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Review

Bioactive Secondary Metabolites from Trichoderma spp. against Phytopathogenic Fungi

by
Raja Asad Ali Khan
1,
Saba Najeeb
1,
Shaukat Hussain
2,
Bingyan Xie
1,* and
Yan Li
1,*
1
Institute of Vegetables and Flowers (Plant Pathology Lab), Chinese Academy of Agricultural Sciences, Beijing 100081, China
2
Department of Plant Pathology, The University of Agriculture Peshawar, Peshawar 25130, Pakistan
*
Authors to whom correspondence should be addressed.
Microorganisms 2020, 8(6), 817; https://doi.org/10.3390/microorganisms8060817
Submission received: 2 April 2020 / Revised: 5 May 2020 / Accepted: 28 May 2020 / Published: 29 May 2020
(This article belongs to the Section Plant Microbe Interactions)
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Abstract

:
Phytopathogenic fungi, causing significant economic and production losses, are becoming a serious threat to global food security. Due to an increase in fungal resistance and the hazardous effects of chemical fungicides to human and environmental health, scientists are now engaged to explore alternate non-chemical and ecofriendly management strategies. The use of biocontrol agents and their secondary metabolites (SMs) is one of the potential approaches used today. Trichoderma spp. are well known biocontrol agents used globally. Many Trichoderma species are the most prominent producers of SMs with antimicrobial activity against phytopathogenic fungi. Detailed information about these secondary metabolites, when grouped together, enhances the understanding of their efficient utilization and further exploration of new bioactive compounds for the management of plant pathogenic fungi. The current literature provides the information about SMs of Trichoderma spp. in a different context. In this review, we summarize and group different antifungal SMs of Trichoderma spp. against phytopathogenic fungi along with a comprehensive overview of some aspects related to their chemistry and biosynthesis. Moreover, a brief overview of the biosynthesis pathway, action mechanism, and different approaches for the analysis of SMs and the factors affecting the regulation of SMs in Trichoderma is also discussed.

1. Introduction

Plant pathogens cause significant losses, which have obstructed efforts to increase agricultural production. In spite of remarkable achievements in the development of chemical pesticides, plant breeding technologies, and different cultural practices, as well as other management strategies for the control of plant pathogens, losses due to disease remain a limiting factor in agricultural production throughout the world, including many developed countries [1]. Among plant pathogens, phytopathogenic fungi are one of the main infectious agents in plants, causing significant economic and production losses. Throughout the history of agriculture, plant pathogenic fungi have been devastating threats and the most diverse group of economic and ecological threats [2].
Several management strategies have been utilized for the control of fungal plant pathogens, including the use of chemical fungicides, the breeding of disease resistance varieties, and several other cultural practices. The excessive and continuous use of chemical fungicides cause serious hazardous concerns related to human, animal, and environmental health. Breeding for disease resistance is a long-lasting process. Though resistance genes have been incorporated successfully in plants for disease management, breeding has to be a continuous process because the pathogens evolve rapidly, break the resistance, and plants become susceptible. In advanced agriculture, most of the fungal plant pathogens can be controlled by modern management practices but epidemics with huge yield losses still occur. Recently, wheat blast outbreaks (Magnaporthe oryzae) and soybean rust (Phakopsora pachyrhizi) in several Asian countries caused devastating yield losses [3]. There is a need to explore alternate management strategies. The use of biological control agents and their secondary metabolites is one of the potential approaches that is consumer and environmentally friendly.
Secondary metabolites (SMs) from microorganisms may have an antifungal role against agriculturally important phytopathogenic fungi [4]. Among different microorganisms, the species of the genus Trichoderma are the most potent biocontrol agents in use today because they produce a diverse range of antimicrobial SMs [5,6]. Trichoderma species secrete a plethora of metabolites into their vicinity while having minimal nutritional needs. These metabolites can be utilized for agricultural, industrial, and medical benefits and hence are important to humans. Several Trichoderma spp. exhibit antifungal activities against phytopathogenic fungi [7], in which different groups of SMs, such as terpenes, pyrones, gliotoxin, gliovirin, and peptaibols may be involved [8]. Comprehensive information about these SMs regarding their antifungal role against phytopathogenic fungi, when grouped together, will enhance the understanding of their efficient utilization and further exploration of new antifungal bioactive metabolites for the management of plant pathogenic fungi. The current literature provides the information about SMs of Trichoderma spp. in a different context [9,10,11,12]. In this review article, we summarize and group different antifungal SMs of Trichoderma spp. against phytopathogenic fungi, along with a comprehensive overview of some aspects related to their chemistry and biosynthesis. In addition, a brief overview of different approaches for the analysis of SMs, the mechanism of action of SMs, the general biosynthesis pathway, and factors influencing SM regulation in Trichoderma is also discussed.

