Differential expression of maize chitinases in the presence or absence of Trichoderma harzianum strain T22 and indications of a novel exo- endo-heterodimeric chitinase activity
© Shoresh and Harman; licensee BioMed Central Ltd. 2010
Received: 22 July 2009
Accepted: 1 July 2010
Published: 1 July 2010
The interaction of plants with endophytic symbiotic fungi in the genus Trichoderma alters the plant proteome and transcriptome and results in enhanced plant growth and resistance to diseases. In a previous study, we identified the numerous chitinolytic enzyme families and individual enzymes in maize which are implicated in plant disease resistance and other plant responses.
We examined the differential expression of the entire suite of chitinolytic enzymes in maize plants in the presence and absence of T. harzianum. Expression of these enzymes revealed a band of chitinolytic enzyme activity that had greater mass than any known chitinase. This study reports the characterization of this large protein. It was found to be a heretofore undiscovered heterodimer between an exo- and an endo-enzyme, and the endo portion differed between plants colonized with T. harzianum and those grown in its absence and between shoots and roots. The heterodimeric enzymes from shoots in the presence and absence of T. harzianum were purified and characterized. The dimeric enzyme from Trichoderma-inoculated plants had higher specific activity and greater ability to inhibit fungal growth than those from control plants. The activity of specific chitinolytic enzymes was higher in plants grown from Trichoderma treated seeds than in control plants.
This is the first report of a dimer between endo- and exochitinase. The endochitinase component of the dimer changed post Trichoderma inoculation. The dimer originating from Trichoderma inoculated plants had a higher antifungal activity than the comparable enzyme from control plants.
Trichoderma spp. are opportunistic root colonizing fungal plant symbionts  that induce numerous changes in plant gene expression and physiology. Among the phenotypic changes are increased systemic resistance to plant diseases [1–8]; increased growth of plants and roots, including an increase in fertilizer use efficiency and uptake [9–12]; and a generalized increase in resistance to abiotic stresses [1, 13].
We recently completed an analysis of the proteome of maize plants in the presence or absence of T. harzianum strain T22 [11, 14]. Even though T22 was present only on roots, there were 141 proteins that we identified as up-regulated and 50 that were down-regulated in shoots , while in roots 20 up-regulated and 11 down-regulated proteins were found . A large portion of the up-regulated proteins were involved in carbohydrate metabolism, while a number of others were involved in photosynthesis or resistance to stress. In addition, starch accumulation in maize plants whose roots were colonized with T22 was greater than in the control . We suggested that Trichoderma induces both increased growth, which is mediated by an increase in photosynthetic and respiratory rates, and systemic induced resistance .
In an earlier study we determined that maize root colonization enhanced expression of chitinolytic enzyme activity . This is frequently assumed to be part of induced systemic resistance . However, in our proteomic studies, we did not identify up- or down-regulation of chitinolytic enzymes, probably primarily because we examined proteins with isoelectric points between 5.3 and 7.5, and the pIs of most chitinolytic enzymes are more basic or acidic than these levels. Prior to a recent study , only seven endochitinases and four partial sequences of exochitinases were identified. Using a combination of in silico and expression analyses, we identified putative 27 endochitinase genes (glycosyl hydrolases families 18 and 19) and four exochitinases (GH20; β-N-acetylhexosaminidases). The full sequences of these genes, domain analyses, and, in many cases, chromosomal locations were identified for these genes .
The chitinolytic enzyme families in plants and microbes are quite complex. They may cleave the chitin or other substrate molecules randomly or a single residue from the non-reducing end of the chitin molecule. These two types are commonly referred to as chitinases (endo-β-N-acetylglucosaminidase; EC 220.127.116.11) and exochitinases (β-N-acetylhexosaminidase; EC. 18.104.22.168). To avoid confusion, hereafter we will refer to the EC 22.214.171.124 enzymes as endochitinases and the 126.96.36.199 proteins as exochitinases, and any protein with enzymatic activity against chitin as a chitinolytic enzyme .
