Arbuscular Mycorrhizal Fungi for the Biocontrol of Plant-Parasitic Nematodes: A Review of the Mechanisms Involved
- 1Laboratory of Tropical Crop Improvement, Department of Biosystems, KU Leuven, Heverlee, Belgium
- 2Unit for Environmental Sciences and Management, North-West University, Potchefstroom, South Africa
- 3Bioversity International, Heverlee, Belgium
- 4Centre of Microbial and Plant Genetics, KU Leuven, Heverlee, Belgium
- 5Department of Plant Systems Biology, Vlaams Instituut voor Biotechnologie, Gent, Belgium
- 6Commonwealth Scientific and Industrial Research Organisation Agriculture, Queensland Bioscience Precinct, Brisbane, QLD, Australia
Arbuscular mycorrhizal fungi (AMF) are obligate root symbionts that can protect their host plant against biotic stress factors such as plant-parasitic nematode (PPN) infection. PPN consist of a wide range of species with different life styles that can cause major damage in many important crops worldwide. Various mechanisms have been proposed to play a role in the biocontrol effect of AMF against PPN. This review presents an overview of the different mechanisms that have been proposed, and discusses into more detail the plausibility of their involvement in the biocontrol against PPN specifically. The proposed mechanisms include enhanced plant tolerance, direct competition for nutrients and space, induced systemic resistance (ISR) and altered rhizosphere interactions. Recent studies have emphasized the importance of ISR in biocontrol and are increasingly placing rhizosphere effects on the foreground as well, both of which will be the focal point of this review. Though AMF are not yet widely used in conventional agriculture, recent data help to develop a better insight into the modes of action, which will eventually lead toward future field applications of AMF against PPN. The scientific community has entered an exciting era that provides the tools to actually unravel the underlying molecular mechanisms, making this a timely opportunity for a review of our current knowledge and the challenges ahead.
Nematodes form a highly diverse group comprising free-living nematodes as well as plant and animal parasites that can be found worldwide in various habitats (Ferraz and Brown, 2002). Many species of plant-parasitic nematodes (PPN) can act as pests on a wide range of important agricultural crops. They mostly live in the soil, but some species such as several Ditylenchus spp. can act as aboveground pests. PPN show a wide array of life styles, but all have a usually hollow, retractable, needle-like mouth spear called the stylet for feeding. They are classified into different groups based on their feeding strategy (Perry and Moens, 2011). Ectoparasitic nematodes remain in the rhizosphere during feeding, using their stylet to acquire food from the epidermal or outer root cortex cells. Endoparasitic nematodes on the other hand completely enter the root and feed inside the root. Migratory endoparasitic nematodes (e.g., Radopholus spp. and Pratylenchus spp.) migrate inter-or intracellularly while feeding on root cortex cells, thus causing damage to the plant along their migration path (Jones et al., 2013). Endoparasitic sedentary nematodes display the most complex feeding strategy of PPN, selecting cells in the vascular cylinder to be converted into a feeding site and then becoming sedentary with the onset of feeding (Gheysen and Mitchum, 2011). This last group includes the cyst and root-knot nematodes, which are considered to be the most damaging pests of agricultural crops worldwide (Jones et al., 2013; Bartlem et al., 2014). The sedentary endoparasitic Meloidogyne spp. such as M. incognita and M. javanica, can result in complete crop losses in tobacco and tomato or sunflower and pepper, respectively (Wesemael et al., 2011). The direct damage caused by PPN can be aggravated by secondary infections of the wounded plant tissues by other pathogens, while some PPN, such as the migratory ectoparasitic Xiphinema spp., can transmit plant viruses (Hao et al., 2012). Yield losses caused by PPN are expected to rise in the near future as a result of climate change and cropping systems intensification (Nicol et al., 2011). The use of nematicides is being limited, given the increasing concern for human health as well as the environment, which has led to their ban. Alternative nematicides are being sought (Oka and Mizukubo, 2009; Wesemael et al., 2011). Scientists are also looking for other nematode management strategies that fit into the recently launched framework of the Integrated Pest Management (IPM) directive of the European Union (EU directive 2009/128/EC), stating that member states have to implement IPM from 2014 onward, with the aim to reduce pesticide use and to promote non-chemical management practices as much as possible. One of the proposed environmentally friendly options to manage PPN is the use of biological control organisms, such as arbuscular mycorrhizal fungi (AMF).
Arbuscular mycorrhizal fungi are obligate root symbionts, estimated to colonize more than 80% of all land plant species. They improve plant growth through increased nutrient uptake in exchange for photosynthetic carbon from their host (Smith et al., 2010). Also, they can alleviate plant stress caused by abiotic as well as biotic factors, including PPN (Gianinazzi et al., 2010; Singh et al., 2011; Vos et al., 2012a). The biocontrol effect of AMF has been observed in a wide range of plant species and against many pathogens, most of them soil-borne fungal pathogens causing root rot or wilting, though successful biocontrol has also been observed against aboveground pathogens such as Alternaria solani in tomato (Harrier and Watson, 2004; Whipps, 2004; Fritz et al., 2006; Pozo and Azcón-Aguilar, 2007; Jung et al., 2012). Both necrotrophic and biotrophic pathogens have been reported to be suppressed by AMF, either directly or indirectly (Veresoglou and Rillig, 2012). AMF can also suppress PPN, as has been previously reviewed by Pinochet et al. (1996) and Hol and Cook (2005). In vitro, greenhouse as well as field experiments indicated protective effects against PPN by AMF in plants such as banana, coffee and tomato (Calvet et al., 2001; Vos et al., 2012b; Alban et al., 2013; Koffi et al., 2013). These protective effects ranged from a reduction in infection and reproduction to an enhanced tolerance. But though there are many reports on the biocontrol effect of AMF, their actual use as biological control agents in the field is still not a routine agricultural practice (Salvioli and Bonfante, 2013). This is partially due to variability in performance, depending on the AMF isolate, pathogen, plant species and environmental conditions (Dong and Zhang, 2006; Veresoglou and Rillig, 2012; Salvioli and Bonfante, 2013). An increased insight into their modes of action will therefore help to increase the efficacy of these biocontrol agents.
Several mechanisms can be involved in the AMF-mediated biocontrol; direct effects of AMF on the pathogen, involving competition for space or nutrients, or indirect, plant-mediated, effects. The latter can further be divided into the effects of AMF on plant tolerance, plant defense induction and altered plant exudation leading to altered rhizosphere interactions (Figure 1). The different mechanisms cannot be considered as completely independent from each other and biocontrol probably results from a combination of different mechanisms (Vierheilig et al., 2008; Cameron et al., 2013). In addition, the relative importance of a specific mechanism can vary depending on the specific AMF-pathogen-plant interaction. In recent years, much progress has been made, especially in the domains of induced systemic resistance (ISR; Pieterse et al., 2014) as well as on the role of the rhizosphere in biological control (Cameron et al., 2013), which will be the focal points of this review. We will present an overview of the different mechanisms that have been proposed to play a role in the AMF-mediated biocontrol, and we will discuss more into detail the possible significance of the different mechanisms for plant infection by PPN.
Figure 1. Overview of the possible mechanisms by which arbuscular mycorrhizal fungi can exert biocontrol against plant-parasitic nematodes. They consist of direct effects of AMF on the pathogen, involving competition for space and nutrients (bottom left) and indirect plant-mediated effects, involving damage compensation and enhanced tolerance (top right). The latter can be further divided into the effects of AMF on plant defense induction (ISR; top left) and altered rhizosphere interactions through changes in plant root exudation (bottom right). The different mechanisms cannot be considered as completely independent from each other and biocontrol probably results from a combination of different mechanisms.
