Open Access

Global transcriptional analysis suggests Lasiodiplodia theobromae pathogenicity factors involved in modulation of grapevine defensive response

  • Marcos Paolinelli-Alfonso1,
  • José Manuel Villalobos-Escobedo2,
  • Philippe Rolshausen3,
  • Alfredo Herrera-Estrella2,
  • Clara Galindo-Sánchez4,
  • José Fabricio López-Hernández2 and
  • Rufina Hernandez-Martinez1Email authorView ORCID ID profile
BMC Genomics201617:615

https://doi.org/10.1186/s12864-016-2952-3

Received: 19 March 2016

Accepted: 19 July 2016

Published: 11 August 2016

Abstract

Background

Lasiodiplodia theobromae is a fungus of the Botryosphaeriaceae that causes grapevine vascular disease, especially in regions with hot climates. Fungi in this group often remain latent within their host and become virulent under abiotic stress. Transcriptional regulation analysis of L. theobromae exposed to heat stress (HS) was first carried out in vitro in the presence of grapevine wood (GW) to identify potential pathogenicity genes that were later evaluated for in planta expression.

Results

A total of 19,860 de novo assembled transcripts were obtained, forty-nine per cent of which showed homology to the Botryosphaeriaceae fungi, Neofusicoccum parvum or Macrophomina phaseolina. Three hundred ninety-nine have homology with genes involved in pathogenic processes and several belonged to expanded gene families in others fungal grapevine vascular pathogens. Gene expression analysis showed changes in fungal metabolism of phenolic compounds; where genes encoding for enzymes, with the ability to degrade salicylic acid (SA) and plant phenylpropanoid precursors, were up-regulated during in vitro HS response, in the presence of GW. These results suggest that the fungal L-tyrosine catabolism pathway could help the fungus to remove phenylpropanoid precursors thereby evading the host defense response. The in planta up-regulation of salicylate hydroxylase, intradiol ring cleavage dioxygenase and fumarylacetoacetase encoding genes, further supported this hypothesis. Those genes were even more up-regulated in HS-stressed plants, suggesting that fungus takes advantage of the increased phenylpropanoid precursors produced under stress. Pectate lyase was up-regulated while a putative amylase was down-regulated in planta, this could be associated with an intercellular growth strategy during the first stages of colonization.

Conclusions

L. theobromae transcriptome was established and validated. Its usefulness was demonstrated through the identification of genes expressed during the infection process. Our results support the hypothesis that heat stress facilitates fungal colonization, because of the fungus ability to use the phenylpropanoid precursors and SA, both compounds known to control host defense.

Keywords

Fungal gene expression Botryosphaeria dieback Vitis vinifera RT-qPCR Graevine vascular diseases RNA-seq Transcriptome Melanin

Background

In recent years, global climate change has had a devastating impact on crop productivity. Drought and heat stress have resulted in an increased tree mortality worldwide [13]. This phenomenon could be attributed in part to endophytic fungi. Fungi inhabiting the vascular system of trees can become pathogenic under abiotic stress. In susceptible plant hosts, this results in the development of wood necrosis and cankers, because trees failed to effectively compartmentalize the pathogen. As the fungus colonizes its host, the plant vascular function becomes increasingly impaired. Prolonged abiotic stress conditions and biotic infections lead to tree decline and eventually death [46]. Two independent studies have analyzed, at the molecular level, the interaction of trees susceptible to fungal pathogens. Both studies highlighted the adaptation capability of the fungus to metabolize terpenoids and stilbene, the main defensive compounds produced by the host in response to infection, and use them as carbon sources for wood colonization [7, 8]. Both compounds are produced in response to biotic and abiotic stress in plants [9, 10], suggesting that the fungal colonization is favored when plants are under abiotic stress.

Grapes are the world’s most economically important fruit crop and have been cultivated in a broad range of environmental conditions [11]. Fungal vascular diseases (a.k.a. Eutypa dieback, Botryosphaeria dieback and Esca) are major factors limiting grape productivity and fruit marketability worldwide [12, 13]. Several taxonomically unrelated fungi are known to cause these diseases. Lasiodiplodia theobromae [teleomorph Botryosphaeria rhodina (Griff. & Maubl., Bull. Soc.Mycol. Fr. 25: 57. 1909)] is one of the causal agents of Botryosphaeria dieback. It is especially predominant in hot climates, and it has been classified as one of the most aggressive vascular pathogen of grapevine [12, 1416]. Despite its socio-economic impact, there is still little knowledge on its biology and no genome sequence information is currently available. In comparison, Eutypa lata (Pers.:Fr.) Tul. & C. Tul. (syn. E. armeniacae Hansf. and Carter), which causes similar wood symptoms, has been extensively studied and its genome has been sequenced [1721]. E. lata has the capacity to colonize the host vascular system targeting non-structural carbohydrate (i.e. starch) and structural hemicellulosic cell wall glucans for its metabolism [20].

L. theobromae and related members of the family Botryosphaeriaceae have been recognized as latent pathogens in many hosts [22, 23]. This pathogen was identified as a causal agent of mortality in dogwood tree under drought stress [24]. Similarly, Álvarez-Loayza et al. [25] observed that the disease incidence caused by Botryosphaeriaceae, Diplodia mutila on tropical palm Iriarte deltoidea, had a clear correlation with light availability, higher plant exposure to sunlight results in faster disease progression. Authors suggest that fungal reactive oxygen species (ROS) detoxification and melanin production triggered the imbalance in the endophyte-host interaction.

Biochemical assays have been used traditionally to identify pathogenicity factors produced by grapevine vascular pathogens, including secondary metabolites and plant cell wall degrading enzymes (PCWDEs) [17, 18, 26]. The advent of high throughput (OMICs) technologies have allowed for a better understanding of the complex plant/pathogen interactions in grapevine diseases. For instance, the secretome analysis of Diplodia seriata identified three necrotic inducible proteins, suggesting that fungi induce a hypersensitive-like response in host grapevine cells [27]. Recently, the genomes of grapevine vascular pathogens Neofusicoccum parvum, D. seriata and E. lata were obtained [21, 28, 29]. Through a genomic comparative study, the expansion of dioxygenase (PF00775), pectate lyase (PF03211), major facilitator superfamily (PF07690), carboxylesterase (PF00135) and glucose-methanol-choline oxidoreductase (C-terminal: PF05199 and N-terminal:PF00732) gene families were identified on these pathogens suggesting a role in pathogenicity [29].

The hot and arid viticulture production areas, provide a unique place to study how commensal interaction between an endophytic fungus and grapevine, become pathogenic under extreme heat conditions. This research aim was to evaluate L. theobromae global transcriptional response in both in in vitro and in planta bioassays. In addition, this work was designed to better understand the impact of heat stress at the fungal transcriptional level, and how it affects pathogenicity and the expression of disease symptom in grapevines.

Methods

Fungal growth condition

L. theobromae UCD256Ma was isolated from grapevine showing symptoms of Botryosphaeria dieback located in Madera County in California, USA by Urbez-Torres et al. [14] and kindly shared by Dr. Douglas Gubler. The isolate was maintained at—20 °C in 20 % glycerol in the laboratory of phytopathology at CICESE. Infection and recovery in Vitis vinifera cv. Cabernet Sauvignon green shoots was used to reactive it. After recovery, a plug of mycelium of the fungus grown on Potato Dextrose Agar (PDA, Difco) was inoculated in Erlenmeyer flasks containing Vogel’s salts (VS) [30] or Vogel’s salts with chips of grapevine wood (GW). Wood samples were obtained from branches of one year old V. vinifera cv. Cabernet Sauvignon grown in greenhouse from cuttings, pieces were frozen in liquid nitrogen, ground with a blender (Waring), filtered through a 0.35 mm sieve (Precision Scientific) and autoclaved. After inoculation, flasks were incubated at 28 °C in darkness, without agitation for 48 h. Then, some flasks were exposed to HS by transferring them at 42 °C for 1 h and then returned to 28 °C, while controls were maintained at 28 °C. Ten minutes after HS, mycelia were collected using previously sterilized tweezers, washed with water treated with diethylpyrocarbonate (DEPC, Sigma) and transferred to 1.5 ml tubes with 500 μl of Nucleic Acid Preservation (NAP) buffer [31] and stored at −80 °C until RNA extraction.

RNA extraction and sequencing

Total RNA extraction was done through modification of protocols based on Reid et al. [32] and Vasanthaiah et al. [33] as described by Paolinelli-Alfonso et al. [34]. RQ1 DNAse (Promega) treatment was done according to manufacturer’s instructions. DNA-free total RNA was sent to the National Laboratory of Genomics for Biodiversity service facilities (Irapuato, Mexico) for sequencing. RNA quality was verified on an Agilent 2100 Bioanalyzer using the RNA 6000 Nano kit according to the manufacturer’s instructions. Complementary DNA (cDNA) and the ligation of adapters were done with the TruSeq Paired-End Cluster Kit v3-cBot-HS (Illumina) according to the manufacturer’s instruction. Libraries of cDNA were made from fungus grown in the conditions described in Fig. 1. These conditions were: grown in the absence of GW (F), in the absence of GW plus HS (FS), in the presence of GW (FW) and in the presence of GW plus HS (FWS). Three biological replicates for each condition were sequenced in 1 lane of an Illumina Hiseq2500, to obtain 100 bp pair-end reads. All sequence data are available from the Gene Expression Omnibus DataSets (GSE75978).
Fig. 1

Contrasting conditions in RNAseq evaluated in general linear model statistics to identify differentially expressed genes. The conditions evaluated were from fungus grown in Vogel’s salts without heat stress (F) or under heat stress (FS), Vogel’s salts with 1 % of grapevine wood (GW), without heat stress (FW) or under heat stress (FWS). To evaluate the gene expression under the effect of heat stress (HS), the expression of FS was compared to F (FS/F). To test only the effect of HS when GW was present, FWS/FW ratio was measured, while to test both effects at the same time the ratio FWS/F was considered. Finally, fungal gene expression only as effect of GW, was measured evaluating FW/F ratio

Bioinformatics analysis

The general pipeline used for transcriptome analysis is schematically represented in Additional file 1: Figure S1. All scripts employed here are available upon request.

De novo transcriptome assembly and functional annotation

All the reads obtained from the Illumina sequencing were filtered using Trimmomatic (Trimmomatic-0.32, [35]) and sequencing quality control program (FastQC [36]) to select only those showing a PHRED quality higher than Q30, absence of adapters and homopolymers, and those with a length higher than 90 bp. The filtered sequences were used for assembly using Trinity (trinityrnaseq_r20140717, [37]) with the default settings (kmer = 25). The assembly quality check was done with the Perl script (analyze_blastPlus_topHit_coverage.pl) included in the trinityrnaseq_r20140717 package [38]. The fasta file output produced by Trinity, containing all possible isoforms, was filtered to retain only the longest using an online available Python script (longest_isoform_filter_trinity_assem.py). The longest isoform sequences were used as queries in BlastX (version 2.2.29+, [39]) from the National Center for Biotechnology Information (NCBI) using the non-redundant (NR) protein database, retaining the highest scored hit with E value < 0.001. The file with BlastX hits was used to retrieve the functional annotations with Blast2GO software (version 3.0, GO-DB version 2014–09, [38]) using the gene ontology (GO) database updated on September 2014 and default parameters as recommended [40]. The InterProScan sequence analysis application [41] in the Blast2GO software was used to predict the secretion signal with SignalP 4.0 [42]. The presence of transmembrane domains was determined with TMHMM [43]. Domain information was retrieved through PfamA [44] and HAMAP [45]. Sequences with positive SignalP predictions [41] in the N-terminal region and without any transmembrane regions as predicted by TMHMM [43] were selected as candidate secreted proteins.

