, genes with different direct or indirect antifungal properties were added to the following classes: (vi) ‘peroxidases’; (vii) ‘genes related to cell wall defence’, for example PGIP1 s (polygalacturonase inhibiting proteins), xylanase inhibitors and glucan endo-1,3-beta-glucosidase precursors, and (viii) ‘secondary metabolism/detoxification’. The remaining gene classes ‘transcription or signalling genes’, ‘miscellaneous defence related genes’ and ‘hormone metabolism’ have been made for the convenience of discussion.
Indications for a Jasmonate-dependent enhancement of FHB resistance in wheat
Indications for the presence of a JA signalling were found in the cv. Dream transcriptome after FHB infection by using GSEA testing. The GO terms ‘lipoxygenase activity’ (GO:0016165), ‘oxylipin biosynthetic process’ (GO:0031408) and ‘lipid biosynthetic process’ (GO:0008610) associated to the oxylipin metabolism were exclusively enriched in the early 32 hai gene expression data (Table2) indicating that the chloroplastic 13-LOX-branch was induced upon FHB infection. Hormone-like compounds such as JA and methyl jasmonate (MeJA), as well as 13-HPL-derived C6 aldehydes, are characteristic products of this pathway. Some oxylipins generated by the 13-LOX pathway, for example thaumatin-like proteins and phytoalexins, exhibit antimicrobial activities by impairing fungal mycelial growth and spore germination[45, 46]. Other oxylipins, such as JA and MeJA are well known to serve important roles in plant defence-signalling by mediating the induction of the expression of some PR-genes[47–50]. Moreover, as 13-LOX oxylipins are substantially produced from cuticle- or cell membrane-associated fatty acids released during the fungal degradation of plant cell walls, they also act as elicitors involved in pathogen recognition.
Threeputative Lox genes (Ta.13650.1.A1_at, Ta.1967.2.A1_x_at and TaAffx.104812.1.S1_s_at) were FHB-responsive induced at 32 hai (Additional file1). The transcript Ta.13650.1.A1_at was found to be a homologue of the maize gene ZmLOX6 (DQ335764) which is a novel chloroplast localized Lox gene described as uniquely regulated by phytohormones and pathogen infection (Table5). The two transcripts Ta.1967.2.A1_x_at and TaAffx.104812.1.S1_s_at showed significant similarity to the barley gene Hordeum vulgare methyljasmonate-inducible lipoxygenase 2 (U56406) (Table5). Therefore, both transcripts might encode for one or two putative methyljasmonate (MeJA)-inducible chloroplastic 13-Lox genes. It was shown that jasmonates regulate their synthesis via positive feedback control by inducing the transcription of biosynthesis genes such as Lox2[53–55]. It is remarkable that both transcripts were also already induced 24 h after F. graminearum inoculation in the resistant spring wheat cv. Sumai 3.
Five Lox genes were up-regulated after both treatments and, in contrast to the solely FHB dependent induced Lox genes, three of them were also expressed at 72 hai (Additional files2 and3). Here, except for the transcript Ta.1967.1.S1_x_at, none of the genes could be assigned to a JA-mediated defence based on sequence similarities to published genes (Table5). Ta.1967.1.S1_x_at, however, a homologue of a barley gene Lox2 involved in different stress responses (Table5), was also shown to be active in cv. Sumai 3 upon F. graminearum infection.
In summary, putative functions regarding defence response mediation were assigned to genes showing FHB-associated expression alterations. Here, all genes were found to be jasmonate and pathogen inducible or were previously identified as being FHB-responsive in cv. Sumai 3. This is remarkable as the cultivars Dream and Sumai 3 represent entirely different (geographical) origins and resistance levels. Additionally, JA and ET defence-signalling pathways were found to be essentially involved in the high level FHB resistance of wheat cv. Wangshuibai in a recent study and were supposed to mediate the early basal defences at 12 to 24 h after F. graminearum infection. However, the contribution of a salicylic acid (SA) signalling towards FHB resistance reported in that study was neither observed in our study nor reported for the cv. Sumai 3. On the other hand, a continual JA production can be involved in pathogen defence as well. Indications for JA-inducible as well as for a continual PR-gene expression were indeed observed in the cv. Dream and both might contribute to the present FHB resistance (see below).
A Jasmonate-responsive and non-specific antifungal defence contributes to FHB resistance
The enrichment of genes belonging to the 13-LOX pathway indicates a systemic accumulation of endogenous jasmonates in the resistant cv. Dream as a result of F. graminearum infections. It is known that members of the jasmonate family, whose levels increase on pathogen infection, activate a specific set of genes encoding antimicrobial peptides (AMPs)[38, 59]. Several cysteine-rich AMPs were found to be up-regulated in FHB infected cv. Dream spikes, which are possible targets of such resistance-related JA signalling, when the two points in time were investigated. The set of identified cysteine-rich AMPs comprises lipid transfer proteins (PR-14), thionins (PR-13), and defensins (PR-12).
Lipid transfer proteins (LTPs) were the most frequently expressed class of AMPs. Three genes were up-regulated independent of the treatment, while two transcripts were up-regulated exclusively 72 h after FHB inoculation. Compared to the other identified cysteine-rich AMPs, most of the LTP genes have shown relatively high fold changes that remained constant at both timepoints (Additional file1,2 and3). BLASTN analyses proved that all present LTP genes encode for putative non-specific lipid-transfer proteins (nsLTPs). Direct antifungal activities and a broad resistance spectrum against biotrophic and necrotrophic fungal pathogens have been reported for various crop species and tissues, notably with nsLTPs[60–62]. The observed antifungal activities also include different Fusarium pathogens, such as F. graminearum (wheat) and F. solani (maize and barley), as well as F. culmorum and F. oxysporum (onion)[61–64]. Thereby, nsLTP proteins were found to strongly inhibit the growth of fungal mycelia as well as the germination of fungal spores, including the conidiospores of F. graminearum[63, 64]. Wheat ns-LTPs are generally supposed to play a role in an enhanced non-specific defence response regulated by different hormonal signals, including jasmonates. In particular, constitutively expressed genes are supposed to contribute to non-host resistance.
A synergistic activity of nsLTP genes with thionins (PR-13) against F. solani and F. graminearum was shown in studies on barley, maize and wheat[62, 63, 65, 66]. In fact, two transcript sequences (Ta.23967.1.S1_s_at and Ta.23967.1.S1_x_at) homologous to the wheat thionin gene THI1.1 were differentially expressed in the cv. Dream after both treatments, but not in the cv. Lynx (Additional file2). Thionins have a general antimicrobial activity against early conidial germination. In addition, a highly inducible expression was observed in the case of the Arabidopsis thionin Thi2.1 after both fungal infections as well as MeJA treatment leading to an enhanced resistance to F. oxysporum.
Peptidase inhibitors of the defensin family (PR-12) make up the third class of continual up-regulated AMPs (Additional file2), represented by homologues of the wheat gene Tad1 (Ta.28319.1.S1_at) and the defensin precursor PRPI-7 from durum wheat (T. durum) (Ta.20930.1.S1_at) (Table5). While the antimicrobial activity of defensins requires typically complex synergistic interactions with other AMPs, their promoters are potentially interesting candidates for the targeted and tissue-specific expression of PR- and R-genes, particularly for the protection against F. graminearum in cereal grains.
An induction by jasmonates was reported for most of the defensin genes and some of the putative antifungal defensins are reported to be markers for the presence of JA- and ET-dependent defence-signalling pathways. Indeed, indications for an active ET signalling were found in the FHB-attacked cv. Dream transcriptome as well (see below).
The majority of up-regulated cysteine-rich AMPs in cv. Dream have shown expression values that were independent of the treatment, but were lower or absent in the susceptible cv. Lynx (Table4, Additional file1 and2). It is likely that the majority of these peptides act synergistically in a generalized non-specific defence providing a basal protection. AMPs transcribed at a constant level are known key components of an immediate defence against invading pathogens[75–77], and many proteins that are pathogen-inducible, for example, in leaves were found to be constitutively present in storage tissues, such as seed. Moreover, it is generally assumed that genes involved in the quantitative FHB resistance of adapted European wheat cultivars represent such a defence mechanism.
Nonetheless, AMPs can also be part of an induced plant defence. In FHB-treated cv. Dream spikes only nsLTP genes were up-regulated in response to the disease (Additional file1). Among these Ta.7843.1.S1_a_at (Table5) seems to be an interesting resistance candidate, as the gene combines a general high antifungal property with considerable fold change expression ratios at both timepoints (Additional file1). Moreover, the putative defensin gene PRPI-7 (Table5) might be a relevant finding as well due to its possible utilization in a resistant strategy aiming at over-expressions of pathogen-inducible promoters to directly target the infection sites or the most vulnerable tissues. Such an approach becomes even more interesting with the recent observation that the biotrophic life form of F. graminearum persists in all colonized tissues. Living host cells form a zone surrounding the most advancing hyphae and could be targets for such an approach as they allow a continuous supply with antifungals onto the intercellular hyphal tips.
Identification of FHB-responsive jasmonate-regulated proteins
Taking into account the observations on the Dream and Sumai 3 cultivars it can be hypothesised that a FHB-responsive JA signalling is active from 24 to 32 hai covering the presumed phase of the general biotrophic fungal growth, since the switching point to increased necrotrophic nutrition was timed around 48 hai[5, 23]. An interesting conformance was observed with the FHB-responsive expressions of genes that encode for jasmonate-regulated proteins (JRP), belonging to the subfamily of mannose-specific jacalin-like lectin containing proteins (mJRL) during that period.
Three mJRL genes, TaAffx.7388.1.S1_at, Ta.188.1.S1_at and Ta.31.1.S1_at, were up-regulated in cv. Dream at 32 hai. The first two transcripts are prominent due to the considerable fold change expression ratios of 20.9 and 21.7 (up) (Additional file1) and their up-regulation exclusively in the FHB treated spikes of cv. Dream. As many mJRL genes are described as strictly inducible defence proteins[80–82], TaAffx.7388.1.S1_at and Ta.188.1.S1_at might be involved in the FHB defence. BLAST analysis showed that all detected putative mJRL genes belong to the mJRP-32 protein subfamily. In general, mJRP-32 genes are specifically induced by JA via transcriptional activation and were initially identified in jasmonate-treated barley leaves. The first mJRP-32 gene analysed in detail was the BGAF (beta-glucosidase aggregating factor-like protein) gene from maize. The sequence of the transcript TaAffx.7388.1.S1_at shows similarities to another maize BGAF gene (NM_001111494) as well as to the wheat gene Ta-JA1 (AY372111). Although detailed knowledge on the defence function of mJRP-32 proteins is still to be gained, a broad resistance spectrum has already been observed. One prominent example is the Ta-JA1 gene that encodes a modular BGAF-related protein with a proven broad-spectrum resistance to infections by bacterial, fungal and viral pathogens in transgenic tobacco plants. All currently known mJRP-32 genes come from Poaceae and share important traits separating them from other mJRLs, for example their exclusive, tissue-specific induction via jasmonates and their single-copy status. However, notably due to their strict tissue-specific expressions, mJRP-32 genes are not supposed to be orthologous, although the proteins share numerous common features. An mJRP-32 gene expressed in spike tissues has not been reported so far. For this reason and due to its FHB-responsive high level induction, a separate study should reveal whether the TaAffx.7388.1.S1_at gene represents a new spike-specific member of the mJRP-32 family.