Enhanced Plant Tolerance
Higher Nutrient Uptake
Arbuscular mycorrhizal fungi are known to be able to increase the uptake of water and mineral nutrients for their host plant, such as phosphate and nitrogen (Parniske, 2008; Baum et al., 2015) but probably also micro-elements such as zinc (Smith and Smith, 2011a,b). In return, they receive photosynthetic carbon from their host (Gianinazzi et al., 2010). Similar to the protection of the plant by AMF against various abiotic stress factors such as drought, cold or heavy metal toxicity (Singh et al., 2011), AMF could also compensate for damage caused by pathogens. Although higher uptake of phosphate has been proposed as a mechanism for the AMF-mediated biocontrol, addition of phosphate to non-mycorrhizal plants did not result in a similar reduction of pathogen infection (Bodker et al., 1998). Fritz et al. (2006) showed that tomato plants colonized by Rhizophagus irregularis showed significantly less symptoms caused by A. solani than non-mycorrhizal plants, while no increase in phosphate uptake was observed. An additional phosphate supply even resulted in higher disease incidence. There is thus not always a positive correlation between increased phosphate uptake and plant growth promotion in mycorrhizal plants, as in some cases plant growth suppression resulted as a consequence of AMF colonization, even when phosphate transport from the AMF to the host plant was taking place (Smith and Smith, 2011a).
Plants with a better nutrient status are able to tolerate higher PPN population densities in their roots, as observed in cotton fields infested with the sedentary semi-endoparasitic nematode Rotylenchulus reniformis (Pettigrew et al., 2005). Regression analysis of nematode population densities against the mineral content in rice also revealed a positive correlation between migratory ectoparasitic Helicotylenchus spp. and Mg, however, a negative correlation was observed between the migratory endoparisitic nematode Pratylenchus zeae and Zn or Fe, and between M. incognita and Mg and Ca (Coyne et al., 2004). These observations indicate that the nutrient status of the host plant can affect PPN population densities in both a positive and negative way. But so far, no solid data are available that prove that the AMF-enhanced nutrient status is a causal agent of a higher resistance against PPN.
Altered Root Morphology
Apart from an increased nutrient status, mycorrhizal plants often show increased root growth and branching (Gamalero et al., 2010; Orfanoudakis et al., 2010; Gutjahr and Paszkowski, 2013). The root morphology responses resulting from AMF colonization seem to depend on plant characteristics, with tap roots for example appearing to profit more from AMF than fibrous roots in terms of gained biomass and nutrient acquisition (Yang et al., 2014).
Increased root branching observed in mycorrhizal plants has been suggested to have implications for pathogen infection as well (Vos et al., 2014), although a clear correlation could not been found (Vierheilig et al., 2008). Positive effects could result from an increase in root vigor, due to a higher nutrient uptake capacity. It might even counterbalance the suppressed root growth caused by PPN. For example, decreased root branching caused by the migratory endoparasitic nematodes Radopholus similis and P. coffeae in banana was counterbalanced by the increased branching due to colonization by the AMF Funneliformis mosseae (Elsen et al., 2003a). Increased root branching can, however, also have a negative impact on the host plant by an increase in potential infection sites, depending on the PPN and plant species. Migratory endoparasitic nematodes, such as R. similis, have a preference for primary roots (Stoffelen et al., 2000; Elsen et al., 2003b). For the sedentary endoparasitic root-knot and cyst nematodes, the root elongation zones and sites of lateral root formation are preferred penetration sites, probably because of increased leakage of exudates in these zones (Wyss, 2002; Curtis et al., 2009). However, increased root branching and root length did not alter plant susceptibility to cyst nematodes, as it was observed that the number of penetrating Heterodera schachtii juveniles in transgenic Arabidopsis thaliana plants with long- or short-root phenotypes was similar to that in wild type plants (Hewezi and Baum, 2012).
The possible role of altered root morphology in AMF-mediated biocontrol has been investigated against several other pathogens. In an earlier study, Norman et al. (1996) investigated the consequences of a highly branched root system of strawberry on Phytophthora fragariae infection, a pathogen that mainly infects through the root tips. For non-mycorrhizal root systems infection was indeed higher on the more highly branched roots, but this was not observed in mycorrhizal root systems. Similar findings in different AMF-pathosystems were also reported later (Fusconi et al., 1999; Gange, 2000; Vigo et al., 2000; Gamalero et al., 2010), pointing toward other mechanisms involved in the AMF-mediated biocontrol. Although such experiments have not been performed specifically with PPN, similar mechanisms can be expected to play a role as well.
Direct Competition for Nutrients and Space
Although no antibiotic production or mycoparasitism potential has so far been shown in AMF species, direct effects of AMF on pathogen infection through competition have been proposed. Competition for nutrients or for space and infection sites do occur between micro-organisms with the same physiological requirements in an ecological niche, especially where resources such as carbon might be limited (Vos et al., 2014).
Nutrient competition, with emphasis on competition for carbon, has been suggested as a mechanism of the AMF-mediated biocontrol though not much evidence is found in the literature (Jung et al., 2012). The carbon transfer from the host plant to the AMF is estimated to range from 4 to 20% of the total assimilated carbon (Hammer et al., 2011). It thus seems plausible that AMF compete with pathogens for this resource (Vos et al., 2014). As there is a difference in carbon sink strength between different AMF species, according to the hypothesis of carbon competition it could thus be expected that different AMF species mediate different levels of biocontrol (Lerat et al., 2003). Thus far, however, this hypothesis is not supported by experimental evidence (Vierheilig et al., 2008; Jung et al., 2012). For example, the AMF R. irregularis could not exert a stronger biocontrol effect on R. similis and P. coffeae in banana nor on M. incognita in tomato despite its higher carbon sink strength compared to F. mosseae (Vos, 2012).
Competition for space could also be involved in AMF-PPN interactions since they both reside in roots (Jung et al., 2012). Negative effects due to space constriction can be exerted on PPN as mycorrhizal arbuscules exclusively form in the cortex, where also migratory endoparasitic nematodes feed. Space competition between AMF and sedentary endoparasitic nematodes could be brought into play in case the feeding cells extend into the cortex (Figure 2). Cyst nematode feeding cells, the so-called syncytia, are confined within the endodermis and should therefore be less affected by AMF. Through PCR and DNA sequencing, del Mar Alguacil et al. (2011) reported that galls produced by M. incognita in Prunus persica roots could be colonized by AMF. However, as mycorrhizal arbuscules are short-lived structures (Parniske, 2008; Javot et al., 2011), it is difficult to distinguish whether AMF or PPN colonized the same root part first.
Figure 2. Tomato roots stained with ink-vinegar solution to observe mycorrhizal colonization by Funneliformis mosseae (in blue). This root fragment shows typical mycorrhizal structures such as hyphae (H), arbuscules (A) and vesicules (V), showing the mature stage of the colonization along with the gall induced by Meloidogyne incognita, of which the egg mass (E) is also visible. As such, direct competition for space between arbuscular mycorrhizal fungi and sedentary endoparasitic nematodes probably can take place. Bar size = 100 μm.
Competition for space also implies that a higher AMF colonization degree of the root should lead to a higher level of AMF-mediated biocontrol (Vierheilig et al., 2008). This hypothesis, however, holds only true to a certain degree. A mature AMF colonization, characterized by the presence of arbuscules, seems to be a prerequisite for biocontrol (Khaosaad et al., 2007; Pozo and Azcón-Aguilar, 2007). Dos Anjos et al. (2010) also concluded that when the symbiosis was well established prior to M. incognita inoculation, M. incognita reproduction was reduced, whereas co-inoculation had no effect. However, when co-inoculating native AMF together with Meloidogyne exigua in coffee plants, a biocontrol effect was observed (Alban et al., 2013). The competition for nutrients and space also implies that AMF could be affected by PPN infection as well. Hol and Cook (2005) concluded following a meta-analysis of the available literature that AMF colonization was reduced by ectoparasitic, migratory endoparasitic and sedentary endoparasitic nematodes. In greenhouse experiments, R. similis and P. coffeae in banana affected the frequency of F. mosseae colonization, but not the intensity (Elsen et al., 2003a,b). Contrastingly, root colonization by R. irregularis in in vitro banana plantlets was not affected either by R. similis (Koffi et al., 2013) or by P. coffeae in transformed carrot roots (Elsen et al., 2003c). For sedentary endoparasitic nematodes, Dos Anjos et al. (2010) showed that M. incognita could negatively affect the sporulation of the AMF Scutellospora heterogama in sweet passion fruit, while Alban et al. (2013) found that pre-inoculation of M. exigua led to a significant increase in the subsequent colonization of AMF compared to uninoculated mycorrhizal plants. del Mar Alguacil et al. (2011) also reported that the highest AMF diversity was found in uninfected roots compared to M. incognita infected roots and galls, and that the composition of the AMF community was different between infected and uninfected roots. Their results indicate that AMF colonization might also be suppressed by PPN, depending on the AMF species as some AMF species were not affected by the PPN.