2. Antifungal SMs Produced by Trichoderma spp.

2.1. Epipolythiodioxopiperazines

Epipolythiodioxopiperazines (ETPs) have a high reactive potential among fungal SMs and are characterized by a diketopiperazine ring that originates from a peptide. Diketopiperazines (DKPs) are considered the product of protein degradation and they were generally nonpreferred peptides because they are synthesized from protein hydrolysates. The toxicity of ETPs is attributed to their disulphide bridges, which bind to thiol groups and generate reactive oxygen species through redox cycles, and in this way inactivate proteins [13]. In the past few years, scientists diverted more towards DKP research because of their strong biological activities. Many DKPs from microorganisms were isolated and studied for their biological activities. The first DPK gliotoxin (1) (Figure 1) was isolated from Trichoderma lignorum in 1936 [14], while a further description of gliotoxin was made from Trichoderma viride in 1944 [15]. Subsequent isolations and biosynthetic analyses have also been performed from this strain [16,17]. In 1975, Hussain et al. also isolated this compound from Trichoderma hamatum. Gliotoxins exhibit bioactivity against the human pathogenic fungus Aspergillus fumigatus, but also play important roles in the biocontrol activity of Trichoderma virens against some plant pathogenic fungi [18,19]. Some biocontrol strains (so-called Q-strains) of T. virens also produce gliotoxin [20]. For example, gliotoxin isolated from T. virens ITC-4777 was active against Rhizoctonia bataticola (with an ED50 of 0.03 g/mL), Macrophomina phaseolina (with an ED50 of 1.76 g/mL), Pythium deharyanum (with an ED50 of 29.38 g/mL), Pythium aphanidermatum (with an ED50 of 12.02 g/mL), Sclerotium rolfsii (with an ED50 of 2.11 g/mL), and Rhizoctonia solani (with an ED50 of 3.18 g/mL) [21]. Gliovirin (Figure 1; 2) is another member of this class of toxin, produces mainly by a strain of T. virens [22]. Two analogues of gliovirin (Figure 1; 2a, 2b) were isolated from Trichoderma longibrachiatum. These analogues exhibited antifungal activity against R. solani [23]. Strains of T. virens that produce gliotoxin also showed antagonistic activity against R. solani [24], while those strains that produce gliovirin were antagonistic to Pythium ultimum [25]. Both gliovirin and gliotoxin come under the epipolythiodioxopiperazine class of toxins and exhibited characteristic disulphide bridges [26]. The DKP gliotoxin gene cluster in the T. virens genome comprises eight genes, a cluster-specific regulator, auxiliary biosynthetic enzymes, and nonribosomal peptide synthetase (NRPS); dioxopiperazine synthetase [20]. The removal of a part from the gliP open reading frame confirmed the association of the gene cluster with gliotoxin production [27]. The gliP mutants that were unable to produce gliotoxin showed less activity against P. ultimum while exhibiting a higher vegetative growth rate [18]. Unexpectedly, another six genes of the gli cluster and gliP were also reported in the genome of T. reesei, but this species does not produce gliotoxin [20].

2.2. Peptaibols

Peptaibols are the linear peptides consisting of α,α-dialkylated amino acids, isovaline, α-amino isobutyric acid (Aib), an acetylated N-terminus, and a C-terminal amino alcohol. They are ecologically and commercially important for their antimicrobial and anti-cancer properties, as well as their ability to induce systemic resistance in plants against microbial invasion. The peptaibols are amphipathic in nature and self-assemble to form voltage-dependent ion channels in membranes. This ability is largely responsible for the antibiotic properties of these compounds [28,29]. Peptaibols are produced largely by members of genus Trichoderma [30], and the first discovered peptaibol, alamethicin F30 (Figure 2; 3), was reported from T. viride [31,32]. Peptaibol subclasses were defined on the basis of peptide chain length. Those peptaibols having 18–20 residue peptides in their chain length are called long-sequence peptaibols [33,34,35,36,37], those having 11–16 residue peptides in their chain length are termed short-sequence peptaibols [38], while peptaibols having only 7–11 residue peptides in their chain length, with N-terminal amino acids acylated by a short lipid chain, are termed lipopeptaibols [39]. Three peptaibols, trichokonins VI (Figure 2; 4), VII (Figure 2; 5), and VIII (Figure 2; 6), obtained from Trichoderma koningii, showed broad-spectrum antimicrobial activity against a range of important plant pathogens, such as R. solani, Fusarium oxysporum, Verticillium dahliae, and Botrytis cinerea. Trichokonins are insensitive to proteolytic enzymes and showed biological activity over a wide pH range even after autoclaving [40]. Trichokonin VI (Figure 2; 4), isolated from Trichoderma pseudokoningii, induced extensive apoptotic programmed cell death in Ascochyta citrullina, B. cinerea, F. oxysporum, Phytophthora parasitica, and V. dahliae [41]. Interestingly, trichokonins were also proved to be highly active against Clavibacter spp., which infects a variety of economically important crops, including potato, maize, and tomato [42]. The peptaibols trichorzianine A1 (Figure 2; 7) and B1 (Figure 2; 8) from Trichoderma harzianum could inhibit the spore germination, as well as hyphal elongation, of plant pathogenic fungi [43,44], and there was a synergistic interaction between hydrolytic enzymes and peptaibols [45]. The antiviral properties of the peptaivirins A (Figure 2; 9) and B (Figure 2; 10) belonging to the peptaibol group has also been reported against tobacco mosaic virus infection in tobacco plants [46]. Peptaibols induce plant defense reactions through the salicylate signal pathway, leading to systemic acquired resistance, which is an interesting feature [47,48,49]. The potential of the peptaibols of Trichoderma qualifies their exploitation as important plant protectants. There are two peptaibol synthetases (of 18 and 14 modules) in Trichoderma genomes. Even though there are more than 700 described peptaibol sequences [50], no genetic studies on their synthesis have been conducted, except in T. virens Gv29-8. Using gene disruptions, the 18-residue peptaibol synthetase Tex1 has been shown to be responsible for the production of the trichovirin II-type 18-residue peptaibol, while the 14-module enzyme assembles both the 14-residue and the 11-residue peptaibol in T. virens [28,51,52].