The fasta file of the longest isoform sequences was used to predict the open reading frames (ORFs) through the usage of TransDecoder (TransDecoder_r20140704; [46]). The predicted ORFs sequences were used in a local BlastP (version 2.2.28+, [38]) analysis in the Pathogen-Host Interaction (PHI) database (version 3.6, [47]).

Differential expression and functional enrichment analysis

The raw reads of both ends obtained for each output file were aligned to the longest isoform transcripts using Bowtie 2 (version 2.1.0, [48]) with default parameters. The resulting output in SAM format was converted to BAM format through Samtools (version 0.1.19-96b5f2294a; [49]). Using the sorted bam file, the number of alignments were counted for each transcript and sample using a homemade Perl script specially designed (count_filebam.pl and count_names.pl) to output a tab delimited table. The statistical analysis was done using edgeR package version 3.4.2 [50] of Bioconductor [51] in the R environment (version 3.0.2, [52]). Normalization was done using counts of reads per million (cpm) and filtered to retain transcripts that had at least 3 cpm in more than 2 samples. The statistical analysis was done using a General Linear Model (GLM) approach. The conditions compared are shown in Fig. 1. The false discovery rate (FDR) < 0.01 was set as the threshold to consider genes as differentially expressed.

Differentially expressed genes (DEGs) for any of the contrasting conditions evaluated were arranged in clusters based on their expression pattern through Pearson correlations in edgeR. The list of genes for each cluster was used as test and all the differentially expressed genes were used as references in an enrichment analysis (Fisher’s exact test, FDR < 0.05) using Blast2GO software (version 3.0, GO-DB version 2014–09, [39]). The GOplot package (version 1.0.1, [53]) in the R environment was used to generate the graph GOcluster and GOcircle in order to obtain a more detailed view of co-regulated genes in relationship with functional enrichment.

Evaluation of L. theobromae growth in benzoate

To evaluate the capacity of L. theobromae to grow in benzoic acid (BZA) as the sole carbon source, the fungus was inoculated in agar plates containing Vogel’s Minimal Medium (VMM) [30] supplemented with 0, 15 or 30 mM of BZA. Photographs were taken after 8 days of incubation at 28 °C.

In vitro and in planta fungal gene expression of selected targets

Twelve genes that were found to be differentially expressed in the RNAseq analysis were selected for validation and relative quantification of gene expression through reverse transcription-quantitative PCR (RT-qPCR), both in vitro and in planta (genes selected and primers are shown in Additional file 2: Table S1).

The effect of HS was simulated in growth chambers by exposing the L. theobromae-infected plants to a daily temperature cycles changing from higher minimal to a higher maximal. One year-old cuttings V. vinifera cv. Merlot, were grown in UC special mix soil in 5 L pots and kept at room temperature at the University of California Riverside lathhouse facilities. Using a sterile razor blade, green shoots from thirty plants were wounded on the second basal internode and inoculated with a 3 mm mycelia plug obtained from a three day-old culture of L. theobromae. A total of 6 plants were inoculated with a PDA plug and used as controls. All wounds were covered with paraffin wax film (Parafilm M) following inoculation. Five days later, fifteen plants inoculated with L. theobromae and three plants inoculated with PDA were exposed to HS using night-day cycles ranging from 20 °C to 42 °C at 50 % humidity on growth chamber (Environmental Growth Chamber EGC-TC2). The remaining plants were incubated in a growth chamber (Conviron PGR15) with night-day cycles ranging from 10 °C to 30 °C at 50 % humidity, and used as controls without HS. At 7, 11 and 15 days post inoculation (dpi) plants were collected, shoots were cut in transversal sections at least 5 mm up or down from the inoculation point, a section was used for stereo microscopy (Leica M125) observation and the remaining were collected in NAP solution and stored at −20 °C until RNA extraction. The RNA extraction was done using a cetyltrimethylammonium bromide (CTAB) -based protocol (details in Additional file 3). Total RNA was treated with RQI DNAse (Promega) and the cDNA obtained with the ImProm AM3800 (Promega) kit, according to the manufacturer’s instruction. The qPCR was done on a CFX96 thermocycler (Bio-Rad) using 3 μl of cDNA and 7 μl of mastermix containing 2.5 mM MgCl2, 1X Taq polymerase Accustart buffer (Quanta), 0.2 mM of dNTPs, 0.03 U/ul Taq polymerase Accustart (Quanta), 1X EVAgreen (Biotium) and 0.2 μM of each primer. Two biological with three technical replicates were used for in vitro and three biological with three technical replicates were used for in planta gene expression analyses.

The HTqPCR package (version 3.2, [54]) for R environment (version 3.0.2, [52]) was used for normalization against β-tubulin mRNA, relative expression quantification and limma statistical analysis. In planta fungal gene expression was calculated as fold change in HS-treated host or non HS-treated and infected plants compared to L. theobromae growing in in vitro conditions. cDNA from non-infected plants was used as negative controls when the specificity was verified through the analysis of melting curves for each gene.

Results

Transcriptome assembly and functional annotations

Sequencing reads varied in number, ranging from 3 to 6 million per sample, with an average of approximately 5 million reads (Additional file 4: Figure S2), showing PHRED quality scores per base of 36. The de novo assembly with Trinity [37] produced 29,621 total components (including isoforms), %GC = 56 and N50 = 3,135 bp (details in Table 1).
Table 1

Main characteristics of Trinity de novo transcriptome assembly

Parameters

All transcript

Only longest Isoform

Number of contigs

29621

19860

Contig N10

6773

5525

Contig N20

5345

4321

Contig N30

4365

3572

Contig N40

3667

2971

Contig N50

3135

2472

Median contig length

1242

658

Average contig

1798.4

1310.58

Total assembled bases

53270493

27680863

From the 29,621 total components, the longest isoforms were selected, rendering 19,860 unique transcripts with N50 = 2,472 bp; the median length was 658 bp and the average contig length was 1,310.58 bp (Table 1). More than 50 % of the assembled transcripts showed at least 80 % full-length coverage as compared to well-annotated proteins, and 33 % showed 100 % coverage, indicating that the assembly fulfills the requirements of quality analysis through ortholog hit ratio [55] which justifies its use to map the reads and analyze gene expression.

When the transcripts were arranged according to the taxonomic information retrieved from BlastX, most hits showed similarity with members of either of the Botryosphaeriaceae family, M. phaseolina (5,800 sequences, 29 %) and N. parvum (3,800 sequences, 19 %), the only two Botryosphaeriaceae genomes available in the NR-NCBI database at the time of analysis, or several other fungi from the Ascomycota phylum (Additional file 5: Figure S3). The high number of L. theobromae sequences homologous to M. phaseolina over N. parvum was supported by previous phylogenetic analyses showing L. theobromae phylogenetically closer to M. phaseolina than to N. parvum [56].

From the 19,860 longest isoforms, 7,547 sequences (38 %) had recognizable functional GO annotation (details of annotation results in Additional file 6: Figure S4). The GO terms associated with each transcript encoded protein were used to associate them according to their function. A wide diversity of functions were identified (details in Additional file 7). Among others, in the Biological process in fourth level of gene ontology classification, most of the transcripts were involved in nitrogen metabolism (684), aromatic (665), organic cycles (689) and heterocycle (676) compounds metabolism. Also there are 589 transcripts involved in oxidation-reduction process.

Based on the importance of genes encoding proteins with extracellular functions in the establishment of the interaction of the fungus with its host, transcripts encoding proteins with N-terminal secretion signal were identified. From 15,981 transcripts that contain at least one ORF, 850 were predicted to be secreted.

On other hand, a total of 399 protein-coding transcripts, showing homology with those included in the Pathogen-Host Interaction database (PHI-base) were identified. PHI-base contains experimentally verified pathogenicity or virulence factors, therefore L. theobromae transcripts showing PHI-base hits are predicted to be involved in pathogenicity. Based on functional annotation of PHI-base hits, they were classified according to their gene ontology information, and were identified as being involved in protein modification processes, metabolism of phosphate-containing compounds, hydrolase activity on glycosyl bonds, and oxidoreductase on CHOH groups (Fig. 2). Additionally, 22 PHI-base hits were predicted to be secreted, and according to their annotation, they could be involved in carbohydrate metabolism, proteolysis and oxido-reduction processes (Additional file 8).
Fig. 2

Pie chart describing the main Gene Ontology (GO) of molecular functions categories of transcripts with putative pathogenicity role. The predicted open reading frames encoded by transcripts were used in a local Blastp to find hits in the experimentally verified Pathogen-Host Interaction database (PHI-base). The PHI-base hits were classified based on its GO information

Differential gene expression, co-regulation and functional enrichment

The analysis of RNAseq data indicated that sufficient differences were achieved among treatments and therefore allowed the identification of DEGs (Additional file 9). In total, 2,386 DEGs (FDR < 0.01) were identified in any of the contrasting conditions tested (Fig. 1). These corresponded to 12 % of the total number of transcripts. Different numbers of DEGs were obtained for the different contrasting conditions, FWS/F contrast has the highest number (Table 2 and Additional file 10). All the contrast generate specific unique DEGs not shared with the DEGs from the other contrasts (Additional file 11: Figure S5). An analysis of their pattern of expression was used to arrange the genes in clusters of co-regulated genes (Fig. 3 and Additional file 12).
Table 2

Number of differentially expressed genes (DEGs, FDR < 0.01) and enrichment test for secretion for each contrasting conditions

Contrasting conditions

Regulation

Differentially expressed genes (DEGs)

Predicted secreted DEGs

FDR (hypergeometric test for enrichment of secreted proteins)

FWS/F

Up-regulated

905

83

0.156003

Down-regulated

887

74

0.549571

FWS/FW

Up-regulated

173

13

0.707640

Down-regulated

233

17

0.770976

FW/F

Up-regulated

565

61

0.012635

Down-regulated

424

47

0.554427

FS/F

Up-regulated

203

23

0.077195

Down-regulated

366

28

0.738934

Fig. 3

Heatmap showing clusters of co-regulated genes with their expression profiles. The dendrogram indicates the relationship between gene expression profiles as determined by hierarchical clustering (Pearson correlation). The differentially colored boxes at the left indicate different clusters of genes with similar expression profiles. The color key indicates logFC values ranging from bright red for most up-regulated to bright green for the most down-regulated genes, considering a FDR < 0.01. The expression pattern for clusters with functional enrichment (clusters 1, 3 and 7) are shown in a graph with gray lines for each gene while the average for all the genes in the cluster is shown in red line. The contrasting conditions evaluated are those indicated in Fig. 1. Briefly, FS/F: effect of heat stress (HS); FWS/FW: effect of HS but in the presence of grapevine wood; FWS/F: effect of HS in the presence of grapevine wood and FW/F: effect of only GW

Functional enrichment was obtained in three clusters of co-regulated genes. An enrichment for oxido-reductase activity was obtained for cluster 1 (FDR = 1.2x10−3), and the shared pattern of expression for the putative genes was mainly the induction in FWS/FW and FWS/F, and repression in FW/F (Fig. 3). Cluster 3 showed enrichment in hydrolase activity, mainly involved in the hydrolysis of O-glycosyl compounds (FDR = 2.3x10−8), and showed an inverse pattern of expression compared to cluster 1, with major protein-coding genes up-regulated in FW/F, but down-regulated in FWS/FW and a lower level of induction or down-regulation in FS/F (Fig. 3). Cluster 7 showed an enrichment (FDR < 0.01) in translation processes, GTPase and methyltransferase activities. The shared pattern of expression in cluster 7 was mainly due to the induction in FS/F (Fig. 3).