Given the great diversity of chitinolytic enzymes in plants, it is not very useful to simply quantify total chitinolytic enzyme activity as a quantitative measure of induced resistance or other factors. The total activity probably indicates little regarding the specific functionality of any individual gene product. In terms of disease resistance, as measured by antifungal activity, the differences between exo- and endo enzymes is quite large. In general, endochitinases have greater activity than exochitinases but mixtures of fungal endo and exo-acting enzymes usually are synergistic, and on a per unit protein basis, a combination of exo and endo enzymes usually are several-fold more active than any single enzyme [18, 19].
In the course of our expression analyses of chitinolytic enzymes in maize with and without T22, we noted a chitinolytic enzyme band with a mass substantially larger than any expected gene product of the 31 different genes we identified in maize. This protein is a heterodimeric enzyme composed of an exo- and an endo-acting enzyme. Such heterodimers have not been heretofore described, and they may be of substantial importance since the heterodimeric enzyme would be expected to have substantially greater antifungal activity than any single protein. Moreover, the endo portion of the heterodimer differs in plants grown in the presence and in the absence of T22.
This paper describes the characterization of the differential expression of chitinolytic enzymes in maize with and without T22, the isolation of the heterodimeric enzyme from T22-treated and untreated plants and describes its very high antifungal activity.
Chitin degrading enzymes of maize are different in shoots and roots and in the presence and absence of T. harzianum
In roots, activity bands were observed to be 95 kDa and 23 kDa in both control and Trichoderma-treated plants in samples that were heated only to 55°C (Fig. 1B). However, no known chitinolytic enzymes have a molecular weight as large as 95 kDa. After boiling, only one activity band was observed at ca. 30 kDa. This suggested the possibility that the 95 kDa chitinolytic activity band is a complex of proteins.
Quantitative analysis of the fluorescence was performed using NIH-image software. Three independent repeats were performed and equal loading was used in each lane. In addition three major bands in each lane were quantified in the Coomassie stained images. These were used to verify equal loading and as a normalizing reference. In most cases the level of chitinolytic activity was 2- to 5-fold higher in plants grown from T22 treated seeds than from control seeds (Fig. 1C and 1D).
Identification of chitinolytic enzymes
Identification of chitinases from the activity bands.
No chitinase identified
No chitinase identified
No chitinase identified
No chitinase identified
No chitinase identified
No chitinase identified
Exo2 was the only protein identified in all tissues and treatments examined. ChiIVA and ChiIVB were identified only in shoots of control plants. ChiIII9675 and ChiI11654 were identified only in shoots from Trichoderma treated plants. ChiI67336 was identified in shoots of both control plants and those grown from seeds treated with T. harzianum. ChiIII9615 was identified in roots of both control plants and Trichoderma inoculated plants.
The molecular weights of the identified proteins fit their position in the gel supporting their identification, with the exception of the 95 kDa protein mentioned earlier. The LC/MS/MS data indicated that this band contained two enzymes; an endochitinase with a mass of a ca. 30 kDa and the other was Exo2 with a mass of 66 kDa (Table 1). This suggested that the protein in this band could be a heterodimer between Exo2 and an endochitinase. The endochitinase in this putative dimer differed according to the source of the tissue--the enzyme identified in shoots in the presence (ChiIII9675) and absence (ChiIVA) of T22 was different and it differed again between roots (ChiIII9615) and shoots of control plants (Table 1).
Purification of the heterodimeric proteins from shoots
Specific activity of chitinase preparations
MUB based Activity
MUA based Activity
Total extracted protein
Rotofor fraction 4
Purified dimeric protein
In order to dissociate the dimers to their components the isolated dimers were boiled for 10 min in the presence of a reducing agent (50 mM TCEP·HCl). While boiling completely abolished activity, it did not completely dissociate the dimers into their components under these conditions. However, faint bands were observed at the sizes of 65 kDa and 30 kDa which are at the expected sizes of the exochitinase and the endochitinase identified by the LC/MS/MS from these 95 kDa proteins (Fig. 2C, Dimer panel, boiled). It is also worth noticing that the intensities of the dissociated bands were stronger for the dimer derived from control plants than the dimer derived from Trichoderma-treated plants. This may suggest that under these conditions dissociation of the control dimer is easier.