Effects Through Induced Systemic Resistance
In many cases the above mentioned mechanisms are not able to explain the observed AMF-mediated biocontrol, as plant-mediated responses seem also to be involved. For example, using a split-root experimental set-up in tomato in which the root system of one plant was divided over two physically separated compartments with one side pre-inoculated with F. mosseae, Vos et al. (2012b) demonstrated that M. incognita or P. penetrans infection in the other root compartment was significantly reduced. De la Peña et al. (2003), however, did not find a systemic biocontrol effect on P. penetrans in the dunegrass Ammophila arenaria pre-colonized by different native AMF species. However, more reports highlight a systemic suppression of nematode infection in mycorrhizal roots. As, for example, systemic suppression was observed in split root experimental set-ups in R. irregularis-colonized banana against R. similis and P. coffeae (Elsen et al., 2008) but also in grapevine against the ectoparasitic nematode X. index (Hao et al., 2012). A systemic biocontrol effect of AMF has also been shown in interactions with several other pathogens (Cordier et al., 1998; Pozo et al., 2002; Zhu and Yao, 2004; Fritz et al., 2006; Khaosaad et al., 2007; Castellanos-Morales et al., 2011), supporting the importance of this mechanism in the AMF-mediated biocontrol.
Novel insights that are shaping our understanding of the induction of systemic plant defense responses by AMF include the notion that plants initially perceive beneficial organisms as putative pathogens, due to MAMPs (microbe-associated molecular patterns) being conserved between beneficial and pathogenic fungi (Zamioudis and Pieterse, 2012). With AMF being obligate biotrophs, it has indeed been shown that a significant overlap exists in the transcriptional profile of the plant response to AMF and a biotrophic pathogen, such as Magnaporthe grisea (Paszkowski, 2006). Then, upon MAMP-recognition by the plant’s pattern recognition receptors, a MAMP-triggered immunity response (MTI) is activated, forming the first line of defense of the plant in an effort to limit further pathogen invasion (Jones and Dangl, 2006). Surprisingly, the presence of an MTI response in the plant roots has only recently been demonstrated (Millet et al., 2010).
Being initially perceived by the plant as a putative biotrophic pathogen, AMF thus also induce a MTI response, leading to transcriptional and hormonal changes in their host plant upon establishment of the symbiosis. Fiorilli et al. (2011) studied the transcriptome of tomato plants during the colonization process by F. mosseae and observed significant gene modulation in both roots and shoots, with the largest alterations in primary and secondary metabolism, as well as in defense and response to biotic stimuli. López-Ráez et al. (2010) compared the transcriptional response of tomato to two AMF differing in colonization pattern, namely F. mosseae and R. irregularis. Despite the common induction of jasmonate (JA)-biosynthesis and signaling-related genes, they only found 35% overlap in the overall transcriptional profiles of tomato roots colonized by either of these two AMF species. In the case of F. mosseae, a stronger induction of the largely root-specific 9-lipoxygenase (9-LOX) pathway was observed, as well as the induction of the isoleucine conjugate of JA (JA-Ile), several JA-dependent markers and increased salicylic acid (SA) levels, which could be linked to its lower degree of colonization compared to R. irregularis. The early MTI-response involving the jasmonate-linked 9-LOX-pathway could have an early effect on root-knot nematodes as well. In maize, the expression or presence of the 9-LOX gene (ZmLox3) proved to be essential for resistance against M. incognita (Gao et al., 2008). However, so far tripartite studies involving the plant, AMF and PPN have not reported similar results.
Typically, the induction of an MTI response in the early stages of AMF colonization is only weak and transient, so that a further successful establishment of the symbiosis becomes possible. AMF try to avoid their detection by the plant as much as possible, but also actively suppress the MTI response using effectors (Zamioudis and Pieterse, 2012). As a biotroph, AMF colonization is negatively impacted by SA, which is why they are thought to attempt to suppress the SA-mediated defense response in the plant (Hause et al., 2007; Miransari et al., 2014). In addition, it has been proposed that the establishment of the symbiotic program, activated upon perception of mycorrhizal Myc factors, also counteracts the MTI response (Zamioudis and Pieterse, 2012). So far, only one effector molecule has been described for AMF, being the SP7 effector of R. irregularis that interferes with ethylene (ET) signaling in the plant (Kloppholz et al., 2011). This can be associated with recent reports highlighting the role of ET in the MTI response (Millet et al., 2010).
The initial interaction phase between AMF and its host plant primes the plant for a faster and stronger induction of usually JA-dependent defense responses upon subsequent pathogen attack. This cost-effective phenomenon is described as ISR, and specifically in the case of AMF the term mycorrhiza-induced resistance (MIR) has been proposed (Pozo and Azcón-Aguilar, 2007; Pieterse et al., 2014). Exogenous JA-applications and study of mutants altered in the JA-pathway have proven that the JA-dependent pathway is indeed able to mediate resistance to PPN (Soriano et al., 2004; Cooper et al., 2005; Fujimoto et al., 2011; Fan et al., 2015). Traditionally, defense responses to microbes fall into two categories, being termed either ISR or systemic acquired resistance (SAR). SAR is typically SA-dependent and leads to the induction of pathogenesis-related (PR) proteins, while ISR is defined as being regulated by JA and ET, and not accompanied by major changes in PR protein expression (Vlot et al., 2008; Pieterse et al., 2009). Recent research efforts, however, prove that the overlap between SAR and ISR is much larger than originally thought, with substantial crosstalk taking place between the different pathways (Mathys et al., 2012; Pieterse et al., 2014). In this context, the MIR defense response against PPN is probably not solely linked to the JA-dependent pathway.
Some light has been shed on this topic by a few transcriptome studies performed in recent years, involving the tripartite interaction of plants, AMF and nematodes. Li et al. (2006) reported the primed transcriptional activation of a class III chitinase gene in Glomus versiforme colonized grapevine roots upon infection by M. incognita. Constitutive expression of this gene in transgenic tobacco plants enhanced the resistance against the RKN, but did not affect the AMF. This strongly suggests that the class III chitinase gene is involved in a protective mechanism against the PPN. Other recent studies also show that transgenic plants with higher chitinase activity were more resistant to RKN. Though this mostly affected the viability of the eggs which contain chitin, it also reduced the amount of egg masses and thus productivity of the females (Chan et al., 2010, 2015). The primed activation of several other plant defense-related genes was recently also reported in R. irregularis colonized grapevine (Vitis spp.) after infection by the ectoparasitic X. index (Hao et al., 2012). Expression analyses of expressed sequence tags (ESTs) generated by suppression subtractive hybridization (SSH) showed several plant genes that are upregulated during MIR. Interestingly, these genes were only upregulated when AMF and nematode were both present in the root, indicating a priming of these defense genes. The products of these genes include chitinase 1b, but also PR 10, which has RNase and antimicrobial activity. Interestingly, a PR10 protein purified from Crotalaria pallida shows nematostatic and nematicidal effects against M. incognita, targeting a digestive proteinase of the nematode (Andrade et al., 2010). Furthermore, the SSH-study by Hao et al. (2012) showed that glutathione S-transferase was upregulated, which is probably involved in the detoxification of reactive oxygen species (ROS) that can be imposed by the stress of the cell’s hypertrophy and necrosis following nematode infection. Stilbene synthase 1 was also upregulated. It is a key enzyme in the phenylpropanoid pathway toward the phytoalexin resveratrol, of which the accumulation is a typical defense response by grapevine to biotic or abiotic stresses. However, in a previous research, resveratrol was not found to be effective in vitro on R. similis, P. penetrans nor M. incognita (Wuyts et al., 2006). Genes of 5-enolpyruvyl shikimate-3-phosphate synthase (ESPS) and a heat shock protein 70-interacting protein (HIP) were also primed (Hao et al., 2012). ESPS catalyzes the penultimate step in the shikimate pathway. The differential expression of shikimate pathway genes has been reported before in response to root-knot nematode infection of tomato (Schaff et al., 2007) and is thought to be related to the regulation of the auxin balance which is of importance for nematode feeding site formation and possibly location (Curtis, 2007; Gheysen and Mitchum, 2011).