On the other hand, the presence of GW resulted in repression of genes encoding enzymes with oxido-reductase activity (GO term: GO0016491) and induction of genes coding for O-glycosyl hydrolyzing enzymes (GO term: GO0004553, Fig. 4 and Fig. 5). In contrast, after HS, the expression pattern was inverse to the fungus growing in GW: genes for oxido-reductase activity were up-regulated while genes coding for O-glycosyl hydrolyzing enzymes were mainly down-regulated (Fig. 4 and Fig. 5). The genes involved in translation activities (GO terms: GO0008135 and GO0003743) and methyltransferase activity (GO term: GO0008168) showed primarily up-regulation in both contrasting conditions, FW/F and FWS/FW (Fig. 4), indicating the importance of the translation process in regulating the response to either change.
Fig. 4

Gene Ontology (GO) of molecular functions categories with enrichment in hierarchical clusters of similar expression profiles. The GO term differential expression is considered through z-score (\( \mathrm{zscore}=\frac{\left(\mathrm{upregulated}\hbox{-} \mathrm{downregulated}\right)}{\sqrt{\left(\mathrm{upregulated}+\mathrm{downregulated}\right)}} \), described in [53]). Red color indicates higher proportion of up-regulated genes and blue color corresponds to higher proportion of down-regulated genes. The color key indicates logFC values ranging from golden for up-regulated genes, to cyan for down-regulated genes. The effects of only grapevine wood (FW/F) and heat stress in the presence of grapevine wood (FWS/FW) were evaluated

Fig. 5

Functional enrichment of Gene Ontology (GO) categories based on the differentially expressed genes in each analyzed contrast. The color key indicate from pale yellow to blue, the increasing percentage of genes representing each functional category. To eliminate general and excessively specific categories, only the functional categories that have at least 5 and maximum 500 genes were considered in the analysis. The contrasting conditions evaluated are those indicated in Fig. 1. Briefly, FS/F: effect of heat stress (HS); FWS/FW: effect of HS but in the presence of grapevine wood; FWS/F: effect of HS in the presence of grapevine wood and FW/F: effect of only GW. * FDR < 0.2 and ** FDR < 0.05

Our results showed that inosine monophosphate (IMP) cyclohydrolase, squalene monooxigenase and protein disulfide monooxigenase GO categories were induced in all the contrasting conditions (Fig. 6). According to the established functions of these GO categories, it seems that basic metabolism such as purine nucleotide biosynthesis, sterol biosynthesis and post-translational modifications are important both to sustain growth on GW and under HS. Similar basic mechanisms might be required to deal with both conditions, perhaps because oxidative stress is produced in response to HS, and also required for GW degradation. On the other hand, genes involved in tyrosine and L-phenylalanine metabolic processes were only induced in FWS/FW, while they were highly repressed in all other contrasted conditions, suggesting a specific requirement of this metabolic pathway to deal with HS when in contact with wood components (Fig. 6).
Fig. 6

Gene Ontology (GO) of biological process categories with enrichment and showing differentially expressed genes in all the contrasting conditions evaluated (FDR < 0.05). The color key indicates logFC values ranging from golden for up-regulated genes, to cyan for down-regulated genes. The dendrogram indicates the relationship through the hierarchical clustering of gene expression (the middle rings show from the center out: effect on L. theobromae gene expression of heat stress (HS) and grapevine wood (FWS/F), only grapevine wood (FW/F), only HS (FS/F), and effect of HS in the presence of grapevine wood (FWS/FW). The Biological Process GOterms are indicated in different colors on the outermost circle

Secreted proteins are more prone to interact with the host; therefore we tested whether an enrichment of genes predicted to encode secreted proteins occurred among the DEGs. Among the upregulated genes in GW condition, there was an enrichment of those enconding for secreted proteins (FDR < 0.05 in Table 2), indicating that the presence of wood promotes the expression of secreted proteins. The list of genes coding for proteins presenting eukaryotic secretion signals, with their respective annotation, and classified in clusters based on co-regulation, is shown in Additional file 13.

L. theobromae gene expression during the interaction with grapevine

Co-regulated clusters (Fig. 3) with functional enrichment indicated a whole fungal transcriptional change when exposed to HS in the presence of GW. Several genes belonging to any of the clusters 1, 3 and 7 (Fig. 3) that were identified as having pathogenicity roles, based on their functional annotation, were selected to evaluate their expression by RT-qPCR. cDNA obtained from in vitro conditions was used for the validation of RNAseq results, and cDNA from in planta conditions in an attempt to elucidate their role in pathogenicity.

The in vitro expression of 7 genes (Additional file 2: Table S1) confirmed the contrasting pattern of expression based on the cluster to which each gene belonged and showed a high correlation with the results obtained through RNAseq (R2 = 0.876 and p-value = 1.9x10−5, Additional file 14: Figure S6).

In general when evaluating the expression in planta, a marked regulation of most genes was observed at 7 dpi, and the changes on gene expression were even more defined in stressed plants (Fig. 7). L. theobromae genes with up-regulated expression in planta were those enconding an intradiol ring cleavage dioxygenase (IRCD, comp4276_c0_seq1, selected from cluster 1), salicylate hydroxylase (SH, comp12473_c0_seq1, selected from cluster 1) pectate lyase (PL, comp16237_c0_seq1, selected from cluster 3), xylosidase glycoside hydrolase (XGH, comp5761_c0_seq2, selected from cluster 3) and a fumarylacetoacetate hydrolase (FMH, comp14342_c0_seq1, selected from cluster 1). IRCD was up-regulated at all infection times evaluated, in both heat-stressed and non-stressed plants (Fig. 6). At 7 dpi on stressed plants, SH was up-regulated when compared to infected and non-stressed grapevines (Fig. 7). In contrast, sugar inositol transporter (SIT, comp8181_c0_seq1), choline dehydrogenase (CHD, comp5526_c0_seq1), homogentisate dioxygenase (HGD, comp8784_c0_seq1), 4-hydroxyphenylpyruvate dioxygenase (HPPD, comp18638_c0_seq1) and glycoside hydrolase family 3 (GH3, comp13725_c0_seq1) did not show differential expression. A putative amylase from glycoside hydrolase family 35 (AML, comp7101_c0_seq1) and multicopper oxidase (MCO, comp7300_c0_seq1, from cluster 3) were highly down-regulated, specially under HS (Fig. 7).
Fig. 7

L. theobromae gene expression during grapevine infection. Fungal gene expression was evaluated at 7, 11 and 15 days post-infection in unstressed or heat-stressed grapevine (HS). Normalization was done using β-tubulin and the relative gene expression is indicated as logFC (in planta/in vitro) using HTqPCR package in R. One asterisk indicates significant differences with general linear model statistics (p-values < 0.05) for in planta/in vitro and quotation marks for heat-stressed/non stressed contrasting conditions. The dendrogram indicates the relationship between gene expression profiles through calculates of Canberra distances and Pearson correlation. The color key indicates logFC values ranging from golden for up-regulated genes, to cyan for down-regulated genes. IRCD: intradiol-ring cleavage dioxygenase (comp4276_c0_seq1); SH: salicylate hydroxylase (comp12473_c0_seq1); FMH: fumarylacetoacetate hydrolase (comp14342_c0_seq1); SIT:sugar inositol transporter (comp8181_c0_seq1), MCO: multicopper oxidase (comp7300_c0_seq1), PL: pectate lyase (comp16237_c0_seq1), AML: amylase (comp7101_c0_seq1), HGD: homogentisate dioxygenase (comp8784_c0_seq1), CHD: choline dehydrogenase (comp5526_c0_seq1), GH3: glycoside hydrolase family 3 (comp13725_c0_seq1), XGH: xylosidase glycoside hydrolase (comp5761_c0_seq2), HPPD: 4- Hydroxyphenylpyruvate dioxygenase (comp18638_c0_seq1)

Discussion

L. theobromae transcriptome features and comparison with related fungal pathogens

The closest fungi taxonomically related to L. theobromae with sequenced genomes are M. phaseolina, which has 14,249 genes (1,863 encoding secreted proteins (SP)) [57], D. seriata with 9,398 genes (910 SP) and N. parvum with 10,470 genes (1,097 SP) [29]. The number of unique predicted proteins derived from unique isoforms (15,981), and those with predicted secretion signal (850) obtained through de novo transcriptome assembly, suggests that the number of genes in L. theobromae is similar to its closest relatives.

Most of the assembled contigs covered the expected transcript length (average: 1,310 bp and N50: 2,472 bp, details in Table 1), considering the 1,531 and 1,574 bp average gene length in N. parvum and D. seriata, respectively [21, 29].

From the unique predicted proteins for all the transcripts, 399 had hits to PHI-base [47]. In M. phaseolina, 537 PHI-base hits were identified [57], while 1,120 were identified in D. seriata and 1,384 in N. parvum [29]. The differences found may be explained based on the different methods employed, since the relatives were fully sequenced and here RNAseq was done only in in vitro conditions. Further RNAseq analysis in planta will be useful to identify higher number of pathogenicity genes in this fungus. The putative pathogenicity transcripts (showing PHI-base hits) in L. theobromae, indicate main involvement in protein metabolic process, hydrolization of glycosyl bonds and oxidoreduction process (Fig. 2). In coincidence, these GO categories showed most marked regulation when the fungus growing on GW was exposed to HS (Fig. 4), suggesting that HS response and pathogenicity require a common transcriptional regulation. From the 399 PHI-base hits, 48 were differentially expressed, 22 were predicted to be secreted, and 8 of them shared both characteristics (Additional file 8), indicating that the L. theobromae transcriptome is useful to identify putative pathogenicity factors, that could help to further validation of function through knockout or gene expression studies.

Gene families showed expansion in fungi causing grapevine vascular diseases producing similar symptoms as L. theobromae [29]. Genes belonging to those families were found in the L. theobromae transcriptome, that have 65 (20 DEG) dioxygenase (PF00775), 11 (2 DEG) pectate lyase (PL, PF03211), 259 (49 DEG) major facilitator superfamily (MFS, PF07690), 37 (5 DEG) carboxylesterase (PF00135) and 22 (5 DEG) glucose-methanol-choline oxidoreductase (GMC, C-terminal: PF05199 and N-terminal: PF00732).

Transcriptional regulation of genes with putative role in pathogenicity

Based on the GO enrichment by clusters containing co-regulated genes, a whole fungal response could be inferred (Fig. 4). In HS in the absence of GW, genes involved in the translation process were induced, suggesting that a change in protein profile is required to cope with stress. The requirement of heat-shock proteins (HSPs) in fungal HS response to keep proteins folded and active is well documented [58, 59]. In fact, several HSP encoding transcripts with different expression levels were identified, indicating the need of the fungal cells to redirect their physiology towards a survival or adaptive condition.