Antifungal activity against Penicillium digitatum
Chitinolytic enzymes in plants are numerous and highly diverse, including those in maize. The enzymes are arranged in various classes and into endo- and exo-acting enzymes based on domain analyses and sequence motifs. The classification of enzymes in Table 1 and in this paper is based on this sequence information; we recently have described the maize chitinolytic enzymes and published the sequences of the 27 endochitinases and four exochitinases from maize . This study demonstrates that root colonization by T. harzianum not only results in changes in shoot and root chitinolytic enzyme activity levels as we have described earlier  but that qualitative changes also are induced. These data suggest that the chitinolytic enzymes in maize are under complex regulatory control and that T. harzianum induces changes in this regulation. Previous study has demonstrated that in our system Trichoderma is present only on roots . Thus, observed changes in proteins in shoots are a consequence of systemic induction by T. harzianum, which has been noted in other studies as well [2, 6, 8, 11, 21, 22]. Probably our assessment of the presence or absence of various chitinolytic enzymes is an underestimate, since we were able to identify only 10 of the activity bands.
There are so many chitinolytic enzymes, probably many with unknown physiological function, and therefore determination of total activity is not very useful. In many studies, only changes in total chitinolytic activity were measured [8, 15]. In other cases, one, or at most a few, of the enzymes that may be produced in plant systems were studied [23–25]. A few studies have been more comprehensive; for example, a study on sugar cane pathogenesis examined four chitinases  and a study in rice examined distribution, structure, organ-specific expression and phylogenetic analysis of 12 chitinase III enzymes . However, so far as we can ascertain, there are no fully comprehensive studies on the role of the total mixture of chitinolytic enzymes or genes in any plant process.
Two endochitinases, which were identified in the activity bands in this study, were previously shown to have antifungal properties . Chitinolytic enzymes are no doubt important in pathogenesis [28, 29, 31–33]. Overexpression, or high level expression of heterologous chitinolytic enzymes, alone or in combination with other antifungal proteins frequently results in protection against pathogens [19, 34–40]. The enhanced protection by the chitinases could be due to direct inhibition of fungal growth or due to induction of plant defense responses by the GlcNAc oligomers generated by their activity . However, in other studies modulation of chitinase expression did not change the resistance of plants pathogens [42, 43]. This suggests that chitinases may also have other roles (as demonstrated by [44, 46–50]). Hence total activity of chitinases does not necessarily represent antifungal activity and a study of specific chitinases could greatly contribute to our understanding of their role.
Several Trichoderma strains induce the Induced Systemic Resistance (ISR) pathway [4, 6] and others are suspected to induce the systemic acquired resistance (SAR) pathway . These data suggest that different pathways of induced resistance may be activated by the presence of different strains. Expression profiles may be more complex when adding effects of pathogens in plants colonized or not colonized by Trichoderma. In cucumber, very different responses were identified in plants infected with the bacterial pathogen Pseudomonas syringae pv. lachrymans after root colonization by T. asperellum  than with the biocontrol agent alone. Thus, altered profiles of the complex mixture of chitinolytic enzymes are likely to be discovered by different combinations of Trichoderma strains and pathogens. It appears to be a very good system to examine the total potential of plants to express induced resistance and changes in chitinolytic enzymes can provide good markers for these differential responses.