More recently, Vos et al. (2013) found through SSH a clear primed defense response against M. incognita by F. mosseae in tomato. The identified differential expressed genes were mainly classified in the categories of defense, signal transduction and protein synthesis and modification. For example, there was a primed upregulation of chorismate synthase, which catalyzes the conversion of the ESPS product to chorismate, which is the last step in the shikimate pathway. The shikimate pathway thus seems to be implicated in AMF-mediated biocontrol in different plant species against several types of nematodes (Hao et al., 2012; Vos et al., 2013). Furthermore, the shikimate pathway produces precursors for various aromatic secondary metabolites which are produced through the phenylpropanoid pathway among which flavonol synthase has been reported to be primed (Vos et al., 2013). The detrimental role of several phenylpropanoid pathway products, including flavonols, on M. incognita, R. similis, and P. penetrans has already been demonstrated in vitro (Wuyts et al., 2006). Through SSH, also the ROS metabolism was linked to the reduction of root-knot nematode infection in mycorrhizal tomato roots (Vos et al., 2013). Similarly, Beneventi et al. (2013) suggested an important role for ROS generation in the resistance of soybean to M. javanica as they found through pyrosequencing an over–representation of genes containing various oxidase and peroxidase domains upregulated in the incompatible interaction. Other noteworthy genes found to be primed upon infection by M. incognita in mycorrhizal tomato plants by Vos et al. (2013) were sinapoylglucose:choline sinapoyltransferase, involved in the biosynthesis of a lignin precursor and 1-aminocyclopropane-1-carboxylate oxidase (ACC oxidase), catalyzing the final step in the biosynthesis of ethylene and related to the jasmonate-ethylene dependency of ISR (Verhagen et al., 2004; Schäfer et al., 2009). These transcriptome data point toward several candidate genes by which AMF can exert biocontrol against PPN through priming of effective plant defenses. However, future research should focus on the elucidation of their specific action toward PPN, with emphasis on the proteome and metabolome AMF-associated changes.
Altered Rhizosphere Interactions
The plant-mediated effects of the AMF-mediated biocontrol go beyond MIR though: the AMF symbiosis also leads to an altered root exudation composition and level (Hodge, 2000; Jones et al., 2004), which can in turn impact the PPN in the rhizosphere in terms of hatching, motility, chemotaxis, and host location. Differences in root exudate quantity and quality between mycorrhizal and non-mycorrhizal plants have been reported for various compounds, including sugars and organic acids (Sood, 2003; Lioussanne et al., 2008; Hage-Ahmed et al., 2013), amino acids (Harrier and Watson, 2004), phenolic compounds (McArthur and Knowles, 1992), flavonoids (Steinkellner et al., 2007) and even for the plant hormone strigolactone (López-Ráez et al., 2011). The root exudation furthermore depends on the plant or AMF species involved (Badri and Vivanco, 2009; Kobra et al., 2009), as well as on the degree of symbiosis (Scheffknecht et al., 2006; Lioussanne et al., 2008).
Differential root exudation is an important instrument used by the host plant for autoregulation of the symbiosis (Pinior et al., 1999; Vierheilig et al., 2003; Vierheilig, 2004; Schaarschmidt et al., 2013). This phenomenon involves a differential root exudation depending upon the degree of colonization, and it has been proposed that the plant in doing so keep AMF colonization under a certain threshold, as well as deter pathogenic rhizospheric micro-organisms (Vierheilig et al., 2008). Vierheilig et al. (2000) first observed autoregulation of the AMF colonization in barley roots, and they hypothesized later that the AMF-mediated biocontrol was related to the autoregulation of the AMF symbiosis (Vierheilig et al., 2008). This hypothesis is supported by the findings of Pozo and Azcón-Aguilar (2007) that a critical degree of colonization is considered as a prerequisite for biocontrol, which is typically characterized by the presence of arbuscules. These structures are typically found in a mature symbiosis, and might thus coincide with the onset of the autoregulation process. Lioussanne et al. (2008) also observed that the attraction of Phytophthora nicotianae zoospores toward R. irregularis colonized root exudates changed to repellency, depending on the maturity of the AMF colonization. Vos et al. (2012b,c) investigated the effect of mycorrhizal root exudates on nematode behavior. Using a twin-chamber experimental set-up with tomato plants, M. incognita juveniles were inoculated onto a bridge connecting a tomato plant colonized by F. mosseae with a non-colonized plant (Figure 3). A few days later similar numbers of nematodes appeared to have moved from the bridge to either compartment, however, in the compartment with the mycorrhizal tomato, the nematodes appeared to have mainly gathered in the soil without penetrating the tomato roots, in contrast to the non-colonized compartment in which most nematodes had entered the plant roots. Further experiments indicated that M. incognita root penetration could even be further reduced by the additional application of mycorrhizal root exudates. Also a temporal paralysis of the second-stage infective juveniles (J2) in the presence of mycorrhizal tomato root exudates was observed in in vitro assays (Vos et al., 2012c). Moreover, mycorrhizal root exudates reduced host location and penetration by R. similis compared to non-mycorrhizal control banana plants (Vos et al., 2012c; Figure 4).
Figure 3. Visualization of the experimental set-up of a twin-chamber with tomato plants used by Dababat and Sikora (2007) and Vos et al. (2012b) to study the differential attraction of Meloidogyne incognita to mycorrhizal roots. The two plant compartments are connected by a bridge. The experiment consisted of three treatments: (i) control plants in both compartments (control treatment), (ii) mycorrhizal plants in both compartments (AMF treatment) and (iii) a control plant in the left compartment and a mycorrhizal plant in the right compartment (mixed treatment). Two days after transplanting, the compartments and bridge were watered to field capacity at time of inoculation and 2,000 freshly hatched M. incognita 2nd-stage juveniles were inoculated per twin chamber, exactly in the middle of the bridge. Twelve days after inoculation, nematode penetration was assessed in control and mycorrhizal root systems of all treatments.
Figure 4. In vitro chemotaxis bio-assay with visualization of nematode tracks on the medium. Pictures were taken 1 h after inoculation with 10 female Radopholus similis nematodes in the middle of the plate. Three hours before nematode inoculation, the opposite wells in the agar medium were filled with (A) water as control, (B) 1% acetic acid (left hole) versus 0,5M CaCl2 (right hole) as repellent and attractive control, or (C) exudates of non-mycorrhizal roots (left) versus exudates of mycorrhizal roots (right) to observe chemotactic behavior of the nematode. Lower nematode movement can be observed in the plate with mycorrhizal root exudates, and the nematodes clearly show a chemotactic response away from them. For experimental set-up, see Vos et al. (2012c).
Altered root exudation can also cause a change in microbial diversity in the rhizosphere, and therefore affect plant-pathogen interactions (Bais et al., 2006; Lioussanne, 2010). Some reports show an increase in facultative anaerobic bacteria, fluorescent pseudomonads, Streptomyces species and chitinase-producing actinomycetes after AMF colonization (Marschner and Baumann, 2003; Wamberg et al., 2003; Harrier and Watson, 2004; Scheublin et al., 2010; Miransari, 2011; Nuccio et al., 2013; Philippot et al., 2013). These micro-organisms can also have antagonistic potential against PPN, either by direct effects such as by nematode-trapping or egg-parasitizing fungi, but also by induction of the plant defense (Kerry, 2000; Tian et al., 2007; Zamioudis and Pieterse, 2012). Root exudates originating from mycorrhizal plants have, for example, been reported to attract plant growth promoting bacteria such as Pseudomonas fluorescens (Sood, 2003) and to affect beneficial soil micro-organisms such as Trichoderma spp. (Filion et al., 1999; Druzhinina et al., 2011) which also have biocontrol potential against PPN (Dong and Zhang, 2006; Sikora et al., 2008). In line with this, Cameron et al. (2013) recently presented an adaptation to the model of MIR in which the induction of systemic resistance by mycorrhizosphere bacteria is emphasized. MIR has also been shown to act against several PPN in dixenic in vitro culture (Elsen et al., 2001; Koffi et al., 2013), clearly suggesting that the AMF-mediated biocontrol does not act only through a change in soil biota, but it might be an important additional factor contributing to the biocontrol under field conditions.