Based on functional enrichment, the fungus respond to HS differently in the presence of GW than in its absence. The specific enrichment of acyl-transferase among up-regulated genes when dealing with HS indicates that this activity could help the fungus to survive periods of stress. Acyl-transferases are involved in the synthesis of polyketides, a large class of secondary metabolites [60] that could provide the fungus with biochemical protection from stress. In contrast, in the presence of GW is not required, suggesting that some compounds, provided by GW fulfill that requirement. Genes in GO categories of integral component of membranes, mainly involved in transmembrane transport, were enriched specially in HS response in the presence of GW (Fig. 5). Most of these genes belong to the major facilitator superfamily (MFS) and have homologues on PHI base, suggesting an important role in fungal pathogenicity. Genes that belong to GO categories involved in nucleotide (GO:0050660), and post-translation modifications (Fig. 6) also are indicative of major change in the metabolism of the fungus to sustain growth under stress and in the presence of wood. On the other hand, GO term enriched GTPase activity, contains genes well known for having a role in translation and signaling events in response to stress [61], evidencing the importance of a rapid adaptation to HS. Additionally, small GTPases are involved in virulence, due to their key role in secretory pathways [61].

The repression of genes associated with electron transport (cytochrome p450 monooxygenase (comp5016_c0_seq3); dsba oxidoreductase protein (comp5774_c1_seq3), acyl- dehydrogenase family protein (comp7418_c0_seq1) and three hypothetical proteins (comp264619_c0_seq1, comp303165_c0_seq1 and comp1_c0_seq1), in response to HS and/or GW (Fig. 5), might contribute to the need of reducing the potential risk of mutation caused by higher production of ROS in mitochondria as an effect of thermal stress [62]. The down-regulation of a superoxide dismutase protein (comp6665_c0_seq1) is an unexpected result, because ROS detoxification has been proposed for superoxide dismutase and, increasing ROS levels in Saccharomyces cerevisiae were observed when responding to HS [63]. In the HS response in the absence of GW a 5-oxoprolinase (comp4986_c0_seq1) was specifically induced. This enzyme participate in glutathione mediated ROS detoxification [64], indicating that an alternative to superoxide dismutase/peroxidase could be used to deal with the ROS produced in response to HS.

A model for the L. theobromae HS response in the presence of GW was constructed (Fig. 8) based on the functional annotation, co-regulation and functional enrichment of genes (Additional file 15), that were identified through the in vitro global transcriptional response. Based on this model, several putative pathogenicity genes were selected and its gene expression was evaluated during fungal-grapevine interaction.
Fig. 8

Hypothetical model of in vitro L. theobromae heat stress (HS) response, in the presence of grapevine wood (GW). The model of whole cell response was constructed using genes from clusters 1, 3 and 7 (in Fig. 2) showing both co-regulation and GO term enrichment. Additional file 13 gives the gene name with its expression pattern. The illustration shows the main functions and processes being carried out by the fungus when growing on GW (a), and the changes that are proposed to be occurring after HS (b). The putative cellular location (intra or extracellular) is indicated in the scheme. A continuous arrow line indicates an enzymatic reaction that is supported on the differentially expression of its encoding gene (shown in red). A dashed arrow line indicates a suggested enzymatic reaction. The substrate/product of reaction is indicated on boxes. TYR: tyrosinase, MCO: multicopper oxidase, DOPA: L-3,4-dihydroxyphenylalanine, HPP: 4-hydroxyphenylpyruvate, HPPD: 4-hydroxyphenylpyruvate dioxygenase, HGD: homogentisate dioxygenase, HGA: homogentisic acid, 4-MAA: 4-maleylacetoacetate, 4-FMAA: 4-fumarylacetoacetate, FM: fumarate, AA: acetoacetate, FMH:fumarylacetoacetate hydrolase, SH: salicylate hydroxylase, IRCD: intradiol ring cleavage dioxygenase, DDP: domon domain containing protein, PCWDEs: Plant cell wall degrading enzymes; PCW: Plant cell wall

Genes with putative role in grapevine wood degradation and pathogenicity

Most of the up-regulated genes in GW but down-regulated in HS are predicted to be involved in the degradation or modification of plant cell wall (PCW) components, based on their functional annotation (hydrolysis of O-glycosyl compounds, GO: 0004553, Fig. 4). A gene coding for a putative secreted enzyme that belongs to the glycosyl hydrolase (GH) family 35, has conserved domains which suggest its role as amylase (comp7101_c0_seq1). Its expression was induced by GW and showed no significant differences in the contrasting condition FWS/FW, indicating that degradation of starch remains active independently of HS. In grapevine wood, starch is stored in ray parenchyma cells, next to xylem vessels and it is used as carbon reserve by the plant [65]. E. lata, a vascular pathogen of grapevine that has similar colonization strategy as L. theobromae, has been shown to degrade plant starch [20] suggesting that this polymer may play a pivotal role as energy reserve for both the vascular pathogen and the plant metabolisms. Since the relationship among starch degradation and pathogenicity seems important for disease progression, the putative amylase (comp7101_c0_seq1) expression was evaluated in planta. Under stress conditions, it showed a marked down-regulation at any time of infection and treatment (Fig. 7), indicating that its activity is not required for the establishment of the infection, at least in the evaluated conditions. This enzyme was annotated as a putative amylase, because of one of its domain is a GH35; since this can be considered as an incomplete annotation, the enzyme encoded by comp7101_c0_seq1 sequence might have another function.

Among the genes coding for proteins predicted to be secreted, three are associated with pectin degradation: PL (comp16237_c0_seq1), GMC (comp7222_c0_seq1) and CHD (comp5526_c0_seq1). These genes encode for PCWDEs belonging to an expanded family in grapevine vascular pathogens [29]. The first one is involved in pectate cleavage [66], while the second and third one correspond to a gene family involved in lignin breakdown [67]. PL and CHD expression during fungal colonization was quite contrasting, while PL was significantly up-regulated, especially under HS at 7 dpi, CHD was down-regulated at any stage (Fig. 7). This suggests that lignin break-down was not required for fungal infection, but pectin degradation seems to be important for fungal pathogenicity. Pectin is the main component of middle lamella [68] and therefore have a fundamental role blocking intercellular fungal growth. Recently, it was clearly determined the importance of pectin degrading enzymes for Fusarium graminearum intercellular colonization of maize parenchyma tissue [69]. We propose that PL allows L. theobromae to colonize grapevine tissues intercellularly.

Genes encoding an endopolygalacturonase (comp4965_c2_seq1) and a pectinesterase (comp13568_c0_seq1) were also up-regulated in response to GW and have been associated with PCW degradation [65, 66]. Furthermore, expression of secreted enzymes, xylosidase glycoside hydrolase (XGH comp5761_c0_seq2), glycoside hydrolase family 3 (GH3 comp13725_c0_seq1) and endo1,4-betagalactanase (comp15147_c0_seq1), which are involved in cellulose and hemicellulose degradation [66], were found up-regulated in response to GW. Rolshausen et al. (2008) also reported in vitro hemicellulose degradation and increased enzymatic activity in the presence of wood in E. lata [20]. Two genes coding for enzymes that belong to GH1 with glucosidase/galactosidase activity (comp2943_c0_seq1 and comp7123_c0_seq1) have homologous genes with recognized intracellular roles in cellobiose and lactose catabolism [67]. The expression of both XGH and GH3 were up-regulated in planta (Fig. 7). XGH showed differential up-regulation at 7 dpi on infected and stressed plants (Fig. 7), suggesting that its function on hemicelluloses degradation is required, thus, deeper access to the host cell wall seems to be favored with HS.

On other hand, an ortholog of the glyoxal oxidase (GOX) gene (comp11184_c0_seq1) showed up-regulation in the presence of GW. GOX was previously associated with PCW degradation of wood in Phanerochaete carnosa, specifically degrading lignin [70]. Furthermore, a gene (comp12572_c0_seq1) that belongs to GH16 encodes an enzyme involved in PCW modification [71] and showed up-regulation only in the presence of GW. Overall, the co-expression of these genes indicates polysaccharide degradation to use the GW as carbon-source. Its concerted enzymatic activity could help L. theobromae to colonize the host and cause the development of canker in wood. The necrosis observed close to the pith in heat-stressed plants (Fig. 9), likely indicates a deeper colonization of stem by L. theobromae. Our data suggest that the change in grapevine phenology occurs in response to HS and this change promotes a faster fungal colonization. Although not all the PCWDEs evaluated were up-regulated in planta, and even the putative amylase was down-regulated, it is possible that a specific role of up-regulated genes encoding PL and XGH favors fungal colonization under HS.
Fig. 9

The effect of heat stress (HS) on grapevines uninfected or infected with L. theobromae. Stereomicroscope images were taken at 15 days post-infection, corresponding to 10 days of HS treatment (day-night cycles, with temperatures ranging from 42 to 20 °C). Uninfected and unstressed grapevine show healthy green tissue (a). Uninfected and heat-stressed grapevine show a change to a white color of the pith and phloem impairment (b). Infected but unstressed grapevine show black, yellow and brown color tissues close to the site of inoculation (c). Infected and stressed grapevine show white pith and brown/yellow color in primary xylem (d)

Genes with putative role in phenolic, melanin, protein metabolism and pathogenicity

Several genes encoding enzymes involved in different melanin synthesis pathways reported in fungi were identified: 3,4-dihydroxyphenylalanine (DOPA)-melanin, DHN (1,8-dihydroxynaphthalene)-melanin and pyomelanin [7278]. Remarkably, the gene for a secreted enzyme associated with DOPA-melanin synthesis (MCO, comp7300_c0_seq1) showed high induction in response to GW, while it did not show regulation upon HS (Additional file 15). This gene was found as belonging to a family expanded in N. parvum and D. seriata, stressing its putative role in pathogenicity [29]. A gene encoding enzyme putatively involved in DHN-melanin synthesis (short-chain dehydrogenase reductase, comp4978_c0_seq2) showed in vitro co-regulation with MCO. On the other hand, the enzyme involved in homogentisic acid synthesis, HPPD (comp18638_c0_seq1) was up-regulated (LFC = 2.18 and FDR = 0.07) in the presence of GW. This gene is associated with pyomelanin synthesis, a fungal adaptation of the L-tyrosine metabolic pathway, where the intermediary homogentisic acid is polymerized to form melanin [73, 74, 78].

After HS, genes that encode enzymes that degrade homogentisic acid, HGD (comp8784_c0_seq1) and FMH (comp14342_c0_seq1), were up-regulated, suggesting that pyomelanin degradation is activated after HS. The gene encoding maleylacetoacetate isomerase, involved in the transformation of 4-maleylacetoacetate to 4-fumarylacetoacetate in the L-tyrosine metabolic pathway [79], was identified (comp3928_c0_seq2 and comp196313_c0_seq1 in Additional file 16) but it was not differentially expressed in the analyzed contrasting conditions. The observation of L-tyrosine metabolic pathway regulation in response to HS is strengthened by the expression pattern (up-regulated by GW and down-regulated by HS) of the C6 transcription factor (comp6826_c0_seq1). This gene was previously found in the Aspergillus fumigatus genome, arranged in a cluster with the genes involved in gentisate catabolism [79], which is an alternative pathway to tyrosine metabolism in fungi. A mutant in the C6-Zn transcription factor ProA in Epichloë festucae was unable to establish a symbiotic interaction with its host Lolium perenne, proving the importance of this gene for the maintenance of the mutualistic relationship [80]. L. theobromae has an endophytic behavior [81, 82], and it has been suggested that abiotic stress promotes its switch to a pathogenic behavior [22, 83]. The C6 transcription factor regulating genes belonging to secondary metabolism pathways in response to HS, suggest the promotion of a pathogenic-like behavior in L. theobromae as an effect of HS.