2.3. Pyrones

The pyrone 6-pentyl-2H-pyran-2-one (6-PP) (Figure 3; 11) is a flavoring agent responsible for the aroma of coconut and has been reported to have antifungal and plant growth-promoting activities [53]. It belongs to the chemically diverse group of low molecular weight metabolites having a high vapor pressure at room temperature and low water solubility, which are classified as volatile organic compounds (VOCs) [54]. Pyrone 6-PP was first discovered in a culture broth of T. viride [55], after which it was also reported to be produced by T. koningii and T. harzianum [56,57]. It caused 31.7% and 69.6% growth reduction in F. oxysporum and R. solani, respectively, at a concentration of 0.3 mg/ml. A positive antifungal correlation had been investigated between pyrone 6-PP production and the antagonistic ability of T. harzianum [58,59]. In stored kiwi fruits, the application of pyrone 6-PP at 0.4 to 4 mg /mL could significantly reduce B. cinerea rots on both naturally infected and artificially inoculated fruits [60]. In addition, 6-PP was also found in T. harzianum T77 and SQR-T037, which were used for the control of grapevine trunk diseases [61] and Fusarium wilt in cucumber in continuously cropped soil [62]. T. harzianum was found to produce three bioactive analogues of pyrone 6-PP (Figure 3; 12–15). The analogue (12) was active against Candida albicans, Penicillium spp., Cryptococcus neoformans, and A. fumigatus [56,63]. In another study, analogue (12), isolated from T. harzianum and T. longibrachiatum, exhibited antifungal activity against Armillaria mellea [64]. The analogue hydro-derivatives massoilactone (13) and d-decanolactone (14) were reported to have activity against Phytophtora and Botrytis species [65]. Another analogue of pyrone, viridepyronone (15), was produced by a strain of T. viride and showed 90% growth inhibition of S. rolfsii at a minimum inhibitory concentration (MIC) of 196 mg/ml [66]. Pyrone 6–PP and its analogues are derived from fatty acids, and their biosynthesis in T. atroviride IMI206040 has been studied by using [1-14C] and [U-14C] linoleic acid. It was suggested that the oxidization of linoleic acid to 13-hydroperoxide-diene, followed by 5-hydroxy-2,4-decenioc acid formation and finally esterification, resulted in the formation of pyrones [67].

2.4. Butenolides

An antifungal butenolide compound, harzianolide (Figure 4; 16), was isolated from three strains of T. harzianum [68,69,70]. The dehydro-derivative (17) of harzianolide (16) was obtained from T. harzianum. Another butanolide, T39butenolide (18), was produced by a commercially available T. harzianum strain [71]. All of these compounds (16–18) showed antifungal activity against Gaeumannomyces graminis var. tritici [68,71]. Harzianolide (16) particularly inhibited the growth G. graminis var. tritici at 200 mg/mL, while T39butenolide (18) inhibited the growth of G. graminis at 100 mg/mL. Additionally, harzianolide (16) and T39butenolide (18) caused growth inhibition in P. ultimum and R. solani [71]. From the fungus T. longibrachiatum Rifai aggr, 5-Hydroxyvertinolide (19) was isolated, which was antagonistic to the fungus Mycena citricolor, the agent responsible for American leaf spot disease of coffee [72]. In another study, the antifungal effect of a compound of harzianolide (16) and T39butenolide (18) was reported against P. ultimum, R. solani, and B. cinerea [73]. The biosynthesis of these butenolides probably involves two Favorskii rearrangements from a C-14-diepoxide, resulting in the extrusion of the two carbons that form the lactone [74].

2.5. Pyridones

Antifungal harzianopyridone (Figure 5; 20) was first isolated from T. harzianum in 1989. It contains a pyridine ring system with a 2,3-dimethoxy-4-pyridinol pattern [75]. The racemic form of harzianopyridone (20) showed strong antifungal activity against plant pathogenic fungi, such as P. ultimum, G. graminis var. tritici [71], R. solani, and B. cinerea [75]. A laevorotatory form of harzianopyridone (20) isolated from T. harzianum exhibited weak antibacterial and antifungal activity and also showed high phytotoxicity in an etiolated wheat coleoptile bioassay analysis. The harzianopyridone (20) was also reported to cause necrosis in corn, bean, and tobacco in a concentration-dependent manner, which suggested that the two harzianopyridone (20) enantiomers may exhibit different activities [74]. In another investigation, harzianopyridone (20) isolated from T. harzianum showed activity against Phytophthora cinnamomi, B. cinerea, and Leptosphaeria maculans [73]. This compound was also reported to inhibit more than 90% of the growth of R. solani, F. oxysporum, and S. rolfsii [76]. The pyridone harzianopyridone (20) was proposed to be biosynthesized from a tetraketide with the possible involvement of aspartic acid [74,75].