In this review we provide an overview of the different mechanisms that have been proposed for AMF-mediated biocontrol, and specifically discuss their potential involvement in reducing PPN infections. The biocontrol effect depends on several factors such as the species involved, meaning that case-by-case studies will have to be carried out to result in field applications of AMF. Biocontrol effects of AMF on PPN have been reported since many years, but due to the technological progress that has been made in recent years we can now unravel the mechanisms behind. The sequencing of the genome of the root-knot nematodes M. incognita (Abad et al., 2008) and M. hapla (Opperman et al., 2008), the cyst nematode G. pallida (Cotton et al., 2014) and of host plants such as soybean (Schmutz et al., 2010), Medicago truncatula (Young et al., 2011) and several members of the Solanaceae family (Xu et al., 2011; Sato et al., 2012) are already contributing to increased insights. In addition, with the increase in microbiome studies, the importance of the mycorrhizosphere in the AMF-mediated biocontrol will be confirmed in the years to come. Progress will also be aided by the shift in attention to the plant root interactions with micro-organisms (De Coninck et al., 2015). This attention shift should already be taken into account in practice, as Castellanos-Morales et al. (2011) showed that older cultivars of wheat (before 1950) showed higher degrees of AMF root colonization compared to modern varieties (after 1950), also showing a higher bioprotective effect by AMF against the pathogen Gaeumannomyces graminis. Therefore, some consideration should be given to the trait of the ability to form symbiosis with AMF in future breeding efforts.
As the market for beneficial microbial inocula is growing steadily (Glare et al., 2012) and the development of beneficial microbial inocula for large-scale field application is moving forward quickly (Ijdo et al., 2011; Salvioli and Bonfante, 2013), field applications of AMF might be realistic. Thus far, few research about AMF-mediated biocontrol involved “omics” tools and systems biology approaches (Salvioli and Bonfante, 2013) but this will increase over time and provide more detailed insights in the complex mechanisms underlying AMF-mediated biocontrol. These insights might in turn lead to the effective application of AMF in the field.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
This work was financially supported by a specialization grant from the Institute for the Promotion of Innovation through Science and Technology in Flanders (IWT-Vlaanderen) to NS and an EU Marie-Curie International Outgoing Fellowship (PIOF-GA-2013-625551) to CV. NS is the main author. DDW corrected the first drafts of the manuscript and commented on the views and statements put forward with emphasis on the nematological content of the manuscript. BP was responsible for the daily supervision of the PhD work of NS, corrected the drafts of the manuscript and commented on its content. CV designed the review outline, co-wrote the manuscript and designed the figures.
Abad, P., Gouzy, J., Aury, J.-M., Castagnone-Sereno, P., Danchin, E. G. J., Deleury, E., et al. (2008). Genome sequence of the metazoan plant-parasitic nematode Meloidogyne incognita. Nat. Biotechnol. 26, 909–915. doi: 10.1038/nbt.1482
Alban, R., Guerrero, R., and Toro, M. (2013). Interactions between a root-knot nematode (Meloidogyne exigua) and arbuscular mycorrhizae in coffee plant development (Coffea arabica). Am. J. Plant Sci. 4, 19–23. doi: 10.4236/ajps.2013.47A2003
Andrade, L. B. D. S., Oliveira, A. S., Ribeiro, J. K. C., Kiyota, S., Vasconcelos, I. M., De Oliveira, J. T. A., et al. (2010). Effects of a novel pathogenesis-related class 10 (PR-10) protein from Crotalaria pallida roots with papain inhibitory activity against root-knot nematode Meloidogyne incognita. J. Agric. Food Chem. 58, 4145–4152. doi: 10.1021/jf9044556
Bais, H. P., Weir, T. L., Perry, L. G., Gilroy, S., and Vivanco, J. M. (2006). The role of root exudates in rhizosphere interactions with plants and other organisms. Annu. Rev. Plant Biol. 57, 233–266. doi: 10.1146/annurev.arplant.57.032905.105159
Baum, C., El-Tohamy, W., and Gruda, N. (2015). Increasing the productivity and product quality of vegetable crops using arbuscular mycorrhizal fungi: a review. Sci. Hortic. (Amsterdam). 187, 131–141. doi: 10.1016/j.scienta.2015.03.002
Beneventi, M. A., da Silva, O. B., de Sá, M. E. L., Firmino, A. A. P., de Amorim, R. M. S., Albuquerque, E. V. S., et al. (2013). Transcription profile of soybean-root-knot nematode interaction reveals a key role of phytohormones in the resistance reaction. BMC Genomics 14:322. doi: 10.1186/1471-2164-14-322
Bodker, L., Kjoller, R., and Rosendahl, S. (1998). Effect of phosphate and the arbuscular mycorrhizal fungus Glomus intraradices on disease severity of root rot of peas (Pisum sativum) caused by Aphanomyces euteiches. Mycorrhiza 8, 169–174.
Calvet, C., Pinochet, J., Hernández-Dorrego, A., Estaún, V., and Camprubí, A. (2001). Field microplot performance of the peach-almond hybrid GF-677 after inoculation with arbuscular mycorrhizal fungi in a replant soil infested with root-knot nematodes. Mycorrhiza 10, 295–300. doi: 10.1007/PL00009998
Castellanos-Morales, V., Keiser, C., Cárdenas-Navarro, R., Grausgruber, H., Glauninger, J., García-Garrido, J. M., et al. (2011). The bioprotective effect of AM root colonization against the soil-borne fungal pathogen Gaeumannomyces graminis var. tritici in barley depends on the barley variety. Soil Biol. Biochem. 43, 831–834. doi: 10.1016/j.soilbio.2010.12.020
Chan, Y., He, Y., Hsiao, T., Wang, C., Tian, Z., and Yeh, K. (2015). Pyramiding taro cystatin and fungal chitinase genes driven by a synthetic promoter enhances resistance in tomato to root-knot nematode Meloidogyne incognita. Plant Sci. 231, 74–81. doi: 10.1016/j.plantsci.2014.11.010
Chan, Y. L., Cai, D., Taylor, P. W. J., Chan, M. T., and Yeh, K. W. (2010). Adverse effect of the chitinolytic enzyme PjCHI-1 in transgenic tomato on egg mass production and embryonic development of Meloidogyne incognita. Plant Physiol. 59, 922–930. doi: 10.1111/j.1365-3059.2010.02314.x
Cooper, W. R., Jia, L., and Goggin, L. (2005). Effects of jasmonate-induced defenses on root-knot nematode infection of resistant and susceptible tomato cultivars. J. Chem. Ecol. 31, 1953–67. doi: 10.1007/s10886-005-6070-y
Cordier, C., Pozo, M. J., Barea, J. M., Gianinazzi, S., and Gianinazzi-Pearson, V. (1998). Cell defense responses associated with localized and systemic resistance to Phytophthora parasitica induced in tomato by an arbuscular mycorrhizal fungus. Mol. Plant Microbe Interact. 11, 1017–1028. doi: 10.1094/MPMI.19188.8.131.527