Several yeast pathogens of mammals showed a phenotypic dimorphic switch (from filamentous to bud-cells and vice versa) when changing from room temperature to 37 °C, also accompanied with a change in melanin metabolism [8487]. In general, a decrease in DOPA-melanin (tyrosinase downregulation) and/or an increase in pyomelanin production or L-tyrosine metabolism (4- hydroxyphenylpyruvate dioxygenase up-regulation) were observed consistently in previous studies [8488]. It seems that in mammalian fungal pathogens, the change in the type of melanin produced is important to trigger the morphogenetic switch and to become pathogenic. We propose that a general mechanism for becoming pathogenic under HS conditions is conserved among several fungal taxa, whereby melanin metabolism could play a role in pathogenicity in plants, similarly to fungal mammalian pathogens. Our results also demonstrated that FMH was up-regulated in planta mainly at 7 dpi under HS (Fig. 7). A fumarylacetoacetase family was exclusively expanded in Ascomycota vascular pathogens [29], suggesting an evolutionary adapted function of these enzymes to favor the colonization of this niche. FMH is involved in the final step of the tyrosine metabolic pathway, converting fumarylacetoacetate to fumarate and acetoacetate, which could be incorporated in the tricarboxilyc acid cycle to obtain energy. Alternatively, the co-regulated genes, malate synthase (MS, comp6659_c0_seq1) and isocitrate lyase phosphorylmutase (ICP, comp8689_c0_seq1), suggest that acetate could be employed for anabolic processing through the glyoxylate cycle [89].

On other hand, it has been suggested that FMH regulates pyomelanin production [73, 74]. The homogentisate, an intermediary in L-tyrosine metabolic pathway, is used by some fungi as a precursor for pigment production [73, 74]. The precursors of lignin are derived from tyrosine or phenylalanine through the phenylpropanoid defensive pathway in plants [90]. This pathway is greatly induced in response to biotic and abiotic stress; therefore the fungal elimination of such precursors for DOPA-melanin or through tyrosine catabolic pathway could help the fungus to evade the plant compartmentalization mediated through lignin. When evaluated in planta, fungal MCO expression was down-regulated, specially under HS (Fig. 7). In contrast, HPPD and FMH were up-regulated at 7 dpi on stressed plants (Fig. 7), indicating that the fungal gene regulation under stress in planta is similar to that obtained in vitro (Fig. 7), supporting the hypothesis that DOPA-melanin could act as a tyrosine storage that then is degraded through tyrosine metabolism pathway. If this is the case, the increase of grapevine phenylpropanoid pathways precursors in response to HS, could be used by L. theobromae for its metabolism to promote colonization (Fig. 10).
Fig. 10

Proposed model of fungal-plant interaction under heat stress (HS). The model was done using gathered information of in vitro L. theobromae HS global transcriptional response, gene expression in planta (Fig. 7) and documented HS response in plant. a When fungus infects unstressed plant, selectively degrades pectin (up-regulation of PL compared with the other PCWDEs), this allows it to growth in intercellular spaces without causing major damage to PCW. The presence of the pathogen could trigger the host defensive mechanism mediated through SA, or by the activation of the phenylpropanoid pathway. However, the host defense could be impaired for the activity of SH and IRCD (degrade SA), or by HPPD (phenylpropanoid precursors). b Heat stress activates the same metabolic pathways increasing SA and the levels of phenylpropanoid precursors, thus the fungus could benefit from the higher availability of compounds using them as carbon sources. The main differential change on stressed plant, compared with unstressed, is the up-regulation of SH, FMH and XGH, whose activities could facilitate fungal colonization. Tyr: tyrosine. Phe: phenylalanine. SA: salicylic acid, IRCD: intradiol-ring cleavage dioxygenase (comp4276_c0_seq1); SH: salicylate hydroxylase (comp12473_c0_seq1); FMH: fumarylacetoacetate hydrolase (comp14342_c0_seq1); SIT:sugar inositol transporter (comp8181_c0_seq1); PL: pectate lyase (comp16237_c0_seq1). XGH: xylosidase glycoside hydrolase (comp5761_c0_seq2), HPPD: 4- Hydroxyphenylpyruvate dioxygenase (comp18638_c0_seq1). FCW: fungal cell wall. PCW: plant cell wall; PCWDEs: plant cell wall degrading enzymes

In this work, SH (comp12473_c0_seq1) was up-regulated upon HS in the presence of GW during in vitro growth (Additional file 14: Figure S6). The product of SH activity, catechol, induces the ROS-mediated plant defensive response [91, 92]. IRCD (comp4276_c0_seq1), a gene coding for an enzyme that catalyze the degradation of aromatic rings [93], was co-regulated with SH. IRCD could act degrading catechol and therefore helping in salicylic acid (SA) degradation [94]. A plausible hypothesis is that the polymerization of catechol to melanin or its catabolism, could prevent this harmful compound from interacting with ROS activating enzymes. Despite the fact that benzoic acid (BZA) is used as a potent fungicide [95], L. theobromae growth was not inhibited in the presence of 15–30 mM of BZA (Additional file 17: Figure S7). No other carbon source was added to the medium VMM, suggesting that the fungus catabolizes BZA to sustain its growth. A marked increase in aerial mycelium and dark color was observed, indicating fungal melanin production [9698] and revealing a relationship between phenolic degradation and melanin production.

Furthermore, we found that IRCD and SH expression in vitro were induced in response to HS when GW was present (Additional file 14: Figure S6). The reason for this response is not clear, since the fungus had no contact with a living plant. However, it suggests a conserved and advantageous response of the fungus to HS, since the enzyme is produced before the plant SA burst starts. To test this hypothesis, the fungal expression in infected grapevine was evaluated and both genes showed significant up-regulation at each time course evaluated (Fig. 7), therefore SH and IRCD could be required for grapevine colonization by the fungus. In particular, fungal SH showed a defined up-regulation when compared heat stressed to none stressed plants at 7dpi (Fig. 7). It was already reported that SA is produced in grapevine to alleviate the photosynthesis impairment produced under HS [99], suggesting that the fungus, instead of using carbohydrate-derived carbon, switches its metabolism to degrade one of the major and readily available plant hormones, i.e. SA (schematic model in Fig. 9). Indeed, in Valsa mali-apple interaction, the fungal benzoate pathway was enriched, indicating an important function in pathogenicity in a lignified host tissue [100]. SH was previously associated with Ustilago maydis pathogenicity promotion in maize, suggesting that SA is used as either a carbon source or to repress the plant defense response signal [101]. Moniliophthora perniciosa, a pathogen of cacao, contains a gene coding for SH in its genome, which could explain the high tolerance of this pathogen to SA [102]. Furthermore, SH was one of the most expressed genes during the endosymbiont phase of E. festucae in grass, suggesting a role for evading the host SA-mediated response [103]. We propose that SH and IRCD activities, help L. theobromae to disrupt the SA defensive system involved in Systemic Acquired Resistance, using at the same time SA as carbon source (Fig. 10).

A metalloproteinase (comp1851_c0_seq1) showed the most significant up-regulation in response to HS (Additional file 9). Metalloproteinases have previously been observed to be up-regulated in the necrotrophic stage of the pathogenic fungus Moniliophthora roreri-Theobromae cacao interaction [104] and belong to an expanded gene family in pathogenic Onygenales [105], indicating a putative role of this enzyme in pathogenicity.

On other hand, an NmrA-like protein-encoding gene (comp1446_c0_seq2) was down-regulated only in the presence of GW, but up-regulated with HS. NmrA is part of a system controlling nitrogen metabolite repression in fungi, acting as a negative transcriptional regulator involved in the post-translational modification of the transcription factor AreA [106108]. The up-regulation of this gene upon HS, suggests a requirement for a different nitrogen source by fungal cells under thermal stress. Besides, AreA has been identified as an important regulator of secondary metabolism in Fusarium fujikuroi and F. graminearum [108, 109] and an NmrA-like protein was strongly up-regulated during a compatible stage in the M. oryzae-rice interaction [110], suggesting an important relationship between nitrogen metabolism and pathogenicity.

Other genes co-regulated with the NmrA-like protein and involved in nitrogen metabolism were a gene coding for an amino acid polyamine transporter I family (comp6363_c0_seq1) that is involved in amino acid/H+ transmembranal symport [111, 112] and several genes that belong to the MFS (comp23378_c0_seq1, comp7071_c0_seq1 and comp3035_c0_seq2) that are involved in general transport, including amino acid transport [113, 114]. The orthologs of genes encoding enzymes involved in L-tyrosine metabolism, HGD (comp8784_c0_seq1) and FMH (comp14342_c0_seq1), in Penicillium marneffei, showed regulation through AreA [77]. The above mentioned gene expression pattern suggests an important change in the general L. theobromae nitrogen metabolism as effect of HS.

Conclusions

The transcriptome of L. theobromae was established, providing nucleotidic sequences to the scientific community that will help to understand and eventually control this important pathogen. Based on functional annotation, several genes with putative functions in pathogenicity were identified, highlighting those encoding PCWDEs and involved in phenolic metabolism. Genes involved in melanin production were co-regulated with key transcription factors that control carbon and nitrogen usage, suggesting that strong metabolic and morphological changes occurs during fungal heat stress adaptation, in a similar manner to those documented for some fungal mammal’s pathogens.

Based on the in vitro L. theobromae global transcriptional regulation under HS, it was possible to identify fungal genes with up-regulation both in planta under optimum conditions and also with distinctive expression under HS, which helped to establish a model of the fungal-plant interaction under stress. These results indicated that HS overall facilitated L. theobromae growth and colonization. We propose that these observations are triggered by the fact that phenylpropanoid precursors increase under heat stress, and that L. theobromae is able to utilize these compounds for its own metabolism Although additional experiments are required to evaluate the robustness of the proposed model, this work provides the foundation to future research in order to understand the complexity of this important grapevine vascular pathogen.