In addition to Ta-JA1, the Poaceae JRP-32 family comprises three other wheat genes: Ver2 (Table5), WCI-1 (Table3) and Hfr-1 (AF483596). In the present work, the wheat chemically-induced gene WCI-1 and the vernalisation-related gene Ver2 were up-regulated in cv. Dream upon F. graminearum infection. WCI-1 (Ta.188.1.S1_at) was characterised as a plant disease resistant response gene that is induced by Benzothiadiazole (BTH). BTH is a functional analogue to SA which was not successful in reducing the FHB-disease caused by F. graminearum. On the other hand, an up-regulation of WCI-1 upon MeJA application has been reported, and the WCI-1 orthologous pea gene DIR1 was found to be involved in the resistance to different Fusarium pathogens. Due to these contradictory observations further examinations are required to clarify the role of WCI-1 in FHB resistance.
The up-regulation of the vernalisation-related gene Ver2 (Ta.31.1.S1_at) upon F. graminearum infection is interesting. Indeed, due to the proven specific induction by MeJA, Ver2 was initially proposed to be involved in a jasmonate mediated plant defence response. However, an induction of expression upon F. culmorum infection could not be confirmed and a native Ver2 induction has so far only been observed in young wheat seedlings during the vernalisation process. Thus, whether the untypical expression of Ver2 in wheat kernels is associated with FHB resistance, or rather is a side effect caused by jasmonate-signalling remains unanswered at this point.
An increased ethylene (ET) production contributes to wheat FHB resistance
Ethylene (ET) plays an important role in plant growth and development but it is also known to be involved in the regulation of primary resistance responses. Indications for an increased ET-metabolism in cv. Dream spikes following FHB infection are provided by several up-regulated putative 1-aminocyclopropane-1-carboxylate (ACC) oxidases and GDSL-like lipases genes.
The ACC oxidase, also called the ET-forming enzyme, catalyses, together with the enzyme ACC synthase, the last biosynthetic step to convert ACC into ET. Both enzymes are known to be rate-limiting components in the ET biosynthetic pathway. A total of 10 ACC oxidase genes were either up-regulated or down-regulated in the cv. Dream, mainly in a constitutive manner (Additional file1 and2). In fact, the expression of individual ACC oxidase genes is generally frequent and differentially regulated at all times due to developmental changes as well as abiotic and biotic stress factors[90, 91].
The occurrence of several GDSL-like lipase genes in the cv. Dream assay further indicates an elevated ET-signalling. GDSL-like lipases were mainly differentially expressed upon both treatments (Additional file1 and2). Among the characterised GDSL-like lipases, the genes GLIP1 and GLIP2 of Arabidopsis are known to play an important role in plant immunity by eliciting local as well as systemic resistance against necrotrophic and hemibiotrophic pathogens. Moreover, GDSL-like lipase transcription was exclusively enhanced by ET, but not by SA or JA. However, none of cv. Dream GDSL-like lipases has shown a sequence homology to the reported resistance candidates from Arabidopsis.
It is generally accepted that the plant defence against necrotrophic pathogens is usually regulated by JA and ET while SA plays a major role in the defences against biotrophic pathogens. A possible involvement of ET in FHB resistance has also been demonstrated for Sumai 3, based on an up-regulated ACC oxidase gene. Furthermore, an increased resistance against FHB was observed for the susceptible cultivar Y1193 after spraying spikelets with JA as well as ET before and after fungal infection. Different studies in Arabidopsis and tobacco have shown that ET and, in particular, the over-expression of certain ACC oxidase genes can extend the symptomless biotrophic phase during hemibiotrophic fungal infections. In addition, it was found that ET can reduce cell death caused by the fungal toxin Fumonisin B1 which is produced by several cereal-attacking Fusarium species.
Indications for FHB-responsive suppression of fungal virulence factors
In addition to the presence of JA- and ET-mediated general antifungal defences, a second line of defence was found to be based on a FHB-responsive and targeted suppression of relevant Fusarium virulence factors, such as proteases and mycotoxins. This defence mechanism was assembled from genes encoding protease inhibitor (PI) proteins (PR-06) and different genes which are proposed to be associated with the detoxification of pathogen-derived mycotoxins. Both, Fusarium proteases and mycotoxins take on relevant roles in the fungal pathogenesis and were found to be secreted in nearly all phases of the fungal wheat spike colonisation[9, 19, 20, 22, 96].
Wheat-derived protease inhibitor genes in FHB disease resistance
In the FHB-treated cv. Dream transcriptome, serine PI proteins of the subtilisin-like protease (SLP) superfamily were significant enriched at both timepoints (Table2), represented by the Go terms ‘serine-type endopeptidase inhibitor activity’ (GO:0004867) and ‘peptidase activity’ (GO:0008233). PI proteins generally feature a high substrate specificity and therefore, it is likely that those genes encode for proteins that specifically bind and impair secreted Fusarium SL proteases. Proteases generally cause the proteolytic digestion of proteins via the hydrolysation of peptide bonds. Fusarium subtilisin-like (SL) and trypsin-like (TL) proteases are released in infected wheat kernels mainly to disrupt host cell membranes during necrotrophic intracellular nutrition. Consequently, defence-related interactions between plant PI proteins and subtilisin-like and trypsin-like proteases of F. graminearum and F. culmorum have already been proven in the grains of barley[6, 24] and ancient emmer wheat (T. dicoccum).
In total, five serine-protease inhibitors were differentially up-regulated in cv. Dream (Additional Table12 and3). Two transcripts were functionally annotated to the Bowman-Birk inhibitor (BBI) family based on sequence homologies to the WRSI5 gene (Table5). WRSI5 was described as a salt-responsive gene with a suggested role in regulating plant growth. Among the remaining transcripts, Ta.2632.2.S1_x_at and Ta.2632.3.S1_x_at were up-regulated in response to FHB at 32 hai, while Ta.22614.1.S1_at was regulated solely at 72 hai.
The Ta.22614.1.S1_at gene was selected for qPCR analysis because of its relativelyhigh and FHB-responsive fold change (9.49 up) at 72 hai (Additional file3). A possible expression at 32 h after Fusarium inoculation was not reliably determined due to missing expression data from two of the three biological replicates. The Ta.22614.1.S1_at expression was measured with an inoculation time-courses of two cultivar pairs: first, the winter cultivars Dream and Lynx described as moderately resistant and susceptible (time-course of 8 to 96 hai); second, the spring cultivars Sumai 3 and Florence-Aurore described as resistant and susceptible (time-course of 0 to 336 hai). Sumai 3 and Florence-Aurore, in particular, were found to represent the extremes of spring wheat responses to Fusarium spread[99, 100].
Upon comparing the FHB-responsive transcript induction levels in the cultivars Dream and Lynx, a generally higher induction over control and cv. Lynx samples was observed for cv. Dream for the period between 24 to 96 hai (Figure2A). As a matter of fact, >4-fold inductions were only obtained at 48 and 72 hai. However, even the 2-fold inductions of earlier and later timepoints were considered relevant due to the strictly suppressed expression in the susceptible genotype (Figure2A). In the FHB-treated spike tissues of Sumai 3, >600 and >300-fold inductions were already observed between 8 to 32 hai and a third peak of >200-fold was found at 96 hai (Figure2B). No gene expression was verifiable in spike samples of cultivars Sumai 3 and Florence-Aurore at 336 hai which was the last timepoint (not shown).
In the first instance, the relative induction peak at 72 hai in cv. Dream is consistent with previous observations that endogenous wheat serine-protease inhibitor proteins are not induced until 72 h after Fusarium inoculation. In fact, in the period between 48 and 72 hai, during which the necrotrophic nutrition becomes predominant, F. graminearum transcripts were found to dominantly encode degrading enzymes such as proteases, lipases and nucleases. A transcript accumulation was even observed in the susceptible genotypes Lynx (Figure2A) and Florence-Aurore (Figure2B) particularly in this period, however, to a lower extent than in the respective resistant counterparts. The physiological responses of PIs are furthermore triggered by negative feedback mechanisms. Therefore, the remarkable suppression of Ta.22614.1.S1 in Sumai 3 during this crucial time might be a consequence of the already high transcript abundance and the subsequent induction at 96 hai is assumed to be stimulated by further secreted fungal proteases (Figure2B).
The early high level activity of Ta.22614.1.S1 until the timepoint 32 hai in cv. Sumai 3 (Figure2B) is consistent with previous data from Sumai 3 gene expression studies, demonstrating the FHB-responsive expression of several PIs at already 24 hai. In this period, an exclusive induction of the tested serine-protease inhibitor was also observed for the moderately resistant cv. Dream (Figure2A). Consequently, the early expression of wheat PI genes could be an immediate reaction to early levels of secreted Fusarium TL and SL proteases which have been reported for different compatible interactions, amongst others between F. graminearum and barley as well as wheat. Here, the activity of fungal proteases has been attested already at 6 to 24 hai, long before a corresponding expression could be observed in kernels[22, 28]. In fact, beside their harmful roles during the phase of a necrotrophic intracellular nutrition, fungal proteases were found to be secreted already during the earlier intercellular colonisation of spike rachis, probably to suppress certain plant defence reactions by degrading PR-proteins[15, 20, 21, 96, 103].
In this sense, the serine-protease inhibitor Ta.22614.1.S1_at seems to be an interesting resistance candidate as transcript accumulations were present during the early and the later phases of fungal spike colonisation. However, this potential still needs to be confirmed in a further study. Nevertheless, PIs are discussed as candidates for an improved resistance strategy against grain infecting fungal pathogens[19, 104] and our results from qPCR and transcriptome analyses do not contradict these considerations.