2.6. Azaphilones

The azaphilones contain a chiral quaternary center and extremely high oxygenated bicyclic core, and hence form a structurally diverse group of SMs. Two azaphilone-type compounds, harziphilone (Figure 6; 21) and fleephilone (Figure 6; 22), were reported to be produced by T. harzianum. These were isolated by the bioassay-guided fractionation of the butanol–methanol extract of the fermentation broth of T. harzianum. T. harzianum was also found to produce another azaphilone, T22azaphilone (23). These compounds exhibited significant antifungal activity against P. ultimum, G. graminis var. tritici, and R. solani [71]. T22azaphilone (23) also exhibited antifungal activity against B. cinerea, P. cinnamomi, and L. maculans at low doses [73]. Gene deletions and biochemical investigations demonstrated that azaphilones were collaboratively synthesized by two separate clusters containing four core enzymes, two nonreducing PKSs, one highly reducing PKS, and one NRPS-like PKS. This is a meaningful mechanism of fungal SMs, which allows fungi to synthesize more complex compounds and gain new physiological functions [77].

2.7. Koninginins

Some species of Trichoderma produced a series of SMs, named koninginins A–E (Figure 7; 24–28) and G (29). Koninginins A (24) and B (25) were identified in the culture broth of a strain of T. koningii obtained from soil and the root of Diffenbachia species [78,79]. Two strains of T. harzianum isolated from wheat roots were also reported to produce koninginins A (24) and B (25) in their liquid cultures [68]. The total synthesis of compounds 24 and 25 allowed for the correction of the relative configurations of koninginins A (24a) and B (25a) [80,81]. Later, in 2002, X-ray analysis was used to confirm this stereochemistry [82]. The koninginins C (26) and D (27) were produced by T. koningii isolated from soil and fermented on a shredded wheat medium [83,84]. The koninginin E (28) was isolated from liquid cultures of T. harzianum and T. koningii [85,86] and koninginin G (29) was obtained from Trichoderma aureoviride [87]. The total synthesis of koninginin D (27) and E (28) has been performed [81]. Except for koninginin C (26), all other koninginins are bioactive against different plant fungal pathogens. For example, koninginins A, B, D, E, and G (24, 25, 27, 28, 29) exhibit activity against G. graminis var. tritici [68,85], while koninginin D (27) was reported to have antifungal activity against several plant pathogenic fungi, such as F. oxysporum, Bipolaris sorokiniana, P. cinnamomi, and Pythium middletonii [84]. In another study, koninginins A, B, and D (24, 25 and 27), obtained from Trichoderma koningiopsis YIM PH30002, exhibited antifungal activity against F. oxysporum, Fusarium solani, and Alternaria panax [88]. Koninginins belong to the secondary metabolite group of polyketides. Generally, the polyketide synthases catalyze the polyketide biosynthesis reaction, which is carried out by the repeated attachment of short chain fatty acids, i.e. propionate and acetate, by similar pathways exhibited by fatty acid biosynthesis [89].

2.8. Steroids

Stigmasterol (Figure 8; 30) was obtained from T. harzianum and T. koningii that showed antifungal activities against R. solani, S. rolfsii, M. phaseolina, and F. oxysporum [76,90]. Two other steroids, ergosterol (31) and 3,5,9-trihydroxyergosta-7,22-dien-6-one (32), isolated from Trichoderma sp. YM 311505, exhibited strong antifungal activities against Pyricularia oryzae, C. albicans, Aspergillus niger, and Alternaria alternata with an MIC value of 32 µg/mL [91].

2.9. Anthraquinones

Three anthraquinones, 1,8-dihydroxy-3-methylanthraquinone (Figure 9; 33), 1-hydroxy-3-methylanthraquinone (34), and 6-methyl-1,3,8-trihydroxyanthraquinone (35), were isolated from T. harzianum strains that were active against R. solani, S. rolfsii, M. phaseolina, and F. oxysporum [76]. Compounds 33 and 34 also showed antifungal activity against G. graminis var. tritici and P. ultimum [71]. It was reported that the low oxidation state of 6-methyl-1,3,8-trihydroxyanthraquinone (35) had the potential to change to a high oxidation state by the host reactive oxygen species that were released in response to attack by microbial pathogens, which means compound 35 may have the ability to increase the efficiency of Trichoderma against host resistance to other pathogens [92].

2.10. Lactones

The antifungal 10-member lactone cremenolide (Figure 10; 36) was isolated from T. cremeum. Along with the promotion of tomato seedling growth, this compound (36) also showed antifungal activities against R. solani, B. cinerea, and F. oxysporum [93]. Another lactone, aspinolide C (37), was isolated from T. arundinaceum and showed an antibiotic effect against B. cinerea and Fusarium sporotrichioides. Beside its direct antibiotic effect, compound (37) also played an important role in the induction of plant resistance against phytopathogenic fungi. [94]. Cerinolactone (38) was isolated from culture filtrates of T. cerinum [95] and showed strong activity against Rosellinia necatrix [96].