Abbreviations

AML, putative amylase; BZA, benzoic acid; CHD, choline dehydrogenase; CTAB, cetyltrimethylammonium bromide; DEGs, differentially expressed genes; DEPC, dyethylpyrocarbonate; DHN; 1,8-dihydroxynaphthalene; DOPA, L-3,4-dihydroxyphenylalanine; dpi, days post-infection; FC, fold change; FDR, false discovery rate; FMH, fumarylacetoacetate hydrolase; GH, glycoside hydrolase; GH3, glycoside hydrolase family 3; GLM, General Linear Model; GMC, glucose-methanol-choline oxidorreductase; GO term, Gene Ontology functional term; GO, gene ontology; GW, grapevine wood; HGD, homogentisate dioxygenase; HPPD, 4- Hydroxyphenylpyruvate dioxygenase; HS, heat stress; HSP, heat-shock protein; ICP, isocitrate lyase phosphorylmutase; IMP, inosine monophosphate; IRCD, intradiol ring cleavage dioxygenase; MAI, maleylacetoacetate isomerase; MCO, multicopper oxidase; MFS, major facilitator superfamily; MS, malate synthase; NAP, nucleic acid preservation buffer; NCBI, National Center for Biotechnology Information; noHS, no heat stress; ORF, open reading frame; PCW, plant cell wall; PCWDEs, plant cell wall degrading enzymes; PDA, potato dextrose agar; PHI-base, Pathogen-Host interaction database; PL, pectate lyase; ROS, reactive oxygen species; RT-qPCR, reverse transcribed-quantitative PCR; SA, salicylic acid; SH, salicylate hydroxylase; SIT, sugar inositol transporter; TYR, tyrosinase; VMM, Vogel’s Minimal Medium; VS, Vogel’s salts; XGH, xylosidase glycoside hydrolase

Declarations

Acknowledgements

Marcos Paolinelli Alfonso received a doctoral scholarship from CONACYT (No. 231418) and a 2014–2015 UC MEXUS-CICESE Graduate Student Short Term Research and Non-degree Training. Authors would like to thank Douglas Gubler, Edgar Alfonso López Landavery, Miguel Angel del Río Portilla and Meritxell Riquelme Perez for helping with isolates, protocols or equipment. Sincere acknowledge to Martha Rendón Anaya, Miguel Ángel Hernández-Oñate and Raúl Llera for its helpful advises in bioinformatics analysis. Thanks to Jérôme Pouzoulet for kindly help with in planta experiments. Thanks to Meritxell Riquelme and Kristina Herbert for their critical review of the manuscript.

Funding

Research was funded by 2015 UC MEXUS-CONACyT Collaborative Research Grant, through the project “Interaction of the phytophatogenic fungus Lasiodiplodia theobromae with grapevine plants grown in thermic stress conditions”.

Availability of data and materials

The dataset supporting the conclusions of this article is available in the Gene Expression Omnibus (GEO) repository GSE75978.

Authors’ contributions

MPA, RHM, CGS, AHE and PR designed the experiments. MPA performed the experiments. MPA, JMVE and JFLH performed the bioinformatic analysis. CGS supervised the RT-qPCR, PR supervised the experiments on grapevine and AHE supervised the RNAseq experiment and bioinformatic analysis. RHM coordinated the experiments. MPA, RHM, PR, AHE and JMVE wrote the manuscript. All authors contributed in data analysis, read and approved the final version of the manuscript.

Competing interests

The authors declare that they have no competing interests.

Consent for publication

Not applicable.

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Authors’ Affiliations

(1)
Departamento de Microbiología, Centro de Investigación Científica y de Educación Superior de Ensenada (CICESE)
(2)
Laboratorio Nacional de Genómica para la Biodiversidad (LANGEBIO), Centro de Investigación y de Estudios Avanzados del I. P. N.
(3)
Department of Botany and Plant Sciences,University of California Riverside
(4)
Departamento de Biotecnología Marina, Centro de Investigación Científica y de Educación Superior de Ensenada (CICESE)