Analysis of the detoxification mechanisms in wheat concerning FHB resistance
Fusarium proteases and mycotoxins act in a kind of strategic cooperation during spike and kernel colonisation by featuring complementary roles during the host defence suppression and the intracellular colonisation of spikelets. From an economic perspective, Fusarium species causing FHB belong to the most important trichothecene producers and DON is a predominant trichothecene toxin produced by these species. Silencing the Fusarium TRI6 gene down-regulates more than 200 genes involved in the mycotoxin production and results in a reduction of DON production and pathogenicity. Meanwhile, several different plant genes are known to be up-regulated at the transcriptional level in response to either DON treatment or DON production which are thus likely to be involved in the DON-resistance.
To analyze the expected impact of a specific mycotoxin defence on the general FHB resistance of cv. Dream, a literature-to-transcriptome approach was used. Known toxin resistance-related genes from wheat and barley were checked for homologous genes on the wheat array and their respective expression profiles in the cultivars Dream and Lynx. A diverse set of 26 wheat genes could be identified as possible members of a general detoxification mechanism. Those genes are listed in Table6, including the respective literature sources. Within this set, 12 genes originate from a study of trichothecene-induced gene expression in barley. Screening the expression patterns of those 26 genes in the cv. Dream vs. cv. Lynx microarray data revealed for all genes similar expression patterns. They were exclusively expressed or induced in Fusarium treated samples collected 72 h after infection. Moreover, they were also up-regulated in both genotypes and, in addition, they were up-regulated in both genotypes and the level of up-regulation was higher in susceptible cv. Lynx in all cases. However, expression differences between both genotypes never reached a level of statistical significance. Finally, they were not expressed in mock control samples at all, although this observation was not reliable in the case of cv. Lynx samples collected at 72 hai due to the above mentioned restrictions. To analyse the observed congruities in more detail and to test whether or not the expression in the susceptible cv. Lynx is just a temporary phenomenon, a selection of six genes representing different functional categories was forwarded to qPCR analysis using the above mentioned inoculation time-courses of the cultivar pairs Dream vs. Lynx and Sumai 3 vs. Florence-Aurore.
The analysed genes associated with DON detoxification are TaUGT3 (UDP-glucosyltransferase protein) and a homologue of the barley UDP-glucosyltransferase gene HvUGT13248. Genes that are supposed to be involved in the resistance to DON accumulation are TaPDR1 (pleiotropic drug resistance 1) and TaMDR1 (MDR-like ABC transporter gene). As representatives of the functional categories “defence-related” and “general” a further putative serine-protease gene and a 12-oxophytodienoate reductase gene were included (Table6).
The qPCR data for the winter wheat cultivars Dream vs. Lynx (Figure3A-3D) showed similar expression patterns for all tested genes as did the microarray experiments. Consequently, a temporary and higher induction peak was found for Lynx at 72 hai compared to Dream. On the other hand, the transcripts of all tested genes peaked at 96 hai in the cv. Dream samples, while Lynx revealed suppressed or consistent inductions. In addition, a >4-fold induction was already observed before 72 hai for most of the cv. Dream alleles and the expressions were showing a general and increasing trend towards the peak at 96 hai (Figure3A-3D). Such a maximum induction at 96 hai has likewise been observed for the DON resistance candidate gene PDR5 (pleiotropic drug resistance5)-like in infected spikes of the Chinese landrace Wangshuibai which represents one of the most important genetic resources for FHB and DON resistance. Like the analysed genes TaPDR1 and TaMDR1 (Figure3A and3B), PDR5-like is like a plasma membrane ABC transporter which co-segregates with the DON resistance QTL Qfhs.ndus-6BS from cv. Wangshuibai.
In the cultivar pair Sumai 3 vs. Florence-Aurore the Fusarium-induced expression levels obtained for the UDP-glucosyltransferase (UGT) and ABC transporter genes were showing typical curve characteristics in cv. Sumai 3 samples; starting with a low level induction at 8 hai, followed by a consistent increase up to the peak at 32 or 48 hai and showing a continuous downtrend thereafter (Figure4A-4D). In contrast, considerable inductions for the susceptible cv. Florence-Aurore did not appear until 96 to 120 hai (Figure4A-4D). Interestingly, both UGT genes show induction peaks at 32 hai in cv. Sumai 3 while both ABC transporter genes peak at 48 hai. Deviating induction patterns were observed for the representatives of the functional categories “defence-related” and “general” (Figure4E and4F). For all tested genes no expressions were measured from samples collected at 336 hai (not shown).
In summary, the expression profiles of genes related to detoxification in both resistant cultivars were following an early beginning steady-state model, providing transcript levels during the reported period of increased DON accumulations between 36 and 144 hai[5, 13, 106]. In contrast, both susceptible cultivars showed typically late and temporary inductions. Our observations for the expressions of UGT and ABC transporter genes in cv. Sumai 3 are furthermore in accordance with expression patterns previously observed for the ABC transporter gene TaPDR1 as well as the UGT gene TaUGT3 in FHB-treated spike samples of cv. Wangshuibai.
The TaPDR1 gene is a member of the ATP-binding cassette (ABC) protein superfamily and has been identified in cv. Wangshuibai due to its strong up-regulation upon DON treatment as well as F. graminearum inoculation. After fungal infection, the relative amount of TaPDR1 transcripts increased in Wangshuibai at 48 hai. The function of TaPDR1 in FHB resistance is proposed to be DON-related because gene expressions were found to peak after 6 to 12 h of DON-inoculation and declined slowly thereafter. In addition, a late expression peak was observed for the susceptible cv. Alondra similar to our observations in the susceptible cv. Florence-Aurore (Figure4A). The general role of PDR transporters in the resistance to antifungal drugs was first characterized in yeast (S. cerevisiae) and a particular function in DON resistance was confirmed based on a yeast mutant carrying a knockout variant of the PDR5 transporter gene resulting in a non-natural hypersensitivity to DON.
The second analysed transporter gene TaMDR1 was initially isolated from wheat root apices as being induced by aluminium toxicity. However, TaMDR1 was up-regulation together with TaPDR1 in cv. Wangshuibai and, thus, was supposed to be involved in DON resistance as well. In fact, our time-course qPCR expression data were able to reveal that both genes show similar expression profiles upon Fusarium infection in the resistant cultivars Dream (Figure 3A and 3B) and Sumai 3 (Figure4A and4B), respectively. Although genotype-specific differences were present, the observed similar expression patterns indicate a possible trichothecene-responsive up-regulation for TaMDR1 as well. Using nullisomic-tetrasomic wheat lines, we have also located the TaMDR1 allele on chromosome 5A where TaPDR1 had already been placed before. These observations may reflect a common mechanism of transcriptional co-regulation for both genes. In general, there is accumulating evidence that gene order in eukaryotic genomes is not completely random and that pathogen-responsive as well as other genes with similar expression levels tend to be clustered within the same genomic neighbourhoods. In fact, for TaPDR1 it was discovered that the gene expression is not induced by JA, SA and abiotic stress factors but by decreasing concentrations of Al3+ and free [Ca2+. This mode of regulation was also reported for the TaMDR1 gene due to its general induction by Al injury in wheat roots. Both toxicities activate plant programmed cell death via an oxidative burst and both inhibit calcium channels of plasma membranes which causes a decrease of the intracellular second messenger [Ca2+[31, 112, 113]. In order to explain the commonalities we have found between both ABC transporters in terms of induction, we suggest that DON induces the expression of TaPDR1 and TaMDR1 indirectly via decreased levels of [Ca2+. Whether TaMDR1 thus has a similar relevance for the detoxification process as can be suggested for TaPDR1, still needs to be proven in a further study.
Two UGT genes supposed to be involved in the DON detoxification were analysed with qPCR. Quite a few of the plant UGTs are related to disease resistance where they play important roles in the detoxification of exogenous compounds, for example fungal metabolites such as DON. BLASTN analysis revealed the homology between the transcript Ta.23272.1.S1_at and the TaUGT3 (FJ236328) gene which had originally been cloned from cv. Wangshuibai. Ta.12887.1.S1_at has revealed a significant full length sequence homology to the barley UGT gene HvUGT13248 (Table4). Both genes have displayed the respective characteristic qPCR expression profiles for cvs. Dream (Figure3C and 3D) and Sumai 3 (Figure4C and4D) as described above. However, higher induction levels were observed for the putative HvUGT13248 gene when compared to TaUGT3.
At the first instance, the wheat gene TaUGT3 was the most interesting candidate since it was suggested to be an efficient candidate gene for improving DON resistance. However, our expression data are in accordance with recent observations which have demonstrated that HvUGT13248 can protect yeast from DON by converting it to DON-3-glucoside while TaUGT3 was not able to convert DON. In addition, with our observations in the cultivars Dream and Sumai 3, HvUGT13248 has demonstrated relevant activities in a number of FHB-treated wheat cultivars as well as in barley, indicating that it be might of general relevance. HvUGT13248 (Ta.12887.1.S1_at) and also TaUGT3 (Ta.23272.1.S1_at) were detected as DON resistance candidates in DON inoculated spikes of cv. Wangshuibai in a gene expression study using the Affymetrix Wheat Gene-Chip®. Moreover, BLASTN analysis could demonstrate that HvUGT13248 has also been identified as DON resistance related gene (TA/EST accession TA88294_4565) in wheat DH-lines carrying the major FHB resistance QTL Fhb1 from cv. CM82036 as well as in two related barley transcriptome studies (Barley1GeneChip® probe Contig13248_at)[106, 117]. Finally, the gene HvUGT13248 appears to be a remarkable candidate gene for FHB resistance. It is considered relevant for a promising strategy to improve FHB resistance not only in wheat but also other cereal species.
As representative for the functional category “general”, the expressions of a putative wheat gene encoding for a 12-oxophytodienoate reductase was analysed (Table4). Ta.1207.1.S1_at was functionally characterised by significant homology to the maize 12-oxo-phytodienoate reductase gene ZmOPR1 (Table6). The homologous barley gene (Contig6194_s_at) was previously found to respond to pathogen-derived trichothecene accumulation. In addition to Ta.1207.1.S1_at, two more putative OPR genes were identified as up-regulated in response to FHB: the gene ZmOPR2 (Table5) and the gene ZmOPR4 (Table5). All three genes are putative wheat homologous of the OPR I group members which preferentially catalyse the formation of the natural JA precursor 12-oxo-phytodienoic acid (OPDA).