2.11. Trichothecenes

Trichothecenes are the sesquiterpenoid-derived SMs mainly produced by Fusarium and other fungal genera, like Trichoderma, Trichothecium, and Stachybotrys [97,98]. The chemical structure of trichothecenes comprises a trichothecene ring, which contains an olefinic ring at C-9,10, and an epoxide group of C-12 [97]. Trichothecenes inhibit protein synthesis by preventing peptide bond formation at the peptidyl transferase center of the 60S ribosomal subunit [99,100]. Trichodermin (Figure 11; 39) was the most widely studied antifungal compound [99,100]. It was first obtained from T. brevicompactum and displayed significant inhibitory activity on R. solani, B. cinerea, and Colletotrichum lindemuthianum (EC50 = 25.60 g/mL) [97]. It was also isolated from T. harzianum and showed activities against several phytopathogenic fungi, such as Cochliobolus miyabeanus, R. solani, C. lindemuthianum, F. oxysporum, Thanatephorus cucumeris, Colletotrichum gloeosporioides, and B. cinerea [101,102].

2.12. Others

Other antifungal compounds belonging to different chemical classes isolated from Trichoderma spp. are briefly described here, and their structures are presented in Figure 12. Diterpene harziandione (Figure 12; 40) was isolated from T. harzianum [103] and T. viride and showed antifungal activity against S. rolfsii [104]. Three antifungal compounds, 10,11-dihydrocyclonerotriol (41), catenioblin C (42), and sohirnone A (43), were obtained from T. longibrachiatum and have been shown to have antifungal activities against C. albicans and P. oryzae [105]. Harzianic acid (44), a tetramic acid produced by the T. harzianum M10 strain, demonstrated remarkable biological properties, including plant growth promotion and antimicrobial activity against different plant pathogenic fungi, such as Pythium irregulare, Sclerotinia sclerotiorum, and R. solani [106]. The cyclopentenoneacrylic acid derivative trichodermester A (45) was isolated from a marine-derived T. atroviride and showed activity against Phaeosphaerella theae with an MIC of 125 µg/disc [107].

3. Antifungal Mechanisms of Trichoderma SMs

The success of Trichoderma spp. for their antifungal activities against phytopathogenic fungi could be attributed to the combined action of SMs and hydrolytic enzymes [108]. The inhibition of B. cinerea spore germination has been shown to be due to the synergetic effect of gliotoxin (Figure 1; 1) and endochitinase enzymes [109], while gliP-deleted mutants of T. virens, which are unable to produce gliotoxin, reduced their mycoparasitism against the soybean pathogen S. sclerotiorum and oomycete pathogen P. ultimum [27]. Similar to other plant beneficial microorganisms, Trichoderma fungi release elicitor-like substances which induce a systemic or localized resistance response in plants [5].
Various SMs produced by Trichoderma spp., such as harzianolides, peptaibols, and certain volatile compounds, are reported to have antifungal potential, as well as acting as a plant growth promoter, resulting in increased plant resistance to pathogen attack. For example, 6-PP (Figure 3; 11), along with reducing the mycelial growth of F. oxysporum, B. cinerea, and R. solani, also promotes plant growth and induces systemic resistance, probably by acting as an auxin-like compound [53]. Recently, it has been shown that tomato plants treated with 6-PP produced significantly more γ-aminobutyric acid and acetylcholine, which helps the plants to resist pathogens [110]. The antifungal activities of peptaibols are due to their ability to form ion channels in membranes and inhibit the enzymes responsible for the synthesis of cell walls [111,112,113]. Trichokonin VI (Figure 2; 4), a peptaibol derived from T. pseudokoningii, showed antifungal activity by inducing extensive apoptotic programmed cell death [41,114]. In addition, peptaibols also trigger plant defense responses. The Dtex1-deleted mutants of T. virens, which were unable to produce 18-residue peptaibol, failed to trigger systemic resistance responses in cucumber [28]. Meanwhile, the application of the 20-residue peptaibol alamethicin F30 (Figure 2; 3) from T. viride induced jasmonic acid- and salicylic acid-mediated resistance in lima bean [47].
Another mechanism of SMs for controlling phytopathogenic fungus is their role in the competition for nutrients. The fast-growing ability of Trichoderma spp. makes them potential competitors for nutrients and space. Trichoderma spp. make iron unavailable for the competing microorganisms by releasing siderophores, which scavenge iron from the environment. Iron competition has been shown to play an important role in the antagonistic activity of T. asperellum against F. oxysporum [115]. The coiling ability of Trichoderma around thehyphae of the prey fungus increases its mycoparasitism activity [116]. It is reported that the anthraquinone SMs, emodin and pachybasin, derived from T. harzianum, play a role in the self-regulation of coiling in T. harzianum [117]. The addition of these compounds increased the number of coils of the mycoparasite around R. solani hyphae, and this effect seems to be due to a stimulation of cAMP synthesis. Some SMs interact with the toxins of pathogenic fungi and inhibit their growth. For example, 6-PP (Figure 3; 11) secreted by T. harzianum degrades fusaric acid and mycotoxins and inhibits Fusarium moniliforme mycelial growth [118].