References

  1. Allen CD, Macalady AK, Chenchouni H, Bachelet D, McDowell N, Vennetier M, et al. A global overview of drought and heat-induced tree mortality reveals emerging climate change risks for forests. For Ecol Manage. 2010. doi:10.1016/j.foreco.2009.09.001.Google Scholar
  2. Teskey R, Wertin T, Bauweraerts I, Ameye M, McGuire MA, Steppe K. Responses of tree species to heat waves and extreme heat events. Plant Cell Environ. 2014. doi:10.1111/pce.12417.PubMedGoogle Scholar
  3. Allen CD, Breshears DD, McDowell NG. On underestimation of global vulnerability to tree mortality and forest die-off from hotter drought in the Anthropocene. Ecosphere. 2015. doi:10.1890/ES15-00203.1.Google Scholar
  4. Oliva J, Stenlid J, Martínez-Vilalta J. The effect of fungal pathogens on the water and carbon economy of trees: implications for drought-induced mortality. New Phytol. 2014. doi:10.1111/nph.12857.PubMedGoogle Scholar
  5. Desprez-Loustau M. Interactive effects of drought and pathogens in forest trees. Ann For Sci. 2006. doi:10.1051/forest:2006040.Google Scholar
  6. Moricca S, Ragazzi A. Fungal endophytes in Mediterranean oak forests: a lesson from Discula quercina. Phytopathology. 2008;98:381–6.View ArticleGoogle Scholar
  7. DiGuistini S, Wang Y, Liao NY, Taylor G, Tanguay P, Feau N, et al. Genome and transcriptome analyses of the mountain pine beetle-fungal symbiont Grosmannia clavigera, a lodgepole pine pathogen. Proc Natl Acad Sci U S A. 2011. doi:10.1073/pnas.1011289108.PubMed CentralPubMedGoogle Scholar
  8. Hammerbacher A, Schmidt A, Wadke N, Wright LP, Schneider B, Bohlmann J, et al. A common fungal associate of the spruce bark beetle metabolizes the stilbene defenses of Norway spruce. Plant Physiol. 2013. doi:10.1104/pp.113.218610.PubMed CentralPubMedGoogle Scholar
  9. Chong J, Poutaraud A, Hugueney P. Metabolism and roles of stilbenes in plants. Plant Sci. 2009. doi:10.1016/j.plantsci.2009.05.012.Google Scholar
  10. Singh B, Sharma RA. Plant terpenes: defense responses, phylogenetic analysis, regulation and clinical applications. Biotech. 2015. doi:10.1007/s13205-014-0220-2.Google Scholar
  11. Keller M. The science of grapevines: anatomy and physiology. San Diego: Elsevier; 2010.Google Scholar
  12. Úrbez-Torres JR. The status of Botryosphaeriaceae species infecting grapevines. Phytopathol Mediterr. 2011;50:5–45.Google Scholar
  13. Bertsch C, Ramírez-Suero M, Magnin-Robert M, Larignon P, Chong J, Abou-Mansour E, et al. Grapevine trunk diseases: complex and still poorly understood. Plant Pathol. 2013;62:243–65. doi:10.1111/j.1365-3059.2012.02674.x.View ArticleGoogle Scholar
  14. Urbez-Torres JR, Leavitt GM, Voegel TM, Gubler WD. Identification and distribution of Botryosphaeria spp. associated with grapevine cankers in California. Plant Dis. 2006. doi:10.1094/PD-90-1490.Google Scholar
  15. Úrbez-Torres JR, Leavitt GM, Guerrero JC, Guevara J, Gubler WD. Identification and pathogenicity of Lasiodiplodia theobromae and Diplodia seriata, the causal agents of Bot Canker disease of grapevines in Mexico. Plant Dis. 2008. doi:10.1094/PDIS-92-4-0519.Google Scholar
  16. Taylor A, Hardy GESJ, Wood P, Burgess T. Identification and pathogenicity of Botryosphaeria species associated with grapevine decline in Western Australia. Australas Plant Pathol. 2005;34:187–95.View ArticleGoogle Scholar
  17. Mahoney N, Lardner R, Molyneux RJ, Scott ES, Smith LR, Schoch TK. Phenolic and heterocyclic metabolite profiles of the grapevine pathogen Eutypa lata. Phytochemistry. 2003;64:475–84.View ArticlePubMedGoogle Scholar
  18. Rolshausen PE, Mahoney NE, Molyneux RJ, Gubler WD. A reassessment of the species concept in Eutypa lata, the causal agent of Eutypa Dieback of grapevine. Phytopathology. 2006. doi:10.1094/PHYTO-96-0369.PubMedGoogle Scholar
  19. Octave S, Roblin G, Vachaud M, Fleurat-Lessard P. Polypeptide metabolites secreted by the fungal pathogen Eutypa lata participate in Vitis vinifera cell structure damage observed in Eutypa dieback. Funct Plant Biol. 2006. doi:10.1071/FP05230.Google Scholar
  20. Rolshausen PE, Greve LC, Labavitch JM, Mahoney NE, Molyneux RJ, Gubler WD. Pathogenesis of Eutypa lata in grapevine: identification of virulence factors and biochemical characterization of cordon dieback. Phytopathology. 2008. doi:10.1094/PHYTO-98-2-0222.PubMedGoogle Scholar
  21. Blanco-Ulate B, Rolshausen PE, Cantu D. Draft genome sequence of the grapevine dieback fungus Eutypa lata UCR-EL1. Genome Announc. 2013. doi:10.1128/genomeA.00228-13.Google Scholar
  22. Sakalidis ML, Hardy GESJ, Burgess TI. Endophytes as potential pathogens of the baobab species Adansonia gregorii: a focus on the Botryosphaeriaceae. Fungal Ecol. 2011. doi:10.1016/j.funeco.2010.06.001.Google Scholar
  23. Slippers B, Wingfield M. Botryosphaeriaceae as endophytes and latent pathogens of woody plants: diversity, ecology and impact. Fungal Biol Rev. 2007. doi:10.1016/j.fbr.2007.06.002.Google Scholar
  24. Müllen JM, Gilliam CH, Hagen AK, Morgan JG. Canker of dogwood caused by Lasiodiplodia theobromae, a disease influenced by drought stress or cultivar selection. Plant Dis. 1991;75:886–9.View ArticleGoogle Scholar
  25. Álvarez-Loayza P, White JF, Torres MS, Balslev H, Kristiansen T, Svenning JC, et al. Light converts endosymbiotic fungus to pathogen, influencing seedling survival and niche-space filling of a common tropical tree, Iriartea deltoidea. PLoS One. 2011. doi:10.1371/journal.pone.0016386.PubMed CentralPubMedGoogle Scholar
  26. Andolfi A, Mugnai L, Luque J, Surico G, Cimmino A, Evidente A. Phytotoxins produced by fungi associated with grapevine trunk diseases. Toxins. 2011. doi:10.3390/toxins3121569.PubMed CentralPubMedGoogle Scholar
  27. Cobos R, Barreiro C, Mateos RM, Coque JJR. Cytoplasmic and extracellular proteome analysis of Diplodia seriata: a phytopathogenic fungus involved in grapevine decline. Proteome Sci. 2010. doi:10.1186/1477-5956-8-46.PubMed CentralPubMedGoogle Scholar
  28. Blanco-Ulate B, Rolshausen P, Cantu D. Draft genome sequence of Neofusicoccum parvum isolate UCR-NP2, a fungal vascular pathogen associated with grapevine cankers. Genome Announc. 2013. doi:10.1128/genomeA.00339-13.Google Scholar
  29. Morales-Cruz A, Amrine KCH, Blanco-Ulate B, Lawrence DP, Travadon R, Rolshausen PE, et al. Distinctive expansion of gene families associated with plant cell wall degradation, secondary metabolism, and nutrient uptake in the genomes of grapevine trunk pathogens. BMC Genomics. 2015. doi:10.1186/s12864-015-1624-z.PubMed CentralPubMedGoogle Scholar
  30. Vogel HJ. A convenient growth medium for Neurospora crassa. Microb Genet Bull. 1956;13:42–3.Google Scholar
  31. Camacho-Sanchez M, Burraco P, Gomez-Mestre I, Leonard JA. Preservation of RNA and DNA from mammal samples under field conditions. Mol Ecol Resour. 2013. doi:10.1111/1755-0998.12108.PubMedGoogle Scholar
  32. Reid KE, Olsson N, Schlosser J, Peng F, Lund ST. An optimized grapevine RNA isolation procedure and statistical determination of reference genes for real-time RT-PCR during berry development. BMC Plant Biol. 2006. doi:10.1186/1471-2229-6-27.PubMed CentralPubMedGoogle Scholar
  33. Vasanthaiah HKN, Katam R, Sheikh MB. Efficient protocol for isolation of functional RNA from different grape tissue rich in polyphenols and polysaccharides for gene expression studies. Electron J Biotechnol. 2008. doi:10.2225/vol11-issue3-fulltext-5.Google Scholar
  34. Paolinelli-Alfonso M, Galindo-Sanchez CE, Hernandez-Martinez R. Quantitative real-time PCR normalization for gene expression studies in the plant pathogenic fungi Lasiodiplodia theobromae. J Microbiol Methods. 2016. doi:10.1016/j.mimet.2016.05.021.PubMedGoogle Scholar
  35. Bolger AM, Lohse M, Usadel B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics. 2014. doi:10.1093/bioinformatics/btu170.PubMed CentralPubMedGoogle Scholar
  36. Andrews S. FastQC a quality control tool for high throughput sequence data. http://www.bioinformatics.babraham.ac.uk/projects/fastqc/.
  37. Grabherr MG, Haas BJ, Yassour M, Levin JZ, Thompson DA, Amit I, et al. Full-length transcriptome assembly from RNA-Seq data without a reference genome. Nat Biotechnol. 2011. doi:10.1038/nbt.1883.PubMed CentralPubMedGoogle Scholar
  38. Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990. doi:10.1016/S0022-2836(05)80360-2.PubMedGoogle Scholar
  39. Conesa A, Götz S, García-Gómez JM, Terol J, Talón M, Robles M. Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics. 2005. doi:10.1093/bioinformatics/bti610.PubMedGoogle Scholar
  40. Gotz S, Garcia-Gomez JM, Terol J, Williams TD, Nagaraj SH, Nueda MJ, et al. High-throughput functional annotation and data mining with the Blast2GO suite. Nucleic Acids Res. 2008. doi:10.1093/nar/gkn176.PubMed CentralPubMedGoogle Scholar
  41. Zdobnov EM, Apweiler R. InterProScan - an integration platform for the signature-recognition methods in InterPro. Bioinformatics. 2001. doi:10.1093/bioinformatics/17.9.847.PubMedGoogle Scholar
  42. Petersen TN, Brunak S, von Heijne G, Nielsen H. SignalP 4.0: discriminating signal peptides from transmembrane regions. Nat Methods. 2011. doi:10.1038/nmeth.1701.PubMedGoogle Scholar
  43. Krogh A, Larsson B, von Heijne G, Sonnhammer EL. Predicting transmembrane protein topology with a hidden Markov model: application to complete genomes. J Mol Biol. 2001. doi:10.1006/jmbi.2000.4315.PubMedGoogle Scholar
  44. Finn RD, Mistry J, Tate J, Coggill P, Heger A, Pollington JE, et al. The Pfam protein families database. Nucleic Acids Res. 2010. doi:10.1093/nar/gkp985.PubMed CentralGoogle Scholar
  45. Lima T, Auchincloss AH, Coudert E, Keller G, Michoud K, Rivoire C, et al. HAMAP: a database of completely sequenced microbial proteome sets and manually curated microbial protein families in UniProtKB/Swiss-Prot. Nucleic Acids Res. 2009. doi:10.1093/nar/gkn661.PubMed CentralGoogle Scholar
  46. Haas BJ, Papanicolaou A, Yassour M, Grabherr M, Blood PD, Bowden J, et al. De novo transcript sequence reconstruction from RNA-seq using the Trinity platform for reference generation and analysis. Nat Protoc. 2013. doi:10.1038/nprot.2013.084.PubMed CentralPubMedGoogle Scholar
  47. Winnenburg R, Baldwin TK, Urban M, Rawlings C, Köhler J, Hammond-Kosack KE. PHI-base: a new database for pathogen host interactions. Nucleic Acids Res. 2006. doi:10.1093/nar/gkj047.PubMedGoogle Scholar
  48. Langmead B, Salzberg SL. Fast gapped-read alignment with Bowtie 2. Nat Methods. 2012. doi:10.1038/nmeth.1923.PubMed CentralPubMedGoogle Scholar
  49. Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, et al. The sequence alignment/map format and SAMtools. Bioinformatics. 2009. doi:10.1093/bioinformatics/btp352.Google Scholar
  50. Robinson MD, McCarthy DJ, Smyth GK. edgeR: a Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics. 2010. doi:10.1093/bioinformatics/btp616.Google Scholar
  51. Bioconductor [http://www.bioconductor.org]
  52. R Development Core Team. R: A language and environment for statistical computing. 2008. http://www.R-project.org.Google Scholar
  53. Walter W, Sánchez-Cabo F, Ricote M. GOplot: an R package for visually combining expression data with functional analysis. Bioinformatics. 2015. doi:10.1093/bioinformatics/btv300.Google Scholar
  54. Dvinge H, Bertone P. HTqPCR: high-throughput analysis and visualization of quantitative real-time PCR data in R. Bioinformatics. 2009. doi:10.1093/bioinformatics/btp578.PubMed CentralPubMedGoogle Scholar
  55. O’Neil ST, Emrich SJ. Assessing De Novo transcriptome assembly metrics for consistency and utility. BMC Genomics. 2013. doi:10.1186/1471-2164-14-465.PubMed CentralPubMedGoogle Scholar
  56. Phillips AJL, Slippers B, Groenewald JZ, Crous PW. Plant pathogenic and endophytic Botryosphaeriales known from culture. Studies in Mycology 76. Utrecht: CBS-KNAW Fungal Biodiversity Centre; 2013. Google Scholar
  57. Islam MS, Haque MS, Islam MM, Emdad EM, Halim A, Hossen QMM, et al. Tools to kill: genome of one of the most destructive plant pathogenic fungi Macrophomina phaseolina. BMC Genomics. 2012. doi:10.1186/1471-2164-13-493.Google Scholar
  58. Albrecht D, Guthke R, Brakhage AA, Kniemeyer O. Integrative analysis of the heat shock response in Aspergillus fumigatus. BMC Genomics. 2010. doi:10.1186/1471-2164-11-32.Google Scholar
  59. Verghese J, Abrams J, Wang Y, Morano KA. Biology of the heat shock response and protein chaperones: budding yeast (Saccharomyces cerevisiae) as a model system. Microbiol Mol Biol Rev. 2012. doi:10.1128/MMBR.05018-11.PubMed CentralPubMedGoogle Scholar
  60. Xie X, Meehan MJ, Xu W, Dorrestein PC, Tang Y. Acyltransferase mediated polyketide release from a fungal megasynthase. J Am Che Soc. 2009. doi:10.1021/ja903203g.Google Scholar