In the course of the current research, we found an activity band with chitinolytic activity that was larger than the protein that would be expressed by any gene that we had identified. The molecular range of all identified maize chitinolytic enzymes is 55-66 kDa for exochitinases and 16-35 kDa for endochitinases. This indicated that none of these could be the sole constituent of this high molecular weight band. To our surprise LC/MS/MS identified an exochitinase, Exo2, together with different endochitinases, depending on the treatment and tissue type. The mass of this 95 kDa protein was equal to the sum of the exo- and endo-chitinases detected by LC/MS/MS and the activity of this band disappeared upon boiling. These data suggested that the 95 kDa protein was, in fact, a heterologous dimer between an exochitinase (Exo2) and an endochitinase (ChiIII9675 or ChiIVA, in the shoot). An exochitinase purified from mungbean was shown to exist in a hetero-dimeric form with an unknown protein . Thus, we have identified novel heretofore unknown heterodimer comprised of an exochitinase and an endochitinase. Although the dimers were identified in vitro from plant extracts we hypothesize they may have an in vivo significance, for example, in plant defense.
We were intrigued by the appearance of the different endochitinase constituents in the dimer in the presence or absence of T. harzianum and their possible role in plant defense, especially since endochitinases and exochitinases were shown to possess synergistic antifungal activity in mixtures [19, 34]. Since the specific chitinolytic activity of the dimeric protein in Trichoderma-treated plants is higher than from control plants, this suggested that the dimer from treated plants might possess higher antifungal activity. This was confirmed since the purified enzyme from shoots of Trichoderma-treated plants was about twice as effective in preventing germination of fungal conidia as was the corresponding protein from control plants. Similarly, lower concentrations of the Trichoderma-derived enzymes were required to cause obvious cell wall damage in germlings of Penicillium digitatum. There are no reports on ChiIII9675, which is one of the components of the Trichoderma-induced heterodimer, but the monomeric maize ChiIVA has antifungal activity . There has been a great deal of interest in producing disease-resistant transgenic plants that express chitinases. For example, Trichoderma chitinases, when introduced transgenically into plants, induce resistance against a range of plant pathogenic fungi [19, 34, 35]. Although tested here only against one fungal model system further study of the dimers activity against other fungal pathogens is under way. Yet, the genes encoding these maize enzymes would appear to be good candidates for such uses since they are derived from a food plant, and therefore may be more acceptable than ones from microbial sources. The mechanisms by which Trichoderma spp. induce plants to be more resistant to disease is just now being understood. It could be that the change in chitinase activity profile and the formation of dimers with higher activity are part of this mechanism. It is likely, but unknown, whether these dimers exist in other plants. The in vivo role of these dimeric chitinase proteins in inducing resistance in plants to fungal attack deserves further attention.
Using chitinase activity assays and gel-based proteomic approach we characterized the differential expression of the entire suite of chitinolytic enzymes in shoots and roots of maize plants in the presence and absence of T. harzianum. We further isolated heretofore undiscovered heterodimeric proteins which include an endo- and exochitinase constituents. Change of the endochitinase component of the dimer resulted in change of the enzymatic activity.
Materials and methods
Plant and fungal material
Seeds of maize (Zea mays L.) inbred Mo17 were treated with Trichoderma harzianum Rifai strain 22 (T22) in a cellulose-dextran formulation (1-2 × 109 cfu/g)  or were treated with water. Previous work with application of the cellulose-dextran powder without T22 gave no observable difference than water application (data not shown). The cellulose-Trichoderma powder was suspended in water (38.5 mg/5 ml) and 100 μl were applied to 5g of seeds. Seeds were planted in sandy loam field soil in boxes (10.5 × 10.5 × 6 cm) with five seeds per box. Seed treatments with T22 result in colonized roots, but the organism does not grow on or in shoots . Boxes were incubated in a growth chamber with diurnal fluorescent lighting with 16 h/8 h (light/dark cycle), at 22 ± 4°C, and watered as needed. Seven-day-old seedlings were harvested: the shoots were first measured for heights and then excised 1 cm above soil level, frozen immediately in liquid nitrogen and stored at -70°C until use.