4. Approaches for the Analysis of SMs in Trichoderma spp.

For SMs, there is not a one-to-one relationship between a metabolite and a gene. The secondary metabolome, however, in many cases is a result of many genes and their enzymes [119]. The fungal sequencing of fungal genomes disclosed the fact that gene clusters associated with SMs exceed the number of SMs from a given fungus and several gene clusters from the prediction remain silent [120]. Different molecular, as well as cultivation-based, approaches involved in the regulation of these silent gene clusters can be utilized for their activation [121,122]. Metabolomics, along with the efforts for the activation of silent gene clusters, can contribute to the development and identification of new SMs (Figure 13). Metabolomics includes the untargeted, as well as targeted, approaches for determining the identity of all low molecular weight SMs of an organism. Untargeted approaches are the methods and techniques for the searching of all known and unknown detectable compounds, while targeted approaches are for the identification of already known compounds. Different chromatographic techniques, such as gas and liquid chromatography, along with mass spectrometry, are useful for the analysis of metabolites in complex samples. These techniques are helpful to detect a large number of metabolites. The applications of liquid chromatography mass spectrometry (LC-MS) allows for the detection of mid- to nonpolar metabolites, while gas chromatography mass spectrometry (GC-MS) is suitable for the study of both volatile and polar small substances [123]. Liquid chromatography, when combined with tandem mass spectrometry (LC-MS/MS), is useful for peptaibiotic detection in the samples extracted from fungal cultures, whereby the specific amino acid, Aib, for peptaibiotics can be indicated by mass differences of D m/z 85 [30]. The known structures of peptaibiotics can be obtained by comparing the amino acid sequences obtained from LC-MS/MS analysis with their respective databases, such as the “Comprehensive Peptaibiotics Database” [124]. The matrix-assisted laser desorption/ionization time of flight mass spectrometry (MALDI-TOF-MS) is an advanced approach, which is much faster and more effective than the traditional bioactive screening techniques, to discover new bioactive SMs in fungus. This technique was used for the detection of peptaibol production profiles from 28 different Trichoderma species [125]. Imaging mass spectrometry (IMS) is another advancement that allows the direct analysis of fungi for SMs. In association with MALDI and coupled to a mass spectrometer, IMS produces images depicting the spatial distribution of natural products [126,127,128,129]. MALDI-IMS has been used for the metabolic analysis of living bacterial communities and interkingdom interactions between fungi and bacteria directly from their cultures [130,131,132]. Recently, MALDI-IMS was used to visualize the SMs in the mycoparasitic interaction of R. solani and T. atroviride [133]. Little, or even no, sample preparation requirements make the MALDI techniques well suited to the analysis of co-cultivations [134].

5. Biosynthesis Pathway and Factors Affecting the Regulation of SMs in Trichoderma spp.

SMs are usually synthesized from a few precursors produced by primary metabolism, which act as raw material for the production of SMs. These precursors are then transformed to first stable intermediates through the action of different core enzymes. Based on the core enzyme involved in the biosynthesis of intermediates, they can be divided into different groups, such as dimethylallyl tryptophan synthases, polyketide synthases (PKSs), terpene cyclases, non-ribosomal peptide synthetases (NRPSs), and hybrid PKS-NRPS enzymes, and are involved in the production of indole alkaloids, polyketides, terpenes, non-ribosomal peptides, and PKS-NRPS hybrids, respectively [135]. The further modification of the first stable intermediates is generally accomplished by decorating or tailoring enzymes, resulting in the formation of a final active product or compound [135]. In addition to these core enzymes, the gene cluster of SMs may also contain other genes that encode transcription factors for the regulation of gene expression involved in biosynthesis and transporters that contribute to self-protection or SM efflux [135,136,137,138]. The evolutionary force responsible for the maintenance and formation of SM genes in physical clustering is unclear [139]. However, the physically linked genes in a cluster exhibit the ability of better co-regulation, which allows a strong coordinated connection among the enzymes involved in the same biosynthesis pathway [140,141,142]. Here, a brief introduction on the SM biosynthetic scheme and their regulation factors in Trichoderma fungi is presented (Figure 14).
Recent studies related to regulatory factors and the influence of environmental conditions on fungal SMs enhanced our understanding on the tightly regulated cellular process of SMs. Like other fungi, in Trichoderma spp., different factors, such as pH signaling, velvet-complex proteins, and interactions with other organisms, are responsible for the expression of genes related to SMs [143,144,145,146,147,148,149]. The transcriptomic responses of T. virens, T. reesei, and T. atroviride to the presence of R. solani were evaluated, and two PKSs were found among the genes induced in T. reesei–R. solani and T. atroviride–R. solani interactions, whereas all the genes in the biosynthesis cluster of gliotoxin were up-regulated [143]. An up-regulation of the lipoxygenase gene, that is involved in the biosynthesis of 6-PP, was also noticed in T. atroviride [150]. In another study, the co-culture of T. arundinaceum and B. cinerea revealed an increase in the expression of tri biosynthetic genes [147]. However, in the interaction zone between T. arundinaceum and B. cinerea, a secondary metabolite of B. cinerea, which is also a virulence factor of B. cinerea, reduced tri gene expression and harzianum A production in T. arundinaceum [147].
It was reported that the presence of the Fusarium mycotoxin fusaric acid resulted in the suppression of 6-PP (Figure 3; 11) production and the induction of sporulation-associated metabolite i.e., 1-octen-3-ol, production [151]. In return, certain Trichoderma strains, due to the secretion of 6-PP, are capable of inhibiting fatty acid production by F. moniliforme and degrading fatty acids [118]. In Trichoderma genomes, gene clusters related to the production of SMs harbor specific transcription factors. In addition to these regulators present in gene clusters, several other key players also take part in the regulation of SM biosynthesis, such as PacC, a pH regulator which influences different fungal genes in response to environmental pH [149,152]. The PacC orthologue of T. virens controls the iron transport and biosynthesis of SMs. In DpacC mutants of T. virens, the gene expression was altered for cytochrome P450, NRPS Tex15, and siderophore-related biosynthesis enzymes [153]. Moreover, biocontrol activity was reduced in T. virens DpacC mutants, which may be because of their inability to adapt to alkaline pH.
The production of SMs is also under the regulation of the heterotrimeric velvet complex. This complex consists of two velvet proteins, VelA and VelB, and methyltransferase LaeA [154]. The velA orthologue vel1 governs the regulation of gene clusters related to the production of SMs. The disruption of the vel1 gene stopped the biosynthesis of gliotoxin and silenced several SM-related genes that encode for one cytochrome P450 monooxygenase, two PKSs, NRPSs, and one O-methyl transferase [148]. A similar role was noticed for the T. reesei LaeA orthologue that influenced the expression of lignocellulose-degrading enzymes [146,155]. The T. atroviride removal of lae1 resulted in abolishing the antifungal activity of T. atroviride. This correlated with a significantly reduced expression in 6-PP-related lipoxygenase genes and PKS-encoding genes. The influence of lae1 on the production of 6-PP was also corroborated when, in antagonism experiments, the enhanced production of 6-PP was noticed in lae1 over-expressing strains [146]. The biosynthesis of 6-PP in T. harzianum is also associated with Thctf1. The deletion of the transcription factor Thctf1 altered the antimicrobial activity of T. harzianum and abolished the production of two SMs derived from 6-PP [156].
The transfer and sensing of environmental cues affecting the regulation of fungal SMs was achieved by membrane bound receptors, such as G protein-coupled receptors (GPCRs), and their associated intracellular signaling pathways. The T. atroviride biosynthesis of SMs was governed by G protein signaling and the associated cAMP pathway [157,158,159]. The decrease in 6-PP and increase in peptaibol production was reported with the deletion of tga1, which encodes an adenylyl cyclase-inhibiting Ga subunit of T. atroviride [158]. The biosynthesis of peptaibol was further dependent on two regulators, BLR1 and BLR2, under certain conditions [160].