  61. Bahn YS, Jung KW. Stress signaling pathways for the pathogenicity of Cryptococcus. Eukaryot Cell. 2013. doi:10.1128/EC.00218-13.PubMed CentralPubMedGoogle Scholar
  62. Davidson JF, Schiestl RH. Mitochondrial respiratory electron carriers are involved in oxidative stress during heat stress in Saccharomyces cerevisiae. Mol Cell Biol. 2001. doi:10.1128/MCB.21.24.8483-8489.2001.Google Scholar
  63. Morano KA, Grant CM, Moye-Rowley WS. The response to heat shock and oxidative stress in Saccharomyces cerevisiae. Genetics. 2012. doi:10.1534/genetics.111.128033.PubMed CentralPubMedGoogle Scholar
  64. Pócsi I, Prade RA, Penninckx MJ. Glutathione, altruistic metabolite in fungi. Adv Microb Physiol. 2004. doi:10.1016/S0065-2911(04)49001-8.PubMedGoogle Scholar
  65. Mullins MG, Bouquet A, Williams LE. Biology of the Grapevine. Cambridge: Cambridge University Press; 1992.Google Scholar
  66. Morais do Amaral A, Antoniw J, Rudd JJ, Hammond-Kosack KE. Defining the predicted protein secretome of the fungal wheat leaf pathogen Mycosphaerella graminicola. PLoS One. 2012. doi:10.1371/journal.pone.0049904.PubMed CentralPubMedGoogle Scholar
  67. Benoit I, Coutinho PM, Schols HA, Gerlach JP, Henrissat B, de Vries RP. Degradation of different pectins by fungi: correlations and contrasts between the pectinolytic enzyme sets identified in genomes and the growth on pectins of different origin. BMC Genomics. 2012. doi:10.1186/1471-2164-13-321.PubMed CentralPubMedGoogle Scholar
  68. Agrios G N. Plant Pathology. 5th Ed. Burlington: Elsevier Academic Press; 2005.Google Scholar
  69. Zhang Y, He J, Jia LJ, Yuan TL, Zhang D, Guo Y, et al. Cellular tracking and gene profiling of Fusarium graminearum during maize stalk rot disease development elucidates its strategies in confronting phosphorus limitation in the host apoplast. PLoS Pathog. 2016. doi:10.1371/journal.ppat.1005485.Google Scholar
  70. MacDonald J, Doering M, Canam T, Gong Y, Guttman DS, Campbell MM, et al. Transcriptomic responses of the softwood-degrading white-rot fungus Phanerochaete carnosa during growth on coniferous and deciduous wood. Appl Environ Microbiol. 2011. doi:10.1128/AEM.02490-10.Google Scholar
  71. Eklöf JM, Brumer H. The XTH gene family: an update on enzyme structure, function, and phylogeny in xyloglucan remodeling. Plant Physiol. 2010. doi:10.1104/pp.110.156844.PubMedPubMed CentralGoogle Scholar
  72. Eisenman HC, Mues M, Weber SE, Frases S, Chaskes S, Gerfen G, et al. Cryptococcus neoformans laccase catalyses melanin synthesis from both D- and L-DOPA. Microbiology. 2007. doi:10.1099/mic.0.2007/011049-0.PubMedGoogle Scholar
  73. Frases S, Salazar A, Dadachova E, Casadevall A. Cryptococcus neoformans can utilize the bacterial melanin precursor homogentisic acid for fungal melanogenesis. Appl Environ Microbiol. 2007. doi:10.1128/AEM.01947-06.PubMedGoogle Scholar
  74. Schmaler-Ripcke J, Sugareva V, Gebhardt P, Winkler R, Kniemeyer O, Heinekamp T, et al. Production of pyomelanin, a second type of melanin, via the tyrosine degradation pathway in Aspergillus fumigatus. Appl Environ Microbiol. 2009. doi:10.1128/AEM.02077-08.PubMedGoogle Scholar
  75. Chiang YM, Meyer KM, Praseuth M, Baker SE, Bruno KS, Wang CCC. Characterization of a polyketide synthase in Aspergillus niger whose product is a precursor for both dihydroxynaphthalene (DHN) melanin and naphtho-γ-pyrone. Fungal Genet Biol. 2011. doi:10.1016/j.fgb.2010.12.001.PubMedGoogle Scholar
  76. Upadhyay S, Torres G, Lin X. Laccases involved in 1,8-dihydroxynaphthalene melanin biosynthesis in Aspergillus fumigatus are regulated by developmental factors and copper homeostasis. Eukaryot Cell. 2013. doi:10.1128/EC.00217-13.PubMed CentralPubMedGoogle Scholar
  77. Liu D, Wei L, Guo T, Tan W. Detection of DOPA-melanin in the dimorphic fungal pathogen Penicillium marneffei and its effect on macrophage phagocytosis in vitro. PLoS One. 2014. doi:10.1371/journal.pone.0092610.Google Scholar
  78. Boyce KJ, McLauchlan A, Schreider L, Andrianopoulos A. Intracellular growth is dependent on tyrosine catabolism in the dimorphic fungal pathogen Penicillium marneffei. PLoS Pathog. 2015. doi:10.1371/journal.ppat.1004790.PubMed CentralPubMedGoogle Scholar
  79. Vasanthakumar A, DeAraujo A, Mazurek J, Schilling M, Mitchell R. Pyomelanin production in Penicillium chrysogenum is stimulated by L-tyrosine. Microbiology. 2015. doi:10.1099/mic.0.000030.PubMedGoogle Scholar
  80. Greene GH, McGary KL, Rokas A, Slot JC. Ecology drives the distribution of specialized tyrosine metabolism modules in fungi. Genome Biol Evol. 2014. doi:10.1093/gbe/evt208.PubMed CentralPubMedGoogle Scholar
  81. Tanaka A, Cartwright GM, Saikia S, Kayano Y, Takemoto D, Kato M, et al. ProA, a transcriptional regulator of fungal fruiting body development, regulates leaf hyphal network development in the Epichloë festucae-Lolium perenne symbiosis. Mol Microbiol. 2013. doi:10.1111/mmi.12385.PubMedGoogle Scholar
  82. Johnson GI, Mead AJ, Cooke AW, Dean JR. Mango stem end rot pathogens - Fruit infection by endophytic colonisation of the inflorescence and pedicel. Ann Appl Biol. 1992. doi:10.1111/j.1744-7348.1992.tb03420.x.Google Scholar
  83. Burgess TI, Barber PA, Mohali S, Pegg G, de Beer W, Wingfield MJ. Three new Lasiodiplodia spp. from the tropics, recognized based on DNA sequence comparisons and morphology. Mycologia. 2006. doi:10.3852/mycologia.98.3.423.PubMedGoogle Scholar
  84. Hwang L, Hocking-Murray D, Bahrami AK, Andersson M, Rine J, Sil A. Identifying phase-specific genes in the fungal pathogen Histoplasma capsulatum using a genomic shotgun microarray. Mol Biol Cell. 2003. doi:10.1091/mbc.E03-01-0027.PubMed CentralPubMedGoogle Scholar
  85. Nunes LR. Costa de Oliveira R, Leite DB, da Silva VS, dos Reis Marques E, da Silva Ferreira ME, et al. Eukaryot Cell: Transcriptome analysis of Paracoccidioides brasiliensis cells undergoing mycelium-to-yeast transition; 2005. doi:10.1128/EC.4.12.2115-2128.2005.Google Scholar
  86. Youngchim S, Nosanchuk JD, Pornsuwan S, Kajiwara S, Vanittanakom N. The role of L-DOPA on melanization and mycelial production in Malassezia furfur. PLoS One. 2013. doi:10.1371/journal.pone.0063764.PubMed CentralPubMedGoogle Scholar
  87. Pasricha S, Payne M, Canovas D, Pase L, Ngaosuwankul N, Beard S. Cell-type-specific transcriptional profiles of the dimorphic pathogen Penicillium marneffei reflect distinct reproductive, morphological, and environmental demands. G3 (Bethesda). 2013. doi:10.1534/g3.113.006809.Google Scholar
  88. Yang E, Wang G, Woo PCY, Lau SKP, Chow WN, Chong KTK, et al. Unraveling the molecular basis of temperature-dependent genetic regulation in Penicillium marneffei. Eukaryot Cell. 2013. doi:10.1128/EC.00159-13.Google Scholar
  89. Lorenz MC, Fink GR. The glyoxylate cycle is required for fungal virulence. Nature. 2001. doi:10.1038/35083594.PubMedGoogle Scholar
  90. Fraser CM, Chapple C. The phenylpropanoid pathway in Arabidopsis. Arabidopsis Book. 2011. doi:10.1199/tab.0152.84.PubMed CentralPubMedGoogle Scholar
  91. Van Wees SCM, Glazebrook J. Loss of non-host resistance of Arabidopsis NahG to Pseudomonas syringae pv. phaseolicola is due to degradation products of salicylic acid. Plant J. 2003;33:733–42.View ArticlePubMedGoogle Scholar
  92. Rudrappa T, Quinn WJ, Stanley-Wall NR, Bais HP. A degradation product of the salicylic acid pathway triggers oxidative stress resulting in down-regulation of Bacillus subtilis biofilm formation on Arabidopsis thaliana roots. Planta. 2007. doi:10.1007/s00425-007-0480-8.PubMedGoogle Scholar
  93. Broderick JB. Catechol dioxygenases. Essays Biochem. 1999;34:173–89.View ArticlePubMedGoogle Scholar
  94. Leatham GF, Crawford RL, Kirk TK. Degradation of phenolic compounds and ring cleavage of catechol by Phanerochaete chrysosporium. Appl Environ Microbiol. 1983;46:191–7.PubMed CentralPubMedGoogle Scholar
  95. Pagnussatt FA, Kupski L, Darley FT, Filoda PF, Del Ponte ÉM, Garda-Buffon J, et al. Fusarium graminearum growth inhibition mechanism using phenolic compounds from Spirulina sp. Ciência e Tecnol Aliment. 2013. doi:10.1590/S0101-20612013000500012.Google Scholar
  96. Choi YE, Goodwin SB. MVE1, encoding the velvet gene product homolog in Mycosphaerella graminicola, is associated with aerial mycelium formation, melanin biosynthesis, hyphal swelling, and light signaling. Appl Environ Microbiol. 2011;77:942–53.View ArticlePubMedGoogle Scholar
  97. Wu D, Oide S, Zhang N, Choi MY, Turgeon BG. ChLae1 and ChVel1 regulate T-toxin production, virulence, oxidative stress response, and development of the maize pathogen Cochliobolus heterostrophus. PLoS Pathog. 2012. doi:10.1371/journal.ppat.1002542.Google Scholar
  98. Yan X, Que Y, Wang H, Wang C, Li Y, Yue X, et al. The MET13 methylenetetrahydrofolate reductase gene is essential for infection-related morphogenesis in the rice blast fungus Magnaporthe oryzae. PLoS One. 2013. doi:10.1371/journal.pone.0076914.Google Scholar
  99. Wang LJ, Fan L, Loescher W, Duan W, Liu GJ, Cheng JS, et al. Salicylic acid alleviates decreases in photosynthesis under heat stress and accelerates recovery in grapevine leaves. BMC Plant Biol. 2010. doi:10.1186/1471-2229-10-34.Google Scholar
  100. Ke X, Yin Z, Song N, Dai Q, Voegele RT, Liu Y, et al. Transcriptome profiling to identify genes involved in pathogenicity of Valsa mali on apple tree. Fungal Genet Biol. 2014. doi:10.1016/j.fgb.2014.04.004.PubMedGoogle Scholar
  101. Rabe F, Ajami-Rashidi Z, Doehlemann G, Kahmann R, Djamei A. Degradation of the plant defence hormone salicylic acid by the biotrophic fungus Ustilago maydis. Mol Microbiol. 2013. doi:10.1111/mmi.12269.PubMedGoogle Scholar
  102. Mondego JMC, Carazzolle MF, Costa GGL, Formighieri EF, Parizzi LP, Rincones J, et al. A genome survey of Moniliophthora perniciosa gives new insights into Witches’ Broom Disease of cacao. BMC Genomics. 2008. doi:10.1186/1471-2164-9-548.PubMed CentralPubMedGoogle Scholar
  103. Ambrose KV, Tian Z, Wang Y, Smith J, Zylstra G, Huang B, et al. Functional characterization of salicylate hydroxylase from the fungal endophyte Epichloë festucae. Sci Rep. 2015. doi:10.1038/srep10939.PubMed CentralPubMedGoogle Scholar
  104. Meinhardt LW, Costa GGL, Thomazella DPT, Teixeira PJPL, Carazzolle MF, Schuster SC, et al. Genome and secretome analysis of the hemibiotrophic fungal pathogen, Moniliophthora roreri, which causes frosty pod rot disease of cacao: mechanisms of the biotrophic and necrotrophic phases. BMC Genomics. 2014. doi:10.1186/1471-2164-15-164.Google Scholar
  105. Li J, Zhang KQ. Independent expansion of zincin metalloproteinases in Onygenales fungi may be associated with their pathogenicity. PLoS One. 2014. doi:10.1371/journal.pone.0090225.Google Scholar
  106. Xiao X, Fu YH, Marzluf GA. The negative-acting NMR regulatory protein of Neurospora crassa binds to and inhibits the DNA-binding activity of the positive-acting nitrogen regulatory protein NIT2. Biochemistry. 1995;34:8861–8.PubMedView ArticleGoogle Scholar
  107. Andrianopoulos A, Kourambas S, Sharp JA, Davis MA, Hynes MJ. Characterization of the Aspergillus nidulans nmrA gene involved in nitrogen metabolite repression. J Bacteriol. 1998;180:1973–7.PubMedPubMed CentralGoogle Scholar
  108. Schönig B, Brown DW, Oeser B, Tudzynski B. Cross-species hybridization with Fusarium verticillioides microarrays reveals new insights into Fusarium fujikuroi nitrogen regulation and the role of AreA and NMR. Eukaryot Cell. 2008. doi:10.1128/EC.00130-08.PubMedPubMed CentralGoogle Scholar
  109. Giese H, Sondergaard TE, Sørensen JL. The AreA transcription factor in Fusarium graminearum regulates the use of some nonpreferred nitrogen sources and secondary metabolite production. Fungal Biol. 2013. doi:10.1016/j.funbio.2013.10.006.PubMedGoogle Scholar
  110. Kawahara Y, Oono Y, Kanamori H, Matsumoto T, Itoh T, Minami E. Simultaneous RNA-seq analysis of a mixed transcriptome of rice and blast fungus interaction. PLoS One. 2012. doi:10.1371/journal.pone.0049423.Google Scholar
  111. Jack DL, Paulsen IT, Saier MH. The amino acid/polyamine/organocation (APC) superfamily of transporters specific for amino acids, polyamines and organocations. Microbiology. 2000. doi:10.1099/00221287-146-8-1797.PubMedGoogle Scholar
  112. Vastermark A, Wollwage S, Houle ME, Rio R, Saier MH. Expansion of the APC superfamily of secondary carriers. Proteins. 2014. doi:10.1002/prot.24643.PubMed CentralGoogle Scholar
  113. Pao SS, Paulsen IT, Saier MH. Major facilitator superfamily. Microbiol Mol Biol Rev. 1998;62:1–34.PubMed CentralPubMedGoogle Scholar
  114. Xu X, Chen J, Xu H, Li D. Role of a major facilitator superfamily transporter in adaptation capacity of Penicillium funiculosum under extreme acidic stress. Fungal Genet Biol. 2014. doi:10.1016/j.fgb.2014.06.002.Google Scholar

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