In our qPCR analysis, the ZmOPR1 homologue Ta.1207.1.S1_at has shown a FHB-associated induction at 32 hai which was common for both the resistant genotypes (Fig 3E and4E). This might indicate a rapid and transient up-regulation of Ta.1207.1.S1_at. In fact, the genes ZmOPR1 and ZmOPR2 have demonstrated a transient induction upon Fusarium verticillioides infection in maize. A similar rapid and transient up-regulation caused by a variety of environmental cues including hydrogen peroxide (H2O2) was observed for the Ta.1207.1.S1_at homologous gene OsOPR1 (EU146300) in rice. DON is known to induce the transient accumulation of H2O2 as the most stable compound involved in oxidative burst[31, 32]. Indeed, yeast studies indicate detoxifying functions for OPRI enzymes.
Indications for a complex crosstalk between fungal and plant proteases and their inhibitors during FHB defence
The putative wheat serine protease gene (Ta.8040.1.A1_at) belongs to the subtilisin-like protease family and was initially detected as a gene (Contig22733_at) that strictly responds to pathogen-derived trichothecene accumulation in barley (Table6). In addition, serine proteases were found to be enriched in the cv. Dream transcriptome upon FHB treatment and were annotated to the GO term ‘serine-type carboxypeptidase activity’ (GO:0004185) (Table2). An early Ta.8040.1.A1_at expression was found for cv. Sumai 3, here, exclusive and equal >2-fold inductions were present at 8, 32 and 72 hai (Figure4F). At 96 hai, both resistant cultivars showed the highest induction level, in cv. Dream even with a peak of >60-fold, while at this timepoints no expressions were found in the susceptible cultivars (Figure3F and4F). An opposing effect was observed at 32 hai, when exclusive expression was observed for both susceptible wheat cultivars, while no expression was detectable in the resistant ones (Figure3F and4F).
As proteolytic and protein-binding enzymes proteases feature important functions for the selective breakdown of regulatory proteins and several plant proteases have been linked to defence responses. Although many questions remain unanswered concerning their mode of action, there is evidence that plant proteases, in particular subtilisin-like proteases, are involved in the crosstalk between pathogen and host. In this context, a defence-counter-defence mechanism was observed between the plant-pathogen interaction tomato/Phytophthora infestans, in which both, host and pathogen are supposed to release specific sets of proteases and protease inhibitors mutually impairing each other[39, 121]. Moreover, such counter-defence mechanism is supported by the assumption of a strong co-evolution between proteases and protease inhibitors which are mutually released during a pathogen-host interaction. It is interesting in this context, that proteases as well as protease inhibitors were enriched in the transcriptome of the resistant cultivar Dream upon F. graminearum infection (Table2). Regarding the role of the reported plant proteases involved in DON resistance (Table6), we suggest that they do not act in response to a DON accumulation but rather in response to a Fusarium protease- rich environment as Fusarium proteases appear together with mycotoxins during spike rachis and kernel colonisation. In addition, a specific function within a detoxification mechanism has yet not been described for plant proteases.
Our transcriptome study provides evidence for the existence of a biphasic defence reaction against FHB in wheat. Jasmonate and ethylene regulated non-specific antifungal protections are supplemented by host gene networks associated to the accumulation of F. graminearum-derived trichothecenes and subtilisin-like proteases. Using a literature-to-transcriptome approach, 26 genes described as related to DON resistance were identified due to analogies in their microarray expression profiles which hence, may belong to a detoxification pathway that is active in different resistant wheat cultivars as well as in barley. Our qPCR expression analyses of seven wheat genes associated with the suppression of fungal virulence factors have demonstrated similar FHB-responsive inductions in the cultivars Dream and Sumai 3. Moreover, an earlier first induction and a steady-state level of expression were found to be associated with FHB resistance, while FHB-responsive gene expression in susceptible cultivars was typically late and temporary.
These results will help not only to understand changes in overall gene expression in wheat during Fusarium infection, but will also help to identify potential targets for development of disease control strategies. In fact, genes interesting for further investigations in this direction were identified in both wheat defence mechanisms. These are, nsLTP (Ta.7843.1.S1_a_at), defensin (Ta.20930.1.S1_at) and mJRP (TaAffx.7388.1.S1_at) genes as well as the PDR-transporter gene TaMDR1 (Ta.2793.1.S1_at), the UGT gene HvUGT13248 (Ta.12887.1.S1_at) and the putative serine-protease inhibitor gene Ta.22614.1.S1_at. The last three genes have shown regulations in response to FHB in the cultivars Dream and Sumai 3. In general, the identification of resistance candidate genes that are commonly active in different resistant wheat and barley cultivars is an important result with regard to the development of novel strategies against FHB severity and grain toxin contamination.
Plant and fungal material, inoculations and sampling
Plant material: Four wheat genotypes with contrasting levels of FHB resistance were used in this study: the German cultivar Dream (Disponent/Kronjuwel//Monopol/3/Orestis), the British cv. Lynx (CWW-44442-64/Redezvous), the Chinese cv. Sumai 3 (Funo/Taiwan wheat) and the French cv. Florence-Aurore (Florence/Aurore). The winter wheats Dream and Lynx are moderately resistant and susceptible, respectively and inoculated samples were used for both microarray analysis and quantitative real-time PCR (qPCR) based expression analysis. The spring types Sumai 3 and Florence-Aurore are highly resistant and highly susceptible, respectively; and inoculated samples were solely used for qPCR expression analyses.
Inoculum production: Macroconidia of the single-spore F. graminearum isolate ‘IFA 65’ (IFA Tulln, Austria) were grown on synthetic nutrient agar medium ‘Spezieller Nährstoffarmer Agar (SNA)’ at 20 °C under cool-white and near-UV light illumination. After seven days macroconidia were collected by centrifugation and washed in double-distilled water. For the inoculations 10 ml stock solutions (1x105 macroconidia ml-1) of the inoculum were stored at −80°C until use.
Inoculation and sampling: Dream and Lynx wheat plants were grown in the greenhouse. After vernalisation at 4°C for eight weeks with a 16/8 h day/night light regime, plants were cultivated at day/ night temperatures of 22/18°C with a photoperiod of 16/8 h (day/night). At early anthesis single floret inoculation with the F. graminearum strain ‘IFA 65’ was carried out by pipetting 10 μl of the fungal suspension (5 x 104 macroconidia ml-1) between the palea and lemma of each floret. Control (mock) plants were inoculated with distilled water instead of the macroconidia suspension. Eight florets per spike were inoculated. Greenhouse day temperature was increased to 24°C to ensure optimum infection conditions. Tissues of inoculated florets (lemma, palea) and a part of the attached rachis of Dream and Lynx spikes were collected. Six plants per genotype/treatment/timepoint were sampled. Samples were immediately frozen in liquid nitrogen and stored at −80°C. For the microarray analysis three replications were made for each inoculation treatment and samples were collected at 32 and 72 h after inoculation (hai). For the qPCR analysis samples were collected at 8, 24, 32, 48, 72, and 96 hai.
Sumai 3 and Florence-Aurore wheat plants were grown under open air conditions. At early anthesis, spikes were spray inoculated with 2 ml of the F. graminearum macroconidia suspension (1 x 105 macroconidia ml-1) or distilled water (mock inoculation) according to. For qPCR analysis whole spikes (one spike per single plant) of treated cv. Sumai 3 and cv. Florence-Aurore plants were collected at 0, 8, 32, 48, 72, 96, 120 and 336 hai. Four plants per genotype/ treatment/ timepoint were sampled. All samples were immediately frozen in liquid nitrogen and stored at −80°C.
RNA extraction and cDNA synthesis
For cv. Dream and cv. Lynx, floret tissue of six wheat heads per genotype, treatment and sampling timepoint were pooled prior to RNA extraction in order to reduce the biological variation between the samples. Accordingly, for cv. Sumai 3 and cv. Florence-Aurore spike tissue of four wheat plants per genotype, treatment and sampling timepoint were pooled prior to RNA extraction.
Total RNA was extracted from fine ground samples using the guanidinium thiocyanate-phenol-chloroform method as described by. Subsequently, a DNase (DNase I, RNase-free, Fermentas) digest was performed according to manufacturer’s instructions. RNA was further purified using phenol-chloroform extraction. RNA quantity and quality were evaluated using ND-1000 spectrophotometer (NanoDrop) measurement and agarose (NEEO Ultra Qualität, Roth, 1.5%) gel electrophoresis. cDNA was synthesised with 1.2 μg total RNA and 0.5 μg oligo(dT)18 primers using the RevertAidTM H Minus First Strand cDNA Synthesis Kit (Fermentas, Germany) according to manufacturer’s instructions. cDNA quantity and quality were evaluated using ND-1000 spectrophotometer (NanoDrop, USA) measurement.
The Affymetrix Wheat Genome GeneChip® Array (Affymetrix Inc., USA) was used to measure the gene expression changes within the bulked RNA samples of cv. Dream and cv. Lynx. RNA labelling and microarray hybridisation were performed according to the Affymetrix technical manual at the Max Planck Institute for Terrestrial Microbiology, Marburg, Germany. The following wheat samples were analysed (1) cv. Dream, F. graminearum-inoculated, 32 hai; (2) cv. Dream, mock-inoculated, 32 hai; (3) cv. Dream, F. graminearum-inoculated, 72 hai; (4) cv. Dream, mock-inoculated, 72 hai; (5) cv. Lynx, F. graminearum-inoculated, 32 hai; (6) cv. Lynx, mock-inoculated, 32 hai; (7) cv. Lynx, F. graminearum-inoculated, 72 hai; and (8) cv. Lynx, mock-inoculated, 72 hai. Three biological replications per genotype/treatment/timepoint were performed. Gene expression intensities were extracted from the scanned GeneChip images, data analysis was performed using the Bioconductor packages "affy", "gcRMA" and "limma" within the R environment. Data were preprocessed using the affy package and normalised by the gcRMA method. The limma package was used for the analysis of differentially expressed genes. Genes with an absolute t-value >1.96 that were at least two-fold regulated were selected as differentially expressed genes. Such genes were assigned as ‘induced’ or ‘repressed’.
To identify enriched gene ontology terms, a gene set enrichment analysis was carried out using the GSEA (Gene Set Enrichment analysis) platform. The gene ontology annotations were received by using Blast2GO. Significant enriched gene sets were selected based on a FDR < 25% and a gene set size > 15.