Shoot tissue samples were ground with liquid nitrogen followed by further grinding in 9 ml of ice cold 0.1 M HEPES and 2% dithiothreitol (DTT) per 3 g tissue powder using an Ultra-Turrax homogenizer (Janke & Kunkel). Two repeats with a total of about 10 g shoot tissue each were processed for each treatment. For ca. 10 g of control plants, 55 plants were used. For Trichoderma-treated plants, 40 plants were used to get ca. 10 g of tissue. The homogenate was then centrifuged for 20 min at 15000 pm at 4°C. Proteins were precipitated from the supernatant by adding 8 volumes of ice-cold acetone and incubating 16 h at -20°C. After another centrifugation the precipitated proteins were washed twice with 2 ml of ice-cold acetone followed by drying under a flow of N2. Powder was than dissolved in sample solubilization buffer (100 mM sodium acetate pH5.5, 10 mM EDTA, 0.1 mM DTT). A small aliquot was diluted 50-fold with water and the protein content was determined using Coomassie Plus Protein Assay (Pierce) according to manufacturer's instructions.
PAGE and in-gel chitinase activity assay
SDS-polyacrylamide gel electrophoresis (SDS-PAGE) was employed to assess the relative amounts and banding patterns of the chitinases in protein samples. Protein samples were mixed with 25% by volume of loading dye (15% sucrose; 2.5% SDS; 125 mM Tris-HCl, pH 6.7; 0.01% Bromo-phenol Blue), loaded on a 4% acrylamide stacking gel and separated in a 12% acrylamide gel using a Mighty Small II electrophoresis system (Amersham). Gels were then used for in-gel chitinase activity or stained with Coomassie or silver stain using standard procedures.
Basic-native PAGE (native-PAGE) was used to isolate the protein from the piece of gel harboring the chitinase activity assay. Protein samples were mixed with 1/5 of loading dye (100 mM of Tris-HCl, pH 6.8; 50% glycerol; 0.01% Bromo-phenol Blue) and were loaded on a 4% acrylamide stacking gel with 50 mM of Tris (pH 6.8) and separated using a 10% acrylamide gel with 360 mM of Tris-HCl (pH 8.9). The running buffer contained 50 mM Tris-Base and 380 mM glycine, pH 8.9. Proteins were separated for about 5 h at a constant 30 mA/gel with cooling.
Before the in-gel chitinase activity assay, native gels were washed with acetate buffer (100 mM, pH 5.0) for 20 min. SDS-gels were washed three times in renaturation buffer (40 mM Tris-HCl, pH 9.0; 2 mM EDTA; 1% casein) for 30 min per wash and then washed for 20 min in 100 mM sodium acetate buffer (pH 5.0) with 1% (v/v) purified Triton-X100. This was followed by two washes with 100 mM sodium acetate buffer (pH 5.0) for 15 min each. Similar procedures have long been used to renaturate chitinolytic enzymes following treatments appropriate for SDS-PAGE gels (Trudel and Asselin, 1989).
Gels were then stained for chitinase activity by overlaying with 1% low melting (≤35°C gelling temperature) agarose that contained methylumbelliferyl substrate in 100 mM acetate buffer (pH 5.0). Substrates used were 4-methylumbelliferyl-N-acetyl-β-D-glucosaminide (MUA; 20 ng/ml), 4-methylumbelliferyl-N-acetyl-β-D-N, N', N"-triacetylchitotrioside (MUB; 16.6 ng/ml), 4-methylumbelliferyl-N-acetyl-β-D-N, N'-diacetylchitobioside (MUC; 10 ng/ml) and 4-methylumbelliferyl N-acetyl-β-D-N, N', N"N'''-tetraacetylchitotetraoside (MUD; 10 ng/ml) (Sigma, St. Louis, MO). Agarose was melted in a microwave oven and kept in a water bath at 37°C and substrates were added prior to application. Gels were kept at room temperature and the activity bands were observed after 2, 15 and 30 min under UV light. Following photo imaging of chitinase activity banding patterns, the agarose layer was gently removed from gel and gels were rinsed in deionized water and stained for protein profiles by coomassie or silver staining using standard procedures.