Cotton, J. A, Lilley, C. J., Jones, L. M., Kikuchi, T., Reid, A. J., Thorpe, P., et al. (2014). The genome and life-stage specific transcriptomes of Globodera pallida elucidate key aspects of plant parasitism by a cyst nematode. Genome Biol. 15, R43. doi: 10.1186/gb-2014-15-3-r43
Coyne, D. L., Sahrawat, K. L., and Plowright, R. A. (2004). The influence of mineral fertilizer application and plant nutrition on plant-parasitic nematodes in upland and lowland rice in Côte d’Ivoire and its implications in long term agricultural research trials. Exp. Agric. 40, 245–256. doi: 10.1017/S0014479703001595
Dababat, A. E. A., and Sikora, R. A. (2007). Influence of the mutualistic endophyte Fusarium oxysporum 162 on Meloidogyne incognita attraction and invasion. Nematology 9, 771–776. doi: 10.1163/156854107782331225
De Coninck, B., Timmermans, P., Vos, C., Cammue, B. P. A., and Kazan, K. (2015). What lies beneath: belowground defense strategies in plants. Trends Plant Sci. 20, 91–101. doi: 10.1016/j.tplants.2014.09.007
De la Peña, E., Echeverría, S. R., Putten, W. H., Van Der Freitas, H., and Moens, M. (2003). Mechanism of control of root-feeding nematodes by mycorrhizal fungi in the dune grass Ammophila arenaria. New Phytol. 169, 829–840. doi: 10.1111/j.1469-8137.2005.01602.x
del Mar Alguacil, M., Torrecillas, E., Lozano, Z., and Roldán, A. (2011). Evidence of differences between the communities of arbuscular mycorrhizal fungi colonizing galls and roots of Prunus persica infected by the root-knot nematode Meloidogyne incognita. Appl. Environ. Microbiol. 77, 8656–8661. doi: 10.1128/AEM.05577-11
Dos Anjos, É. C. T., Cavalcante, U. M. T., Gonçalves, D. M. C., Pedrosa, E. M. R., dos Santos, V. F., and Maia, L. C. (2010). Interactions between an arbuscular mycorrhizal fungus (Scutellospora heterogama) and the root-knot nematode (Meloidogyne incognita) on sweet passion fruit (Passiflora alata). Brazilian Arch. Biol. Technol. 53, 801–809. doi: 10.1590/S1516-89132010000400008
Druzhinina, I. S., Seidl-Seiboth, V., Herrera-Estrella, A., Horwitz, B. A., Kenerley, C. M., Monte, E., et al. (2011). Trichoderma: the genomics of opportunistic success. Nat. Rev. Microbiol. 9, 749–759. doi: 10.1038/nrmicro2637
Elsen, A., Beeterens, R., Swennen, R., and De Waele, D. (2003a). Effects of an arbuscular mycorrhizal fungus and two plant-parasitic nematodes on Musa genotypes differing in root morphology. Biol. Fertil. Soils 38, 367–376. doi: 10.1007/s00374-003-0669-3
Elsen, A., Baimey, H., Swennen, R., and De Waele, D. (2003b). Relative mycorrhizal dependency and mycorrhiza-nematode interaction in banana cultivars (Musa spp.) differing in nematode susceptibility. Plant Soil 256, 303–313. doi: 10.1023/A:1026150917522
Elsen, A., Declerck, S., and De Waele, D. (2003c). Use of root organ cultures to investigate the interaction between Glomus intraradices and Pratylenchus coffeae. Appl. Environ. Microbiol. 69, 4308–4311. doi: 10.1128/AEM.69.7.4308-4311.2003
Elsen, A., Declerck, S., and De Waele, D. (2001). Effects of Glomus intraradices on the reproduction of the burrowing nematode (Radopholus similis) in dixenic culture. Mycorrhiza 11, 49–51. doi: 10.1007/s005720100100
Elsen, A., Gervacio, D., Swennen, R., and De Waele, D. (2008). AMF-induced biocontrol against plant-parasitic nematodes in Musa sp.: a systemic effect. Mycorrhiza 18, 251–256. doi: 10.1007/s00572-008-0173-6
Fan, J. W., Hu, C. L., Zhang, L. N., Li, Z. L., Zhao, F. K., and Wang, S. H. (2015). Jasmonic acid mediates tomato’s response to root knot nematodes. J. Plant Growth Regul. 34, 196–205. doi: 10.1007/s00344-014-9457-6
Filion, M., St-Arnaud, M., and Fortin, J. A. (1999). Direct interaction between the arbuscular mycorrhizal fungus Glomus intraradices and different rhizosphere microorganisms. New Phytol. 141, 525–533. doi: 10.1046/j.1469-8137.1999.00366.x
Fiorilli, V., Catoni, M., Francia, D., Cardinale, F., and Lanfranco, L. (2011). The arbuscular mycorrhizal symbiosis reduces disease severity in tomato plants infected by Botrytis cinerea. J. Plant Pathol. 93, 237–242.
Fritz, M., Jakobsen, I., Lyngkjaer, M. F., Thordal-Christensen, H., and Pons-Kühnemann, J. (2006). Arbuscular mycorrhiza reduces susceptibility of tomato to Alternaria solani. Mycorrhiza 16, 413–9. doi: 10.1007/s00572-006-0051-z
Fusconi, A., Gnavi, E., Trotta, A., and Berta, G. (1999). Apical meristems of tomato roots and their modifications induced by arbuscular mycorrhizal and soilborne pathogenic fungi. New Phytol. 142, 505–516. doi: 10.1046/j.1469-8137.1999.00410.x
Fujimoto, T., Tomitaka, Y., Abe, H., Tsuda, S., Futai, K., and Mizukubo, T. (2011). Jasmonic acid signaling pathway of Arabidopsis thaliana is important for root-knot nematode invasion. Nematol. Res. 41, 9–17. doi: 10.3725/jjn.41.9
Gamalero, E., Pivato, B., Bona, E., Copetta, A., Avidano, L., Lingua, G., et al. (2010). Interactions between a fluorescent pseudomonad, an arbuscular mycorrhizal fungus and a hypovirulent isolate of Rhizoctonia solani affect plant growth and root architecture of tomato plants. Plant Biosyst. Int. J. Deal. Asp. Plant Biol. 144, 582–591. doi: 10.1080/11263504.2010.489315
Gao, X., Starr, J., Göbel, C., Engelberth, J., Feussner, I., Tumlinson, J., et al. (2008). Maize 9-lipoxygenase ZmLOX3 controls development, root-specific expression of defense genes, and resistance to root-knot nematodes. Mol. Plant. Microbe. Interact. 21, 98–109. doi: 10.1094/MPMI-21-1-0098
Gianinazzi, S., Gollotte, A., Binet, M.-N., van Tuinen, D., Redecker, D., and Wipf, D. (2010). Agroecology: the key role of arbuscular mycorrhizas in ecosystem services. Mycorrhiza 20, 519–30. doi: 10.1007/s00572-010-0333-3
Hage-Ahmed, K., Moyses, A., Voglgruber, A., Hadacek, F., and Steinkellner, S. (2013). Alterations in root exudation of intercropped tomato mediated by the arbuscular mycorrhizal fungus Glomus mosseae and the soilborne pathogen Fusarium oxysporum f.sp. lycopersici. J. Phytopathol. 161, 763–773. doi: 10.1111/jph.12130
Hammer, E. C., Pallon, J., Wallander, H., and Olsson, P. A. (2011). Tit for tat? A mycorrhizal fungus accumulates phosphorus under low plant carbon availability. FEMS Microbiol. Ecol. 76, 236–244. doi: 10.1111/j.1574-6941.2011.01043.x
Hao, Z., Fayolle, L., Van Tuinen, D., Chatagnier, O., Li, X., Gianinazzi, S., et al. (2012). Local and systemic mycorrhiza-induced protection against the ectoparasitic nematode Xiphinema index involves priming of defence gene responses in grapevine. J. Exp. Bot. 63, 3657–3672. doi: 10.1093/jxb/ers046
Harrier, L. A., and Watson, C. A. (2004). The potential role of arbuscular mycorrhizal (AM) fungi in the bioprotection of plants against soil-borne pathogens in organic and/or other sustainable farming systems. Pest Manag. Sci. 60, 149–57. doi: 10.1002/ps.820