The following publicly available databases were considered for functional annotations: PLEXdb (Gene expression resource for plants and plant pathogens), NCBI (National Center for Biotechnology Information), RGAP 6.1 (Rice Genome Annotation Project), TAIR (The Arabidopsis Information Resource), the Gene Ontology Database, the Fusarium Comparative Database and the MIPS Fusarium graminearum Genome Database (MIPS). Generally, a homology was considered as a significant hit according to a threshold at an e-value of ≤1e-20 and a sequence identity of ≥70% in a sequence segment of at least 100 nucleotides for all BLAST analyses.
Quantitative real-time PCR (qPCR) assay
The qPCR expression analyses for selected genes were realised using the 7500 Fast Real-Time System with its corresponding software 7500 v2.0.4 (Applied Biosystems Inc., Foster City, USA). Each reaction contained 5 μl Power SYBR® Green Master Mix (Applied Biosystems Inc., Foster City, USA), 4 ng cDNA, 1 μM of both forward and reverse primer in a final volume of 10 μl. The following thermal profile was used: 2 min at 50°C; 10 min at 94°C; 45 cycles of 45 s at 94°C, 45 s at annealing temperature 60 to 62°C, and 45 s at 72°C. All cDNA samples of each treatment were amplified simultaneously in one PCR plate. After the final PCR cycle, a melting curve analysis was conducted to determine the specificity of the reaction.
Target gene expression was quantified using the comparative 2-ΔΔCt method. The efficiency of each primer pair was determined using 10-fold cDNA dilution series in order to reliable determine the fold changes. The expression of each target gene is presented as fold change normalised to the reference gene ubiquitin (Ta.28553.1.S1_s_at) and relative to the untreated control sample (mock).
Primers for qPCR were designed using the Primer3Plus software based on published EST and gene sequences. Primer sequences together with the used respective EST and gene accession numbers are listed in Additional file4.
Chromosomal localisation of the gene TaMDR1 in wheat
A set of nullisomic-tetrasomic lines (2n = 42) of the spring wheat cultivar Chinese Spring obtained from the Wheat Genetic and Genomic Resources Center, Kansas State University were used to determine the chromosomal location of the TaMDR1 gene in wheat. Primers designed for qPCR analysis were used for TaMDR1 gene amplification (Additional file4).
Buerstmayr H, Lemmens M, Schmolke M, Zimmermann G, Hartl L, Mascher F, Trottet M, Gosman NE, Nicholson P: Multi-environment evaluation of level and stability of FHB resistance among parental lines and selected offspring derived from several European winter wheat mapping populations. Plant Breed. 2008, 127: 325-332. 10.1111/j.1439-0523.2008.01507.x.
McMullen M, Jones R, Gellenberg D: Scab of wheat and barley: a re-emerging disease of devastating impact. Plant Dis. 1997, 81: 1340-1348. 10.1094/PDIS.1918.104.22.1680.
Buerstmayr H, Ban T, Anderson JA: QTL mapping and marker-assisted selection for Fusarium head blight resistance in wheat: a review. Plant Breed. 2009, 128: 1-26. 10.1111/j.1439-0523.2008.01550.x.
Lulin M, Yi S, Aizhong C, Zengjun Q, Liping X, Peidu C, Dajun L, Xiu-e W: Molecular cloning and characterization of an up-regulated UDP-glucosyltransferase gene induced by DON from Triticum aestivum L. cv. Wangshuibai. Mol Biol Rep. 2010, 37: 785-795.
Walter S, Nicholson P, Doohan FM: Action and reaction of host and pathogen during Fusarium head blight disease. New Phytol. 2010, 185: 54-66. 10.1111/j.1469-8137.2009.03041.x.
Pekkarinen AI, Jones BL: Purification and identification of barley (Hordeum vulgare L.) proteins that inhibit the alkaline serine proteinases of Fusarium culmorum. J Agric Food Chem. 2003, 51: 1710-1717. 10.1021/jf026035v.
Boenisch MJ, Schaefer W: Fusarium graminearum forms mycotoxin producing infection structures on wheat. BMC plant biology. 2011, 11: 110-10.1186/1471-2229-11-110.
Seong KY, Pasquali M, Zhou X, Song J, Hilburn K, McCormick S, Dong Y, Xu JR, Kistler HC: Global gene regulation by Fusarium transcription factors Tri6 and Tri10 reveals adaptation for toxin biosynthesis. Mol Microbiol. 2009, 72: 354-367. 10.1111/j.1365-2958.2009.06649.x.
Brown NA, Bass C, Baldwin TK, Chen H, Massot F, Carion PWC, Urban M, Allison Meene AML, Hammond-Kosack KE: Characterisation of the Fusarium graminearum-Wheat Floral Interaction. Journal of Pathogens. 2011, 10.4061/2011/626345.
Maier FJ, Miedaner T, Hadeler B, Felk A, Salomon S, Lemmens M, Kassner H, Schäfer W: Involvement of trichothecenes in fusarioses of wheat, barley and maize evaluated by gene disruption of the trichodiene synthase (Tri5) gene in three field isolates of different chemotype and virulence. Mol Plant Pathol. 2006, 7: 449-461. 10.1111/j.1364-3703.2006.00351.x.
Bai GH, Desjardins AE, Plattner RD: Deoxynivalenol-nonproducing Fusarium graminearum causes initial infection, but does not cause disease spread in wheat spikes. Mycopathologia. 2002, 153: 91-98. 10.1023/A:1014419323550.
Proctor RH, Holm TM, McCormick SP: Reduced virulence of Gibberella zeae caused by disruption of a trichothecene toxin biosynthetic gene. Mol Plant Microbe Interact. 1995, 8: 593-601. 10.1094/MPMI-8-0593.
Kang Z, Buchenauer H: Immunocytochemical localization of Fusarium toxins in infected wheat spikes by Fusarium culmorum. Physiol Mol Plant Pathol. 1999, 55: 275-288. 10.1006/pmpp.1999.0233.
Kimura M, Kaneko I, Komiyama M, Takatsuki A, Koshino H, Yoneyama K, Yamaguchi I: Trichothecene 3-O-acetyltransferase protects both the producing organism and transformed yeast from related mycotoxins. Cloning and characterization of Tri101. J Biol Chem. 1998, 273: 1654-1661. 10.1074/jbc.273.3.1654.
Ilgen P, Hadeler B, Maier FJ, Schäfer W: Developing kernel and rachis node induce the trichothecene pathway of Fusarium graminearum during wheat head infection. Mol Plant Microbe Interact. 2009, 22: 899-908. 10.1094/MPMI-22-8-0899.
Cuzick A, Urban M, Hammond Kosack K: Fusarium graminearum gene deletion mutants map1 and tri5 reveal similarities and differences in the pathogenicity requirements to cause disease on Arabidopsis and wheat floral tissue. New Phytol. 2008, 177: 990-1000. 10.1111/j.1469-8137.2007.02333.x.
Brown NA, Urban M, van de Meene AM, Hammond-kosack KE: The infection biology of Fusarium graminearum: Defining the pathways of spikelet to spikelet colonisation in wheat ears. Fungal Biology. 2010, 114: 555-571. 10.1016/j.funbio.2010.04.006.
Jansen C, von Wettstein D, Schäfer W, Kogel KH, Felk A, Maier FJ: Infection patterns in barley and wheat spikes inoculated with wild-type and trichodiene synthase gene disrupted Fusarium graminearum. PNAS. 2005, 102: 16892-16897. 10.1073/pnas.0508467102.
Pekkarinen AI, Longstaff C, Jones BL: Kinetics of the inhibition of Fusarium serine proteinases by barley (Hordeum vulgare L.) inhibitors. J Agric Food Chem. 2007, 55: 2736-2742. 10.1021/jf0631777.
Jackowiak H, Packa D, Wiwart M, Perkowski J, Buśko M, Borusiewicz A: Scanning electron microscopy of mature wheat kernels infected with Fusarium culmorum. J Appl Genet. 2002, 43A: 167-176.
Olivieri F, Zanetti ME, Oliva CR, Covarrubias AA, Casalongué CA: Characterization of an extracellular serine protease of Fusarium eumartii and its action on pathogenesis related proteins. Eur J Plant Pathol. 2002, 108: 63-72. 10.1023/A:1013920929965.
Wang Y, Yang LM, Xu HB, Li QF, Ma ZQ, Chu CG: Differential proteomic analysis of proteins in wheat spikes induced by Fusarium graminearum. Proteomics. 2005, 5: 4496-4503. 10.1002/pmic.200401317.
Boddu J, Cho S, Kruger WM, Muehlbauer GJ: Transcriptome analysis of the barley–Fusarium graminearum interaction. Mol Plant Microbe Interact. 2006, 19: 407-417. 10.1094/MPMI-19-0407.
Pekkarinen AI, Jones BL: Trypsin-like proteinase produced by Fusarium culmorum grown on grain proteins. J Agric Food Chem. 2002, 50: 3849-3855. 10.1021/jf020027x.
Agrios GN: Plant Pathology. 1997, London: Academic, 635-4th
Chen LF, Song YL, Xu YG: Variations in the concentrations of deoxynivalenol in the spikes of winter wheat infected by Fusarium graminearum Schw. Acta Phys Plants. 1996, 26: 25-28.
Savard ME, Sinha RC, Seaman WL, Fedak G: Sequential distribution of the mycotoxin deoxynivalenol in wheat spike after inoculation with Fusarium graminearum. Can J Plant Pathol. 2000, 22: 280-285. 10.1080/07060660009500476.
Güldener U, Seong K-Y, Boddu J, Cho S, Trail F, Xu J-R, Adam G, Mewes H-W, Muehlbauer GJ, Kistler HC: Development of a Fusarium graminearum Affymetrix GeneChip for profiling fungal gene expression in vitro and in planta. Fungal genetics and biology. 2006, 43: 316-325. 10.1016/j.fgb.2006.01.005.
Stein JM, Osborne LE, Bondalapati KD, Glover KD, Nelson CA: Fusarium Head Blight severity and deoxynivalenol concentration in wheat in response to Gibberella zeae inoculum concentration. Phytopathology. 2009, 99: 759-764. 10.1094/PHYTO-99-6-0759.
Phalip V, Delalande F, Carapito C, Goubet F, Hatsch D, Leize-Wagner E, Dupree P, Dorsselaer AV, Jeltsch J-M: Diversity of the exoproteome of Fusarium graminearum grown on plant cell wall. Curr Genet. 2005, 48: 366-379. 10.1007/s00294-005-0040-3.
Desmond OJ, Manners JM, Stephens AE, Maclean DJ, Schenk PM, Gardiner DM, Munn AL, Kazan K: The Fusarium mycotoxin deoxynivalenol elicits hydrogen peroxide production, programmed cell death and defence responses in wheat. Mol Plant Pathol. 2008, 9: 435-445. 10.1111/j.1364-3703.2008.00475.x.