6. Conclusions

Fungi, being a most diverse group of phytopathogens, exert a huge impact on agriculture. High genetic flexibility and broad-spectrum lifecycles allow the pathogenic fungi to develop fungicide resistance and invade new hosts. Therefore, new management strategies are needed for fighting against pathogenic fungi. The utilization of SMs from Trichoderma spp. has been used in plant protection as an environmentally friendly and efficient management tool against a variety of phytopathogens. This review presented the fungicidal SMs from Trichoderma spp. against phytopathogenic fungi. Some aspects of the structural overview of SMs and their biosynthesis were reviewed. Brief information on the biosynthesis pathway, action mechanism, different approaches for the analysis of SMs, and factors affecting the regulation of SMs in Trichoderma was also discussed.

Author Contributions

R.A.A.K. and S.H. conducted the review of the literature and extracted data. R.A.A.K. and S.N. analyzed data, discussed data, and drafted the first versions of the manuscript. B.X. and Y.L. contributed to data interpretation and revised the manuscript. All authors read and approved the final manuscript.

Funding

This work was supported by grants from the Central Public-interest Scientific Institution Basal Research Fund IVF-BRF2019012 and National Key R&D Program of China 2018YFD0201200.

Conflicts of Interest

The authors declare that they have no conflict of interest.