Javot, H., Penmetsa, R. V., Breuillin, F., Bhattarai, K. K., Noar, R. D., Gomez, S. K., et al. (2011). Medicago truncatula mtpt4 mutants reveal a role for nitrogen in the regulation of arbuscule degeneration in arbuscular mycorrhizal symbiosis. Plant J. 68, 954–965. doi: 10.1111/j.1365-313X.2011.04746.x
Jones, J. T., Haegeman, A., Danchin, E. G. J., Gaur, H. S., Helder, J., Jones, M. G. K., et al. (2013). Top 10 plant-parasitic nematodes in molecular plant pathology. Mol. Plant Pathol. 14, 946–961. doi: 10.1111/mpp.12057
Kerry, B. R. (2000). Rhizosphere interactions and the exploitation of microbial agents for the biological control of plant-parasitic nematodes. Annu. Rev. Phytopathol. 38, 423–441. doi: 10.1146/annurev.phyto.38.1.423
Khaosaad, T., García-Garrido, J. M., Steinkellner, S., and Vierheilig, H. (2007). Take-all disease is systemically reduced in roots of mycorrhizal barley plants. Soil Biol. Biochem. 39, 727–734. doi: 10.1016/j.soilbio.2006.09.014
Kobra, N., Jalil, K., and Youbert, G. (2009). Effects of three Glomus species as biocontrol agents against Verticillium-induced wilt in cotton. J. Plant Prot. Res. 49, 185–189. doi: 10.2478/v10045-009-0027-z
Koffi, M. C., Vos, C., Draye, X., and Declerck, S. (2013). Effects of Rhizophagus irregularis MUCL 41833 on the reproduction of Radopholus similis in banana plantlets grown under in vitro culture conditions. Mycorrhiza 23, 279–288. doi: 10.1007/s00572-012-0467-6
Li, H. Y., Yang, G. D., Shu, H. R., Yang, Y. T., Ye, B. X., Nishida, I., et al. (2006). Colonization by the arbuscular mycorrhizal fungus Glomus versiforme induces a defense response against the root-knot nematode Meloidogyne incognita in the grapevine (Vitis amurensis Rupr.), which includes transcriptional activation of the class III chitin. Plant Cell Physiol. 47, 154–163. doi: 10.1093/pcp/pci231
Lioussanne, L. (2010). Review. The role of the arbuscular mycorrhiza-associated rhizobacteria in the biocontrol of soilborne phytopathogens. Spanish J. Agric. Res. 8, 3–5. doi: 10.5424/sjar/201008S1-5301
Lioussanne, L., Jolicoeur, M., and St-Arnaud, M. (2008). Mycorrhizal colonization with Glomus intraradices and development stage of transformed tomato roots significantly modify the chemotactic response of zoospores of the pathogen Phytophthora nicotianae. Soil Biol. Biochem. 40, 2217–2224. doi: 10.1016/j.soilbio.2008.04.013
López-Ráez, J. A., Charnikhova, T., Fernández, I., Bouwmeester, H., and Pozo, M. J. (2011). Arbuscular mycorrhizal symbiosis decreases strigolactone production in tomato. J. Plant Physiol. 168, 294–297. doi: 10.1016/j.jplph.2010.08.011
López-Ráez, J. A., Verhage, A., Fernández, I., García, J. M., Azcón-Aguilar, C., Flors, V., et al. (2010). Hormonal and transcriptional profiles highlight common and differential host responses to arbuscular mycorrhizal fungi and the regulation of the oxylipin pathway. J. Exp. Bot. 61, 2589–2601. doi: 10.1093/jxb/erq089
Mathys, J., De Cremer, K., Timmermans, P., Van Kerckhove, S., Lievens, B., Vanhaecke, M., et al. (2012). Genome-wide characterization of ISR induced in Arabidopsis thaliana by Trichoderma hamatum T382 against Botrytis cinerea infection. Front. Plant Sci. 3:108. doi: 10.3389/fpls.2012.00108
McArthur, D. A., and Knowles, N. R. (1992). Resistance responses of potato to vesicular-arbuscular mycorrhizal fungi under varying abiotic phosphorus levels. Plant Physiol. 100, 341–351. doi: 10.1104/pp.100.1.341
Millet, Y. A., Danna, C. H., Clay, N. K., Songnuan, W., Simon, M. D., Werck-Reichhart, D., et al. (2010). Innate immune responses activated in Arabidopsis roots by microbe-associated molecular patterns. Plant Cell 22, 973–990. doi: 10.1105/tpc.109.069658
Miransari, M., Abrishamchi, A., Khoshbakht, K., and Niknam, V. (2014). Plant hormones as signals in arbuscular mycorrhizal symbiosis. Crit. Rev. Biotechnol. 8551, 1–12. doi: 10.3109/07388551.2012.731684
Nicol, J. M., Turner, S. J., Coyne, D. L., den Nijs, L., Hockland, S., and Tahna Maafi, Z. (2011). “Current nematode threats to world agriculture,” in Genomics and Molecular Genetics of Plant-Nematode Interactions, eds J. Jones, G. Gheysen, and C. Fenoll (Heidelberg: Springer), 347–367. doi: 10.1007/978-94-007-0434-3
Norman, J., Atkinson, D., and Hooker, J. (1996). Arbuscular mycorrhizal fungal-induced alteration to root architecture in strawberry and induced resistance to the root pathogen Phytophthora fragariae. Plant Soil 185, 191–198.
Nuccio, E. E., Hodge, A., Pett-Ridge, J., Herman, D. J., Weber, P. K., and Firestone, M. K. (2013). An arbuscular mycorrhizal fungus significantly modifies the soil bacterial community and nitrogen cycling during litter decomposition. Environ. Microbiol. 15, 1870–1881. doi: 10.1111/1462-2920.12081
Opperman, C. H., Bird, D. M., Williamson, V. M., Rokhsar, D. S., Burke, M., Cohn, J., et al. (2008). Sequence and genetic map of Meloidogyne hapla: a compact nematode genome for plant parasitism. Proc. Natl. Acad. Sci. U.S.A. 105, 14802–14807. doi: 10.1073/pnas.0805946105
Orfanoudakis, M., Wheeler, C. T., and Hooker, J. E. (2010). Both the arbuscular mycorrhizal fungus Gigaspora rosea and Frankia increase root system branching and reduce root hair frequency in Alnus glutinosa. Mycorrhiza 20, 117–126. doi: 10.1007/s00572-009-0271-0
Perry, R. N., and Moens, M. (2011). “Introduction to plant-parasitic nematodes; modes of parasitism,” in Genomics and Molecular Genetics of Plant–Nematode Interactions, eds J. T. Jones, L. Gheysen, and C. Fenoll (Heidelberg: Springer), 3–20.
Pettigrew, W. T., Meredith, W. R., and Young, L. D. (2005). Potassium fertilization effects on cotton lint yield, yield components, and reniform nematode populations. Agron. J. 97, 1245–1251. doi: 10.2134/agronj2004.0321
Philippot, L., Raaijmakers, J. M., Lemanceau, P., and van der Putten, W. H. (2013). Going back to the roots: the microbial ecology of the rhizosphere. Nat. Rev. Microbiol. 11, 789–99. doi: 10.1038/nrmicro3109
Pieterse, C. M. J., Zamioudis, C., Berendsen, R. L., Weller, D. M., van Wees, S. C. M., and Bakker, P. A. H. M. (2014). Induced systemic resistance by beneficial microbes. Annu. Rev. Phytopathol. 52, 347–375. doi: 10.1146/annurev-phyto-082712-102340
Pinior, A., Wyss, U., Piché, Y., and Vierheilig, H. (1999). Plants colonized by AM fungi regulate further root colonization by AM fungi through altered root exudation. Can. J. Bot. 77, 891–897. doi: 10.1139/cjb-77-6-891
Pinochet, J., Calvet, C., Camprubí, A., and Fernández, C. (1996). Interactions between migratory endoparasitic nematodes and arbuscular mycorrhizal fungi in perennial crops: a review. Plant Soil 185, 183–190.