Masuda D, Ishida M, Yamaguchi K, Yamaguchi I, Kimura M, Nishiuchi T: Phytotoxic effects of trichothecenes on the growth and morphology of Arabidopsis thaliana. J Exp Bot. 2007, 58: 1617-1626. 10.1093/jxb/erl298.
Wu F, Munkvold GP: Mycotoxins in ethanol co-products: modeling economic impacts on the livestock industry and management strategies. J Agric Food Chem. 2008, 56: 3900-3911. 10.1021/jf072697e.
Jackowiak H, Packa D, Wiwart M, Perkowski J: Scanning electron microscopy of Fusarium damaged kernels of spring wheat. International J Food Microbiol. 2005, 98: 113-123. 10.1016/j.ijfoodmicro.2004.05.014.
Wang J, Wieser H, Pawelzik E, Weinert J, Keutgen AJ, Wolf GA: Impact of the fungal protease produced by Fusarium culmorum on the protein quality and breadmaking properties of winter wheat. Eur Food Res Technol. 2005, 220: 552-559. 10.1007/s00217-004-1112-1.
Eriksen GS, Pettersson H: Toxicological evaluation of trichothecenes in animal feed. Anim Feed Sci Technol. 2004, 114: 205-239. 10.1016/j.anifeedsci.2003.08.008.
Subramanian A, Tamayo P, Mootha VK, Mukherjee S, Ebert BL, Gillette MA, Paulovich A, Pomeroy SL, Golub TR, Lander ES, Mesirov JP: Gene set enrichment analysis: a knowledge-based approach for interpreting genome-wide expression profiles. PNAS. 2005, 102: 15545-15550. 10.1073/pnas.0506580102.
Van Loon LC, Rep M, Pieterse CMJ: Significance of inducible defense-related proteins in infected plants. Annu Rev Phytopathol. 2006, 44: 135-162. 10.1146/annurev.phyto.44.070505.143425.
Xia Y: Proteases in pathogenesis and plant defence. Cell Microbiol. 2004, 6: 905-913. 10.1111/j.1462-5822.2004.00438.x.
Lee JR, Park SC, Kim JY, Lee SS, Parkc Y, Cheonga GW, Hahm KS, Lee SY: Molecular and functional characterization of a cyclophilin with antifungal activity from Chinese cabbage. Biochem and Biophys Res Communications. 2007, 353: 672-678. 10.1016/j.bbrc.2006.12.102.
Ye XY, Ng TB: Isolation of a new cyclophilin-like protein from chickpeas with mitogenic, antifungal and anti-HIV-1 reverse transcriptase activities. Life Sci. 2002, 70: 1129-1138. 10.1016/S0024-3205(01)01473-4.
Shin S, Mackinosh CA, Lewis J, Heinen SJ, Radmer L, Dill-Macky R, Baldridge GD, Zeyen RJ, Muehlbauer GJ: Transgenic wheat expressing a barley class II chitinase gene has enhanced resistance against Fusarium graminearum. J Exp Bot. 2008, 59: 2371-2378. 10.1093/jxb/ern103.
Eggert K, Zörb C, Mühling KH, Pawelzik E: Proteome analysis of Fusarium infection in emmer grains (Triticum dicoccum). Plant Pathol. 2011, 60: 918-928. 10.1111/j.1365-3059.2011.02442.x.
Li G, Yen Y: Jasmonate and ethylene signaling pathway may mediate Fusarium head blight resistance in wheat. Crop Sci. 2008, 48: 1888-1896. 10.2135/cropsci2008.02.0097.
Prost I, Dhondt S, Rothe G, Vicente J, Rodriguez MJ, Kift N, Carbonne F, Griffiths G, Esquerre-Tugaye M-T, Rosahl S, Castresana C, Hamberg M, Fournier J: Evaluation of the antimicrobial activities of plant oxylipins supports their involvement in defense against pathogens. Plant Physiol. 2005, 139: 1902-1913. 10.1104/pp.105.066274.
Feussner I, Wasternack C: The lipoxygenase pathway. Annu Rev Plant Biol. 2002, 53: 275-297. 10.1146/annurev.arplant.53.100301.135248.
Robert-Seilaniantz A, Navarro L, Bari R, Jones JDG: Pathological hormone imbalances. Current Opinion in Plant Biology. 2007, 10: 372-379. 10.1016/j.pbi.2007.06.003.
Glazebrook J: Contrasting mechanisms of defense against biotrophic and necrotrophic pathogens. Annu Rev Phytopathol. 2005, 43: 205-227. 10.1146/annurev.phyto.43.040204.135923.
Blée E: Impact of phyto-oxylipins in plant defense. Trends Plant Sci. 2002, 7: 315-322. 10.1016/S1360-1385(02)02290-2.
Turner JG, Ellis C, Devoto A: The jasmonate signal pathway. The Plant Cell. 2002, 14: S153-S164.
Wasternack C: Jasmonates: an update on biosynthesis, signal transduction and action in plant stress response, growth and development. Ann Bot. 2007, 100: 681-697. 10.1093/aob/mcm079.
Gao X, Stumpe M, Feussner I, Kolomiets M: A novel plastidial lipoxygenase of maize (Zea mays) ZmLOX6 encodes for a fatty acid hydroperoxide lyase and is uniquely regulated by phytohormones and pathogen infection. Planta. 2008, 227: 491-503.
Seo HS, Song JT, Cheong JJ, Lee YH, Lee YW, Hwang I, Lee JS, Choi YD: Jasmonic acid carboxyl methyltransferase: a key enzyme for jasmonate-regulated plant responses. PNAS USA. 2001, 98: 4788-4793. 10.1073/pnas.081557298.
Mussig C, Biesgen C, Lisso J, Uwer U, Weiler EW, Altmann T: A novel stress-inducible 12-oxophytodienoate reductase from Arabidopsis thaliana provides a potential link between Brassinosteroid-action and Jasmonic-acid synthesis. J Plant Physiol. 2000, 157: 143-152. 10.1016/S0176-1617(00)80184-4.
Laudert D, Weiler EW: Allene oxide synthase: a major control point in Arabidopsis thaliana octadecanoid signalling. The Plant J. 1998, 15: 675-684. 10.1046/j.1365-313x.1998.00245.x.
Bachmann A, Hause B, Maucher H, Garbe E, Vörös K, Weichert H, Wasternack C, Feussner I: Jasmonate-induced lipid peroxidation in barley leaves initiated by distinct 13-LOX forms of chloroplasts. Biol Chem. 2002, 383: 1645-1657.
Ding L, Xu H, Yi H, Yang L, Kong Z, Zhand L, Xue S, Jia H: Resistance to hemi-biotrophic F. graminearum infection is associated with coordinated and ordered expression of diverse defense signaling pathways. PLoS One. 2011, 6: e19008-10.1371/journal.pone.0019008.
Ellis C, Karafyllidis I, Wasternack C, Turner JG: The Arabidopsis Mutant cev1 Links Cell Wall Signaling to Jasmonate and Ethylene Responses. Society. 2002, 14: 1557-1566.
Thomma BP, Eggermont K, Penninckx IA, Mauch-Mani B, Vogelsang R, Cammue BP, Broekaert WF: Separate jasmonate-dependent and salicylate-dependent defense-response pathways in Arabidopsis are essential for resistance to distinct microbial pathogens. PNAS USA. 1998, 95: 15107-15111. 10.1073/pnas.95.25.15107.
Park CJ, Shin R, Park JM, Lee GJ, You JS, Paek KH: Induction of pepper cDNA encoding a lipid transfer protein during the resistance response to tobacco mosaic virus. Plant Mol Biol. 2002, 48: 243-254. 10.1023/A:1013383329361.
Cammue BP, Thevissen K, Hendriks M, Eggermont K, Goderis IJ, Proost P, Van Damme J, Osborn RW, Guerbette F, Kader JC: A potent antimicrobial protein from onion seeds showing sequence homology to plant lipid transfer proteins. Plant Physiol. 1995, 109: 445-455. 10.1104/pp.109.2.445.
Molina A, Segura A, García-Olmedo F: Lipid transfer proteins (nsLTPs) from barley and maize leaves are potent inhibitors of bacterial and fungal plant pathogens. FEBS Lett. 1993, 316: 119-122. 10.1016/0014-5793(93)81198-9.
Sun JY, Gaudet DA, Lu ZX, Frick M, Puchalski B, Laroche A: Characterization and antifungal properties of wheat nonspecific lipid transfer proteins. Mol Plant Microbe Interact. 2008, 21: 346-360. 10.1094/MPMI-21-3-0346.
Regente MC, Giudici a M, Villalaín J, de la Canal L: The cytotoxic properties of a plant lipid transfer protein involve membrane permeabilization of target cells. Lett Appl Microbiol. 2005, 40: 183-189. 10.1111/j.1472-765X.2004.01647.x.
Molina A, Garcia-Olmedo F: Developmental and pathogen induced expression of three barley genes encoding lipid transfer proteins. Plant J. 1993, 4: 983-991. 10.1046/j.1365-313X.1993.04060983.x.
Kader JC: Lipid-Transfer Proteins in Plants. Annual review of plant physiology and plant molecular biology. 1996, 47: 627-654. 10.1146/annurev.arplant.47.1.627.
Castagnaro A, Maraia C, Carbonero P, García-Olmedo F: cDNA cloning and nucleotide sequences of α1 and α2 thionins from hexaploid wheat endosperm. Plant Physiol. 1994, 106: 1221-1222. 10.1104/pp.106.3.1221.
Oh BJ, Ko MK, Kostenyuk I, Shin B, Sang Kim KS: Coexpression of a defensin gene and a thionin-like gene via different signal transduction pathways in pepper and Colletotrichum gloeosporioides interactions. Plant Mol Biol. 1999, 41: 313-319. 10.1023/A:1006336203621.
Epple P, Apel K, Bohlmann H: An Arabidopsis thaliana thionin gene is inducible via a signal transduction pathway different from that for pathogenesis-related proteins. Plant Physiol. 1995, 109: 813-820. 10.1104/pp.109.3.813.
Koike M, Okamoto T, Tsuda S, Imai R: A novel plant defensin-like gene of winter wheat is specifically induced during cold acclimation. Biochem Biophys Res Commun. 2002, 298: 46-53. 10.1016/S0006-291X(02)02391-4.