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Figure 1. Structures of diketopiperazines from Trichoderma spp.: [1] gliotoxin isolated from Trichoderma lignorum, [2] gliovirin isolated from T. virens, [2a, 2b] analogues of gliovirin isolated from T. longibrachiatum.
Figure 1. Structures of diketopiperazines from Trichoderma spp.: [1] gliotoxin isolated from Trichoderma lignorum, [2] gliovirin isolated from T. virens, [2a, 2b] analogues of gliovirin isolated from T. longibrachiatum.
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Figure 2. Structures of antifungal peptaibols from Trichoderma spp.: [3] alamethicin F30, [4] trichokonin VI, [5] trichokonin VII, [6] trichokonin VIII, [7] trichorzianine A1, [8] trichorzianine B1, [9] peptaivirin A, [10] peptaivirin B; peptaibols [4], [5], and [6] were isolated from T. koningii, [7], [8], [9], and [10] were isolated from T. harzianum.
Figure 2. Structures of antifungal peptaibols from Trichoderma spp.: [3] alamethicin F30, [4] trichokonin VI, [5] trichokonin VII, [6] trichokonin VIII, [7] trichorzianine A1, [8] trichorzianine B1, [9] peptaivirin A, [10] peptaivirin B; peptaibols [4], [5], and [6] were isolated from T. koningii, [7], [8], [9], and [10] were isolated from T. harzianum.
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Figure 3. Structures of antifungal pyrones from Trichoderma spp.: [11] 6-PP isolated from T. viride; [12], [13], [14], and [15] analogues of 6-PP isolated from T. harzianum.
Figure 3. Structures of antifungal pyrones from Trichoderma spp.: [11] 6-PP isolated from T. viride; [12], [13], [14], and [15] analogues of 6-PP isolated from T. harzianum.
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Figure 4. Structures of antifungal butenolides from Trichoderma spp. [16]: harzianolide, [17] dehydro-derivative of harzianolide, [18] T39butenolide, [19] 5-hydroxyvertinolide butenolides; [16], [17], and [18] were isolated from T. harzianum and [19] was isolated from T. longibrachiatum.
Figure 4. Structures of antifungal butenolides from Trichoderma spp. [16]: harzianolide, [17] dehydro-derivative of harzianolide, [18] T39butenolide, [19] 5-hydroxyvertinolide butenolides; [16], [17], and [18] were isolated from T. harzianum and [19] was isolated from T. longibrachiatum.
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Figure 5. Structure of antifungal pyridone [20] harzianopyridone from T. harzianum.
Figure 5. Structure of antifungal pyridone [20] harzianopyridone from T. harzianum.
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Figure 6. Structures of antifungal azaphilones isolated from T. harzianum: [21] harziphilone, [22] fleephilone, [23] T22azaphilone.
Figure 6. Structures of antifungal azaphilones isolated from T. harzianum: [21] harziphilone, [22] fleephilone, [23] T22azaphilone.
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Figure 7. Structures of antifungal koninginins from Trichoderma spp.: [24] koninginin A, [25] koninginin B, [26] koninginin C, [27] koninginin D, [28] koninginin E, [29] koninginin G; koninginins [A], [B], [C], [D], and [E] were produced by T. koningii and koninginin [E] was produced by T. aureoviride.
Figure 7. Structures of antifungal koninginins from Trichoderma spp.: [24] koninginin A, [25] koninginin B, [26] koninginin C, [27] koninginin D, [28] koninginin E, [29] koninginin G; koninginins [A], [B], [C], [D], and [E] were produced by T. koningii and koninginin [E] was produced by T. aureoviride.
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Figure 8. Structures of antifungal steroids from Trichoderma spp.: [30] stigmasterol, [31] ergosterol, [32] 3,5,9-trihydroxyergosta-7,22-dien-6-one.
Figure 8. Structures of antifungal steroids from Trichoderma spp.: [30] stigmasterol, [31] ergosterol, [32] 3,5,9-trihydroxyergosta-7,22-dien-6-one.
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Figure 9. Structures of antifungal anthraquinones from Trichoderma spp.: [33] 1,8-dihydroxy-3-methylanthraquinone, [34] 1-hydroxy-3-methylanthraquinone, [35] 6-methyl-1,3,8-trihydroxyanthraquinone.
Figure 9. Structures of antifungal anthraquinones from Trichoderma spp.: [33] 1,8-dihydroxy-3-methylanthraquinone, [34] 1-hydroxy-3-methylanthraquinone, [35] 6-methyl-1,3,8-trihydroxyanthraquinone.
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Figure 10. Structures of antifungal lactones from Trichoderma spp.: [36] cremenolide, [37] aspinolide C, [38] cerinolactone.
Figure 10. Structures of antifungal lactones from Trichoderma spp.: [36] cremenolide, [37] aspinolide C, [38] cerinolactone.
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Figure 11. Structure of antifungal trichothecene: [39] trichodermin from Trichoderma spp.
Figure 11. Structure of antifungal trichothecene: [39] trichodermin from Trichoderma spp.
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Figure 12. Structures of other antifungal compounds from Trichoderma spp.: [40] harziandione, [41] 10,11-dihydrocyclonerotriol, [42] catenioblin C, [43] sohirnone A, [44] harzianic acid, [45] trichodermester A.
Figure 12. Structures of other antifungal compounds from Trichoderma spp.: [40] harziandione, [41] 10,11-dihydrocyclonerotriol, [42] catenioblin C, [43] sohirnone A, [44] harzianic acid, [45] trichodermester A.
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Figure 13. Schematic presentation of approaches for the analysis of SMs in Trichoderma spp.
Figure 13. Schematic presentation of approaches for the analysis of SMs in Trichoderma spp.
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Figure 14. Proposed biosynthetic scheme and the regulation factors of SMs in Trichoderma spp.
Figure 14. Proposed biosynthetic scheme and the regulation factors of SMs in Trichoderma spp.
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MDPI and ACS Style

Khan, R.A.A.; Najeeb, S.; Hussain, S.; Xie, B.; Li, Y. Bioactive Secondary Metabolites from Trichoderma spp. against Phytopathogenic Fungi. Microorganisms 2020, 8, 817. https://doi.org/10.3390/microorganisms8060817

AMA Style

Khan RAA, Najeeb S, Hussain S, Xie B, Li Y. Bioactive Secondary Metabolites from Trichoderma spp. against Phytopathogenic Fungi. Microorganisms. 2020; 8(6):817. https://doi.org/10.3390/microorganisms8060817

Chicago/Turabian Style

Khan, Raja Asad Ali, Saba Najeeb, Shaukat Hussain, Bingyan Xie, and Yan Li. 2020. "Bioactive Secondary Metabolites from Trichoderma spp. against Phytopathogenic Fungi" Microorganisms 8, no. 6: 817. https://doi.org/10.3390/microorganisms8060817

APA Style

Khan, R. A. A., Najeeb, S., Hussain, S., Xie, B., & Li, Y. (2020). Bioactive Secondary Metabolites from Trichoderma spp. against Phytopathogenic Fungi. Microorganisms, 8(6), 817. https://doi.org/10.3390/microorganisms8060817

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