Pozo, M. J., Cordier, C., Dumas-Gaudot, E., Gianinazzi, S., Barea, J. M., and Azcón-Aguilar, C. (2002). Localized versus systemic effect of arbuscular mycorrhizal fungi on defence responses to Phytophthora infection in tomato plants. J. Exp. Bot. 53, 525–534. doi: 10.1093/jexbot/53.368.525
Sato, S., Tabata, S., Hirakawa, H., Asamizu, E., Shirasawa, K., Isobe, S., et al. (2012). The tomato genome sequence provides insights into fleshy fruit evolution. Nature 485, 635–641. doi: 10.1038/nature11119
Schaarschmidt, S., Gresshoff, P. M., and Hause, B. (2013). Analyzing the soybean transcriptome during autoregulation of mycorrhization identifies the transcription factors GmNF-YA1a/b as positive regulators of arbuscular mycorrhization. Genome Biol. 14, R62. doi: 10.1186/gb-2013-14-6-r62
Schäfer, P., Pfiffi, S., Voll, L. M., Zajic, D., Chandler, P. M., Waller, F., et al. (2009). Manipulation of plant innate immunity and gibberellin as factor of compatibility in the mutualistic association of barley roots with Piriformospora indica. Plant J. 59, 461–474. doi: 10.1111/j.1365-313X.2009.03887.x
Schaff, J. E., Nielsen, D. M., Smith, C. P., Scholl, E. H., and Bird, D. M. (2007). Comprehensive transcriptome profiling in tomato reveals a role for glycosyltransferase in Mi-mediated nematode resistance. Plant Physiol. 144, 1079–1092. doi: 10.1104/pp.106.090241
Scheffknecht, S., Mammerler, R., Steinkellner, S., and Vierheilig, H. (2006). Root exudates of mycorrhizal tomato plants exhibit a different effect on microconidia germination of Fusarium oxysporum f. sp. lycopersici than root exudates from non-mycorrhizal tomato plants. Mycorrhiza 16, 365–370. doi: 10.1007/s00572-006-0048-7
Scheublin, T. R., Sanders, I. R., Keel, C., and van der Meer, J. R. (2010). Characterisation of microbial communities colonising the hyphal surfaces of arbuscular mycorrhizal fungi. ISME J. 4, 752–763. doi: 10.1038/ismej.2010.5
Sikora, R. A., Pocasangre, L., Felde Zum, A., Niere, B., Vu, T. T., and Dababat, A. A. (2008). Mutualistic endophytic fungi and in planta suppressiveness to plant-parasitic nematodes. Biol. Control 46, 15–23. doi: 10.1016/j.biocontrol.2008.02.011
Smith, F. A., and Smith, S. E. (2011a). What is the significance of the arbuscular mycorrhizal colonisation of many economically important crop plants? Plant Soil 348, 63–79. doi: 10.1007/s11104-011-0865-0
Smith, S. E., and Smith, F. A. (2011b). Roles of arbuscular mycorrhizas in plant nutrition and growth: new paradigms from cellular to ecosystem scales. Annu. Rev. Plant Biol. 62, 227–250. doi: 10.1146/annurev-arplant-042110-103846
Smith, S. E., Facelli, E., Pope, S., and Smith, F. A. (2010). Plant performance in stressful environments: interpreting new and established knowledge of the roles of arbuscular mycorrhizas. Plant Soil 326, 3–20. doi: 10.1007/s11104-009-9981-5
Sood, G. S. (2003). Chemotactic response of plant-growth-promoting bacteria towards roots of vesicular-arbuscular mycorrhizal tomato plants. FEMS Microbiol. Ecol. 45, 219–227. doi: 10.1016/S0168-6496(03)00155-7
Soriano, I. R., Asenstorfer, R. E., Schmidt, O., and Riley, I. T. (2004). Inducible flavone in oats (Avena sativa) is a novel defense against plant-parasitic nematodes. Phytopathology 94, 1207–1214. doi: 10.1094/PHYTO.2004.94.11.1207
Steinkellner, S., Lendzemo, V., Langer, I., Schweiger, P., Khaosaad, T., Toussaint, J.-P., et al. (2007). Flavonoids and strigolactones in root exudates as signals in symbiotic and pathogenic plant-fungus interactions. Molecules 12, 1290–1306. doi: 10.3390/12071290
Stoffelen, R., Verlinden, R., Xuyen, N. T., De Waele, D., and Swennen, R. (2000). Host plant response of Eumusa and Australimusa bananas (Musa spp.) to migratory endoparasitic and root-knot nematodes. Nematology 2, 907–916. doi: 10.1163/156854100750112851
Tian, B., Yang, J., and Zhang, K. Q. (2007). Bacteria used in the biological control of plant-parasitic nematodes: populations, mechanisms of action, and future prospects. FEMS Microbiol. Ecol. 61, 197–213. doi: 10.1111/j.1574-6941.2007.00349.x
Verhagen, B. W. M., Glazebrook, J., Zhu, T., Chang, H.-S., van Loon, L. C., and Pieterse, C. M. J. (2004). The transcriptome of rhizobacteria-induced systemic resistance in Arabidopsis. Mol. Plant. Microbe. Interact. 17, 895–908. doi: 10.1094/MPMI.2004.17.8.895
Vierheilig, H., Garcia-Garrido, J. M., Wyss, U., and Piché, Y. (2000). Systemic suppression of mycorrhizal colonization of barley roots already colonized by AM fungi. Soil Biol. Biochem. 32, 589–595. doi: 10.1016/S0038-0717(99)00155-8
Vierheilig, H., Lerat, S., and Piché, Y. (2003). Systemic inhibition of arbuscular mycorrhiza development by root exudates of cucumber plants colonized by Glomus mosseae. Mycorrhiza 13, 167–170. doi: 10.1007/s00572-002-0219-0
Vierheilig, H., Steinkellner, S., and Khaosaad, T. (2008). “The biocontrol effect of mycorrhization on soilborne fungal pathogens and the autoregulation of the AM symbiosis: one Mechanism, Two Effects?” in Mycorrhiza, ed. A. Varma (Berlin: Springer-Verlag), 307–320. doi: 10.1007/978-3-540-78826-3_15
Vigo, C., Norman, J. R., and Hooker, J. E. (2000). Biocontrol of the pathogen Phytophthora parasitica by arbuscular mycorrhizal fungi is a consequence of effects on infection loci. Plant Physiol. 49, 509–514. doi: 10.1046/j.1365-3059.2000.00473.x
Vos, C. M., Tesfahun, A. N., Panis, B., De Waele, D., and Elsen, A. (2012a). Arbuscular mycorrhizal fungi induce systemic resistance in tomato against the sedentary nematode Meloidogyne incognita and the migratory nematode Pratylenchus penetrans. Appl. Soil Ecol. 61, 1–6. doi: 10.1016/j.apsoil.2012.04.007
Vos, C., Claerhout, S., Mkandawire, R., Panis, B., de Waele, D., and Elsen, A. (2012b). Arbuscular mycorrhizal fungi reduce root-knot nematode penetration through altered root exudation of their host. Plant Soil 354, 335–345. doi: 10.1007/s11104-011-1070-x
Vos, C., Van Den Broucke, D., Lombi, F. M., De Waele, D., and Elsen, A. (2012c). Mycorrhiza-induced resistance in banana acts on nematode host location and penetration. Soil Biol. Biochem. 47, 60–66. doi: 10.1016/j.soilbio.2011.12.027
Vos, C., Schouteden, N., van Tuinen, D., Chatagnier, O., Elsen, A., De Waele, D., et al. (2013). Mycorrhiza-induced resistance against the root-knot nematode Meloidogyne incognita involves priming of defense gene responses in tomato. Soil Biol. Biochem. 60, 45–54. doi: 10.1016/j.soilbio.2013.01.013
Wamberg, C., Christensen, S., Jakobsen, I., Müller, a. K., and Sørensen, S. J. (2003). The mycorrhizal fungus (Glomus intraradices) affects microbial activity in the rhizosphere of pea plants (Pisum sativum). Soil Biol. Biochem. 35, 1349–1357. doi: 10.1016/S0038-0717(03)00214-1
Wuyts, N., Swennen, R., and De Waele, D. (2006). Effects of plant phenylpropanoid pathway products and selected terpenoids and alkaloids on the behaviour of the plant-parasitic nematodes Radopholus similis, Pratylenchus penetrans and Meloidogyne incognita. Nematology 8, 89–101. doi: 10.1163/156854106776179953
Yang, H., Zhang, Q., Dai, Y., Liu, Q., Tang, J., Bian, X., et al. (2014). Effects of arbuscular mycorrhizal fungi on plant growth depend on root system: a meta-analysis. Plant Soil 389, 361–374. doi: 10.1007/s11104-014-2370-8
Young, N. D., Debellé, F., Oldroyd, G. E. D., Geurts, R., Cannon, S. B., Udvardi, M. K., et al. (2011). The Medicago genome provides insight into the evolution of rhizobial symbioses. Nature 480, 520–524. doi: 10.1038/nature10625
Keywords: arbuscular mycorrhizal fungi, biocontrol, cyst nematodes, induced systemic resistance, plant-parasitic nematodes, migratory nematodes, mycorrhiza induced resistance, root-knot nematodes
Citation: Schouteden N, De Waele D, Panis B and Vos CM (2015) Arbuscular Mycorrhizal Fungi for the Biocontrol of Plant-Parasitic Nematodes: A Review of the Mechanisms Involved. Front. Microbiol. 6:1280. doi: 10.3389/fmicb.2015.01280
Received: 26 August 2015; Accepted: 31 October 2015;
Published: 17 November 2015.
Edited by:Aurelio Ciancio, Istituto per la Protezione Sostenibile delle Piante, Italy
Reviewed by:Maria J. Pozo, Consejo Superior de Investigaciones Científicas, Spain
Isabel Abrantes, Centre for Functional Ecology, Portugal
Erwin O. Aballay, Universidad de Chile, Chile
Copyright © 2015 Schouteden, De Waele, Panis and Vos. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Christine M. Vos, email@example.com