Kovalchuk N, Li M, Wittek F, Reid N, Singh R, Shirley N, Ismagul A, Eliby S, Johnson A, Milligan AS, Hrmova M, Langridge P, Lopato S: Defensin promoters as potential tools for engineering disease resistance in cereal grains. Plant biotechnology journal. 2010, 8: 47-64. 10.1111/j.1467-7652.2009.00465.x.
Silverstein KAT, Graham MA, Paape TD, Vandenbosch KA: Genome Organization of More Than 300 Defensin-Like Genes in Arabidopsis. Plant Physiol. 2005, 138: 600-610. 10.1104/pp.105.060079.
McMullen M, Halley S, Schatz B, Meyer S, Jordahl J, Ransom J: Integrated strategies for Fusarium head blight management in the United States. Cereal Res Commun. 2008, 36: 563-568. 10.1556/CRC.36.2008.Suppl.B.45.
Lay FT, Anderson MA: Defensins-components of the innate immune system in plants. Curr Protein Pept Sci. 2005, 6: 85-101. 10.2174/1389203053027575.
Marshall E, Costa LM, Gutierrez-Marcos J: Cysteine-rich peptides (CRPs) mediate diverse aspects of cell-cell communication in plant reproduction and development. J Exp Bot. 2011, 62: 1677-1686. 10.1093/jxb/err002.
Silverstein KA, Moskal WA, Wu HC, Underwood BA, Graham MA, Town CD, VandenBosch KA: Small cysteine- rich peptides resembling antimicrobial peptides have been under-predicted in plants. The Plant Journal. 2007, 51: 262-280. 10.1111/j.1365-313X.2007.03136.x.
Castro MS, Fontes W: Plant defense and antimicrobial peptides. Protein Pept Lett. 2005, 12: 13-18.
Poland JA, Balint-Kurti PJ, Wisser RJ, Pratt RC, Nelson RJ: Shades of gray: the world of quantitative disease resistance. Trends Plant Sci. 2009, 14: 21-29. 10.1016/j.tplants.2008.10.006.
Van Loon LC, Van Strien EA: The families of pathogenesis-related proteins, their activities, and comparative analysis of PR-1 type proteins. Physiol Mol Plant Pathol. 1999, 55: 85-97. 10.1006/pmpp.1999.0213.
Wasternack C, Parthier B: Jasmonate-signalled plant gene expression. Trends Plant Sci. 1997, 2: 302-307. 10.1016/S1360-1385(97)89952-9.
Tian Q, Wang W, Miao C, Peng H, Liu B, Leng F, Dai L, Chen F, Bao J: Purification, characterization and molecular cloning of a novel mannose-binding lectin from rhizomes of Ophiopogon japonicus with antiviral and antifungal activities. Plant Science. 2008, 175: 877-884. 10.1016/j.plantsci.2008.09.008.
Wang XM, Ma QH: Characterization of a jasmonate-regulated wheat protein related to a beta-glucosidase-aggregating factor. Plant Physiol Biochem. 2005, 43: 185-192. 10.1016/j.plaphy.2005.01.018.
Kittur FS, Yu HY, Bevan DR, Esen A: Deletion of the N-terminal dirigent domain in maize beta-glucosidase aggregating factor and its homolog sorghum lectin dramatically alters the sugar-specificities of their lectin domains. Plant Physiol Biochem. 2010, 48: 731-734. 10.1016/j.plaphy.2010.03.007.
Ma QH, Tian B, Li YL: Overexpression of a wheat jasmonate-regulated lectin increases pathogen resistance. Biochimie. 2010, 92: 187-193. 10.1016/j.biochi.2009.11.008.
Görlach J, Volrath S, Knauf-Beiter G, Hengy G, Beckhove U, Kogel KH, Oostendorp M, Staub T, Ward E, Kessmann H, Ryals J: Benzothiadiazole, a novel class of inducers of systemic acquired resistance, activates gene expression and disease resistance in wheat. The Plant cell. 1996, 8: 629-643.
Yu GY, Muehlbauer GJ: Benzothiadiazole-induced gene expression in wheat spikes does not provide resistance to Fusarium head blight. Physiol Mol Plant Pathol. 2001, 59: 129-136. 10.1006/pmpp.2001.0348.
Subramanyam S, Sardesai N, Puthoff D, Meyer J, Nemacheck J, Gonzalo M, Williams C: Expression of two wheat defense-response genes, Hfr-1 and Wci-1, under biotic and abiotic stresses. Plant Science. 2006, 170: 90-103. 10.1016/j.plantsci.2005.08.006.
Ralph S, Park JY, Bohlmann J, Mansfield SD: Dirigent proteins in conifer defense: gene discovery, phylogeny, and differential wound- and insect-induced expression of a family of DIR and DIR-like genes in spruce (Picea spp.). Plant Mol Biol. 2006, 60: 21-40. 10.1007/s11103-005-2226-y.
Bertini L, Proietti S, Caporale C, Caruso C: Molecular characterization of a wheat protein induced by vernalisation. Protein J. 2009, 28: 253-262. 10.1007/s10930-009-9190-3.
Wang KL, Li H, Ecker JR: Ethylene Biosynthesis and Signaling Networks. Plant Cell. 2002, 14: S131-S151.
Mathooko FM, Tsunashima Y, Kubo Y, Inaba A: Expression of a 1-aminocyclopropane-1-carboxylate (ACC) oxidase gene in peach (Prunus persica L.) fruit in response to treatment with carbon dioxide and 1-methylcyclopropene: possible role of ethylene. Afr J Biotechnol. 2004, 3: 497-502.
Kwon SJ, Jin HC, Lee S, Nam MH, Chung JH, Kwon SI, Ryu C-M, Park OK: GDSL lipase-like 1 regulates systemic resistance associated with ethylene signaling in Arabidopsis. Plant J. 2009, 58: 235-245. 10.1111/j.1365-313X.2008.03772.x.
Koornneef A, Pieterse CMJ: Cross talk in defense signaling. Plant Physiol. 2008, 146: 839-844. 10.1104/pp.107.112029.
Shan XC, Goodwin PH: Silencing an ACC oxidase gene affects the susceptible host response of Nicotiana benthamiana to infection by Colletotrichum orbiculare. Plant cell reports. 2006, 25: 241-247. 10.1007/s00299-005-0063-8.
Asai T, Stone JM, Heard JE, Kovtun Y, Yorgey P, Sheen J, Ausubel FM: Fumonisin B1-induced cell death in Arabidopsis protoplasts requires jasmonate-, ethylene-, and salicylate-dependent signaling pathways. Plant Cell. 2000, 12: 1823-1835.
Nightingale MJ, Marchylo BA, Clear RM, Dexter JE, Preston KR: Fusarium head blight: effect of fungal proteases on wheat storage proteins. Cereal Chemistry. 1999, 76: 150-158. 10.1094/CCHEM.1922.214.171.124.
Page MJ, Cera ED: Serine Proteases and Serine Protease Inhibitors. Wiley Encyclopedia of Chemical Biology. 2008, 1-29. 10.1002/9780470048672.wecb534.
Shan L, Li C, Chen F, Zhao C, Xia G: A Bowman-Birk type protease inhibitor is involved in the tolerance to salt stress in wheat. Plant Cell Environ. 2008, 31: 1128-1137. 10.1111/j.1365-3040.2008.01825.x.
Badea A, Eudes F, Graf RJ, Laroche A, Gaudet DA, Sadasivaiah RS: Phenotypic and marker-assisted evaluation of spring and winter wheat germplasm for resistance to fusarium head blight. Euphytica. 2008, 164: 803-819. 10.1007/s10681-008-9735-0.
Schmolke M, Zimmermann G, Buerstmayr H, Schweizer G, Miedaner T, Korzun V, Ebmeyer E, Hartl L: Molecular mapping of Fusarium head blight resistance in the winter wheat population Dream/Lynx. Theor Appl Genet. 2005, 111: 747-756. 10.1007/s00122-005-2060-2.
Roberts TH, Hejgaard J: Serpins in plants and green algae. Functional & integrative genomics. 2008, 8: 1-27. 10.1007/s10142-007-0059-2.
Ryan CA: PROTEASE INHIBITORS IN PLANTS : Genes for Improving Defenses Against Insects and Pathogens. Annu Rev Phytopathol. 1990, 28: 425-449. 10.1146/annurev.py.28.090190.002233.
Bushnell WR, Hayen BE, Pritsch C: Histology and physiology of Fusarium head blight. Fusarium Head Blight of Wheat and Barley. Edited by: Leonard KJ, Bushnell WR. 2003, St. Paul, MN, USA: American Phytopathological Society, 44-83.
Habib H, Fazili KM: Plant protease inhibitors: a defense strategy in plants. Mol Biol. 2007, 2: 068-085.
Rocha O, Ansari K, Doohan FM: Effects of trichothecene mycotoxins on eukaryotic cells: a review. Food Addit Contam. 2005, 22: 369-378. 10.1080/02652030500058403.
Boddu J, Cho S, Muehlbauer GJ: Transcriptome analysis of trichothecene-induced gene expression in barley. Mol Plant Microbe Interact. 2007, 20: 1364-1375. 10.1094/MPMI-20-11-1364.
Ghaffari MR, Mardi M, Ehya F, Farsad LK: Mapping and expression analysis of a Fusarium head blight resistance gene candidate pleiotropic drug resistance 5 (PDR5) in wheat. Planta. 2010, 8: 112-116.
Shang Y, Xiao J, Ma L, Wang H, QI Z, Chen P, Liu D, Wang X: Characterization of a PDR type ABC transporter gene from wheat (Triticum aestivum L.). Chinese Sci Bull. 2009, 54: 3249-3257. 10.1007/s11434-009-0553-0.
Poppenberger B, Berthiller F, Lucyshyn D, Sieberer T, Schuhmacher R, Krska R, Kuchler K, Glössl J, Luschnig C, Adam G: Detoxification of the Fusarium mycotoxin deoxynivalenol by a UDP-glucosyltransferase from Arabidopsis thaliana. J Biol Chem. 2003, 278: 47905-47914. 10.1074/jbc.M307552200.
Sasaki T, Ezaki B, Matsumoto H: A gene encoding multidrug resistance (MDR)-like protein is induced by aluminum and inhibitors of calcium flux in wheat. Plant Cell Physiol. 2002, 43: 177-185. 10.1093/pcp/pcf025.
Postnikova OA, Minakova NY, Boutanaev AM, Nemchinov LG: Clustering of Pathogen-Response Genes in the Genome of Arabidopsis thaliana. Journal of Integrative Plant Biology. 2011, 53: 824-834. 10.1111/j.1744-7909.2011.01071.x.