For dissociation of dimers, tris(2-carboxyethyl) phosphine (TCEP·HCl) was added to a final concentration of 50 mM with the sample buffer and protein samples were boiled for 10 min before loading on the gel.
Proteins were separated according to their pI using a Rotofor Cell (Bio-Rad) according to manufacturer's instructions. Before separation proteins were dissolved in 2% ampholyte (Bio-Lyte 5/8, Bio-Rad) and 1% purified Triton X-100. Twenty fractions were collected and the pH of each fraction was recorded. Proteins were precipitated with addition of 8 volumes of cold acetone and incubated 16 h at -20°C. After 20 min of centrifugation at 15000 rpm at 4°C, pellets were washed twice with cold acetone and dissolved in 250 μl of 100 mM sodium acetate (pH 5.0). Three μl were diluted 1:10 in water and the dilutions were used to measure protein concentration and chitinase activity (in 96-well plates).
Chitinolytic enzyme activity assay in plates
Chitinolytic activities were quantified in 96-well plates. In each well 10 μl of BSA, 30 μl of tested sample (at the desired dilution) and 30 μl of substrate (0.2 mM of either MUA or MUB) were added, keeping the plate on ice. The plate was then covered, sealed in a plastic bag and incubated for 30 min at 37°C. The reaction was stopped with 30 μl of 1 M sodium carbonate and the fluorescence was determined at 360/460 (excitation/emission) with a CytoFluor II fluorescence multiwell plate reader. Fluorescence of known concentrations of 4-methylumbeliferone (Sigma) was used to plot a standard curve to determine the activity of the chitinase in samples tested. The activity was defined as micromolar methylumbeliferone released per min per microgram of protein.
Extraction of proteins from acrylamide gels
Activity bands were cut out of the native gels (care was taken to obtain pieces that were as narrow as possible). Gel bands were mashed through a nylon mesh (SpectraMesh poly; Spectrum Medical Industries, Los Angeles, CA). After addition of 100 μl water, the gel was left overnight at 4°C with occasional mixing. Mashed gels were loaded on glass fiber columns (3 mm height) and centrifuged at maximum for 5 min. The eluted protein was transferred to a new tube and 50 μl of water were added to the column. After incubation of 1 h at room temperature, centrifugation was repeated.
Mass-spectrometry analysis and protein identification
Proteins were identified by peptide sequencing using nanospray ion-trap tandem mass spectrometry (nESI-IT MS/MS). The nESI-IT MS/MS experiments were performed on an LC Packings (Dionex)/4000 Q Trap (Applied Biosystems) in positive ion mode. Protein identification was carried out using the PMF - GPS Explorer, ESI - Analyst (Applied Biosystems) software. Non-redundant NCBI (National Center for Biotechnology Information, W) and SwissProt (European Bioinformatics Institute, Heidelberg, Germany) databases as well as our local chitinase sequences database were used for the search. Searches were performed in the full range of Mr and pI. Positive identification was considered only for C.I.% of ≥95%.
Antifungal assays were conducted in 96-well plates using a standard assay . Each well contained a spore suspension of Penicillium digitatum (1000 spores per well) and purified dimer at different concentrations in a final volume of 30 μl in 1/3 strength PDB (potato dextrose broth, Difco). Extraction from an empty gel was performed and this solution was added in place of enzyme solutions for the control. The microplates were incubated for 16-18 h at 25°C. Observations following incubation were taken directly from the microplate wells under a Nikon Diaphot brightfield microscope (Nikon Inc., Melville, NY, U.S.A.). The percentage of conidia germinated was determined based on a screen focused to the center of the well. Microscope slides were also prepared for observation at higher levels of magnification. Abnormal mycelial growth and morphological anomalies such as branching, bursting, appearance of necrotic zones, and lysis of the hyphal tips were recorded and photographed. The assay was repeated independently on two separate days.
This research was supported in part by the US-Israel Agricultural Research and Development fund (BARD) grant US-3507-04 R and by Advanced Biological Marketing (Van Wert, Ohio).
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