Meriño-Gergichevich C, Alberdi M, Ivanov AG, Reyes-Díaz M: Al3+-Ca2+ Interaction in plants growing in acid soils: Al-phytotoxicity response to calcareous amendments. J Soil Sci Plant Nutr. 2010, 10: 217-243.
Peng SQ, Yang JS: Blocking effect of deoxynivalenol (DON) on calcium channels in cultured cardiomyocytes of rats. China Prev Med. 2004, 5: 241-243.
Karlovsky P: Biological detoxification of the mycotoxin deoxynivalenol and its use in genetically engineered crops and feed additives. Appl Microbiol Biotechnol. 2011, 91: 491-504. 10.1007/s00253-011-3401-5.
Schweiger W, Boddu J, Shin S, Poppenberger B, Berthiller F, Lemmens M, Muehlbauer GJ, Adam G: Validation of a candidate deoxynivalenol-inactivating UDP-glucosyltransferase from barley by heterologous expression in yeast. Mol Plant Microbe Interact. 2010, 23: 977-986. 10.1094/MPMI-23-7-0977.
Walter S, Brennan JM, Trognitz F, Trognitz B, Leonard G, Egan D, Doohan FM: Components of the gene network associated with genotype-dependent response of wheat to the Fusarium mycotoxin deoxynivalenol. Funct Integr Genomics. 2008, 8: 421-427. 10.1007/s10142-008-0089-4.
Gardiner SA, Boddu J, Berthiller F, Hametner C, Stupar R, Adam G, Muehlbauer GJ: Transcriptome analysis of the barley-deoxynivalenol interaction: Evidence for a role of glutathione in deoxynivalenol detoxification. Mol Plant Microbe Interact. 2010, 23: 962-976. 10.1094/MPMI-23-7-0962.
Zhang J, Simmons C, Yalpani N, Crane V, Wilkinson H, Kolomiets M: Genomic analysis of the 12-oxo-phytodienoic acid reductase gene family of Zea mays. Plant Mol Biol. 2005, 59: 323-343. 10.1007/s11103-005-8883-z.
Agrawal GK, Jwa NS, Shibato J, Han O, Iwahashi H, Rakwal R: Diverse environmental cues transiently regulate OsOPR1 of the “octadecanoid pathway” revealing its importance in rice defense/stress and development. Biochem Biophys Res Commun. 2003, 310: 1073-1082. 10.1016/j.bbrc.2003.09.123.
Schaller A: A cut above the rest: the regulatory function of plant proteases. Planta. 2004, 220: 183-197. 10.1007/s00425-004-1407-2.
Tian M, Huitema E, Da Cunha L, Torto-Alalibo T, Kamoun S: A Kazal-like extracellular serine protease inhibitor from Phytophthora infestans targets the tomato pathogenesis-related protease P69B. J Biol Chem. 2004, 279: 26370-26377. 10.1074/jbc.M400941200.
Lopez-Otin C, Overall CM: Protease degradomics: a new challenge for proteomics. Nat Rev Mol Cell Biol. 2002, 3: 509-519. 10.1038/nrm858.
Nirenberg H: Untersuchungen über die morphologische und biologische Differenzierung in der Fusariensektion Liseola. 1976, Forstwirtsch, Berlin-Dahlem: Mitt Biol Bundesanst Land- u, 1-117. 169th
Steiner B, Kurz H, Lemmens M, Buerstmayr H: Differential gene expression of related wheat lines with contrasting levels of head blight resistance after Fusarium graminearum inoculation. Theor Appl Genet. 2009, 118: 753-764. 10.1007/s00122-008-0935-8.
Buchenauer H, Kang Z: 13. Wissenschaftliche Fachtagung 7. November 2001: Fusarium-Befall und Mykotoxinbelastung von Getreide -Ursachen, Auswirkungen, Vermeidungsstrategien-. Bonn, Druck Center Meckenheim. Cytologische Studien zur Infektion und Ausbreitung von Fusarien in Weizenähren sowie zu Abwehrreaktionen in Ähren resistenter und anfälliger Weizensorten. 2002, 45-54.
Chomczynski P, Sacchi N: Single-step method of RNA isolation by acid guanidinium thiocyanate-phenol-chloroform extraction. Anal Biochem. 1987, 162: 156-159.
Sambrook J, Fritsch EF, Maniatis T: Molecular Cloning – A laboratory manual. 1989, New York: Cold Spring Harbor Laboratory Press, 2nd
Affymetrix Inc: GeneChip® Expression Analysis Technical Manual. 2005–2009, Santa Clara, CA, USA
Bioconductor packages. http://www.bioconductor.org/.
Gautier L, Cope L, Bolstad BM, Irizarry RA: affy-analysis of affymetrix genechip data at the probe level. Bioinformatics. 2004, 20: 307-315. 10.1093/bioinformatics/btg405.
Wu Z, Irizarry R, Gentlemen R, Martinez-Murillo F, Spencer F: A model-based background adjustment for oligonucleotide expression arrays. J Am Stat Assoc. 2004, 99: 909-917. 10.1198/016214504000000683.
Smyth GK: Linear models and empirical Bayes methods for assessing differential expression in microarray experiments. Stat Appl Genet Mol Biol. 2004, 3 (Article 3): 10.2202/1544-6115.1027.
GSEA platform. [http://www.broadinstitute.org/gsea/index.jsp]
RGAP 6.1. [http://rice.plantbiology.msu.edu].
Gene Ontology Database. [http://www.geneontology.org]
139.Fusarium Comparative Database. [http://www.broadinstitute.org/annotation/genome/Fusarium_group/MultiHome.html].
140.MIPS Fusarium graminearum Genome Database. [http://mips.helmholtz-muenchen.de/genre/proj/Fusarium/].
Michalek W, Weschke W, Pleissner K-P, Graner A: EST analysis in barley defines a unigene set comprising 4,000 genes. Theor Appl Genet. 2002, 104: 97-103. 10.1007/s001220200011.
Livak KJ, Schmittgen TD: Analysis of Relative Gene Expression Data Using Real- Time Quantitative PCR and the 2-ΔΔCT Method. Methods. 2001, 25: 402-408. 10.1006/meth.2001.1262.
Voros K, Feussner I, Kuhn H, Lee J, Graner A, Lobler M, Parthier B, Wasternack C: Characterization of a methyljasmonate-inducible lipoxygenase from barley (Hordeum vulgare cv. Salome) leaves. Eur J Biochem. 1998, 251: 36-44. 10.1046/j.1432-1327.1998.2510036.x.
Feng B, Dong Z, Xu Z, An X, Qin H, Wu N, Wang D, Wang T: Molecular analysis of lipoxygenase (LOX) genes in common wheat and phylogenetic investigation of LOX proteins from model and crop plants. J Cereal Sci. 2010, 52: 387-394. 10.1016/j.jcs.2010.06.019.
Handa H, Namiki N, Xu DH, Ban T: Dissecting of the FHB resistance QTL on the short arm of wheat chromosome 2D using a comparative genomic approach: from QTL to candidate gene. Mol Breed. 2008, 27: 71-84.
Bushnell WR, Seeland TM: Effects of DON on barley leaf tissues, summary of results. The Effects of Deoxynivalenol on Barley Leaf Tissue. Proceedings of the National Fusarium Head Blight Forum 10–12 December 2006. Edited by: Canty SM, Clark A, Sanford D. 2006, North Carolina, USA: Research Triangle Park, 35-36.
The authors thank Petra Kretschmer and Stavros Tzigos for excellent technical assistance and Markus Kolmer (Phytotron Facility, Field station Rauischholzhausen, Justus-Liebig University Giessen, Germany) for support during the cultivation of cultivars Sumai 3 and Florence-Aurore. We are grateful to Günther Schweizer and Manuela Diethelm (Bavarian State Research Center for Agriculture (LfL), Institute for Crop Science and Plant Breeding, Freising, Germany) for providing inoculated spike tissues of cultivars Dream and Lynx as well as substantial help, and Markus Rhiel for performing microarray hybridizations. We would like to thank Marc Lemmens (University of Natural Resources and Applied Life Sciences, Department for Agrobiotechnology, Vienna, Austria) for kindly providing the F. graminearum inoculum. Financial support of the project was provided by the Deutsche Forschungsgemeinschaft DFG (Schw 1201/1-2).
'The authors declare that they have no competing interests.
SG carried out the data analysis and interpretation, coordinated the experimental work and drafted the manuscript. BS performed the microarray data analysis and participated in writing the manuscript. SL assisted in the coordination of experimental work, performed qPCR analyses and helped to draft the manuscript. WF supervised the project, contributed to the project design and revised the manuscript. All authors read and approved the final manuscript.
Electronic supplementary material
Additional file 1: Table 1. Dream FHB-responsive genes categorised as defence related. Supplemental table showing 117 genes that are FHB-responsive induced or repressed in the resistant genotype Dream. Genes were revealed by transcriptome analysis using Affymetrix GeneChip Wheat Genome Array and assigned to 11 gene classes related to a defence response, as well as to the respective timepoints of differential expression. (DOC 212 KB)
Additional file 2: Table 2. Dream genotype-specific genes categorised as defence related. Supplemental table showing 173 constitutive Dream controlled genes. Genes were revealed by transcriptome analysis using Affymetrix GeneChip Wheat Genome Array and assigned to 11 gene classes related to a defence response, as well as to the respective timepoints of differential expression. (DOC 286 KB)
Additional file 3: Table 3. Dream 72 hai-specific genes categorised as defence related. Supplemental table showing 82 genes exclusively differential expressed at the sampling timepoint 72 hai. Genes were revealed by transcriptome analysis using Affymetrix GeneChip Wheat Genome Array and assigned to 11 gene classes related to a defence response, as well as to the respective timepoints of differential expression. (DOC 164 KB)
Additional file 4: Table 4. Sequences of primers used for qPCR analysis of gene expression. Supplemental table showing sequences of primers that were used for the qPCR assays. Accession numbers of Expressed sequence tags (ESTs) and genes that were used to design primers are listed as well. All primers were designed using Primer3Plus software. (DOC 36 KB)
About this article
Cite this article
Gottwald, S., Samans, B., Lück, S. et al. Jasmonate and ethylene dependent defence gene expression and suppression of fungal virulence factors: two essential mechanisms of Fusarium head blight resistance in wheat?. BMC Genomics 13, 369 (2012). https://doi.org/10.1186/1471-2164-13-369
- Jasmonic Acid
- Fusarium Head Blight
- Fusarium Head Blight Resistance
- nsLTP Gene