Abstract
Plants are associated with complex microbiomes, and many of the microorganisms that reside on plant surfaces (epiphytes) or within plant tissues (endophytes) are beneficial for the host plant and improve plant growth or stress resistance by a variety of plant growth-promoting capabilities. The plant microbiome could serve as a tool box to design synthetic microbiomes to enhance plant growth and crop resiliency under stress or to integrate benefits of plant microbiomes as important traits into plant breeding programs. For legumes, the most important members of the plant microbiome are nitrogen (N)-fixing rhizobia and arbuscular mycorrhizal (AM) fungi. Legumes harbor rhizobia in specialized root nodules, in which the bacteria fix gaseous N from the atmosphere and transfer plant available forms of N to host. AM fungi play a key role for the uptake of nutrients such as phosphate and nitrogen and improve the resistance of plants against abiotic (e.g. drought, salinity, and heavy metals) and biotic (herbivores and pathogens) stresses. Both partners compete with these benefits for photosynthetically fixed carbon from the host. In this review, we will summarize our current understanding of these interactions and will also focus on cooperative or competitive interactions between these two root symbionts in tripartite interactions.
Keywords
- arbuscular mycorrhizal symbiosis
- biological nitrogen fixation
- mutualism
- nutrient uptake
- plant biotic interaction
- rhizobia
1. Introduction
Plants are sessile organisms, and to compensate for their lack in mobility, plants evolved specialized mechanisms that allowed them to adapt to changing environments and to a variety of abiotic and biotic stresses. Arguably, the most important adaptation to stress was the development of beneficial plant microbe interactions. Due to recent developments in sequencing technologies, we have a better understanding of the concept that plants are meta-organisms, whose phenotype, particularly under stress, is not only shaped by plant traits but also by their associated microbiomes. The plant microbiome represents “the second plant genome” and consists of 10 times more genes than typical plant genomes and is an unexplored resource for a wide range of potentially plant growth-promoting capabilities [1]. A better understanding of beneficial plant microbe interactions could be a key to the development of microbial fertilizers or microbial pesticides, as well as new biotechnological tools that increase the nutrient efficiency and stress tolerance of crops in environments that are increasingly affected by climate change and other stresses.
The most important root symbioses for legumes are interactions with nitrogen-fixing rhizobia and arbuscular mycorrhizal (AM) fungi. Legumes harbor rhizobia in specialized root organs or nodules, and their biological nitrogen (N) fixation can contribute with up to 77% to the total N nutrition of crop legumes [2]. AM fungi colonize the majority of land plants and transfer nutrients such as phosphate (P), N, and potassium (K) to their host and improve the host plant’s resistance against abiotic (drought, salinity, and heavy metals) and biotic (herbivores and root pathogens) stresses [3]. Arbuscule-like structures found in the cells of early land plant fossils suggests that the AM symbiosis played a key role during the evolution of land plants, and the AM symbiosis is therefore also called “the mother of all root endosymbioses” [4, 5]. We will focus here on the symbiosis between legumes, rhizobia, and AM fungi and will summarize our current knowledge about the development and nutritional benefits of these interactions and discuss knowledge gaps that still limit their application potential.
2. Beneficial root symbioses of legumes
2.1 Arbuscular mycorrhizal symbiosis
The arbuscular mycorrhizal (AM) symbiosis is a mutualistic interaction between approximately 70% of all known land plant species and fungi of the phylum
Roots that are colonized with AM fungi have two pathways for nutrient uptake: the plant uptake pathway (PP) and the mycorrhizal uptake pathway (MP). The PP involves the uptake of nutrients from the soil via high- or low-affinity uptake transporters in the epidermis or root hairs. However, nutrients such as P are relatively immobile in the soil, and the efficiency of the PP is often limited by the development of depletion zones around the roots. The MP, on the other hand, is characterized by the uptake of nutrients from the soil via high-affinity nutrient transporters in the ERM, followed by the translocation of nutrients from the ERM to the IRM in the root cortex, and the uptake of nutrients from the mycorrhizal interface through AM-inducible plant uptake transporters. In AM roots, the MP represents often the dominant pathway for plant nutrient uptake [9, 10].
AM fungi and their plant partners form a complex network of many-to-many interactions; each plant host is colonized by communities of AM fungi, and AM fungi colonize multiple host plants and connect plants via common mycorrhizal networks (CMNs). CMNs are involved in the long-distance transport of nutrients, water, stress chemicals, and allelochemicals and allow plants to “communicate” with other plants of the same or of different species that share the same CMN [11, 12, 13]. Many-to-many interactions allow both partners in the AM symbiosis to choose among multiple trading partners and force both partners to compete with other partners for nutrient or carbon resources.
The colonization of the root by AM fungi is initiated through a bidirectional exchange of signals. Before the AM symbiosis is established, plants release the carotenoid-derived plant hormone strigolactone, which activates fungal metabolism and stimulates hyphal branching during the pre-symbiotic growth phase (Figure 1) [14, 15, 16]. In addition to their role in plant partner recognition in parasitic and beneficial plant microbe interactions, strigolactones play a key role for the adaptation of plants against a variety of abiotic stresses and actively participate within regulatory networks of plant stress adaptation regulated by phytohormones. Abiotic stresses that have been shown to affect strigolactone production and/or the expression of genes involved in strigolactone biosynthesis include P and N deficiency, heat, UV, wounding, salinity, and drought [17]. For example, as part of the P starvation signal activated by PHR proteins in plants, strigolactone biosynthesis increases [18]. In response to strigolactones, AM fungi secrete Myc factors that are composed of lipo-chitooligosaccharides (LCOs) and chitin oligomers and are likely recognized by LysM-receptor-like kinases of the plant (RLKs) and prepare the root for colonization.
The developmental events in the establishment of the AM symbiosis include epidermal penetration, restructuring of the underlying epidermal and cortical cells, the assembly of a pre-penetration apparatus (PPA), intraradical colonization by hyphal elongation, and the development of arbuscules in inner cortical cells (Figure 1). After fungal hyphae have established contact with the host root, the AM fungus forms an appressorium or hyphopodium, a specialized cell or adhesion structure on the root surface. After the recognition of AM fungal appressoria, root epidermal cells develop a PPA, which directs AM hyphae through the epidermis into the root cortex and controls the intracellular path of hyphal penetration [19]. Arbuscules are highly branched structures that act as sites of nutrient exchange between the fungal and plant partner. Concurrent with these morphological events, a signaling cascade involving receptor kinases, nucleoproteins, ion channels, and a transcriptional complex takes place to accommodate the fungus inside roots (see 2.3 below).
2.2 The rhizobium-legume symbiosis
Legumes are characterized by their ability to establish symbiotic interactions with diazotrophic soil bacteria (known as rhizobia). Rhizobia can fix gaseous N2 and convert it into plant-available forms of N in specialized root structures or nodules. Critical for the establishment of the symbiosis between legumes and rhizobia is a two-way recognition process between both partners. A key component of this recognition process is the secretion of flavonoid compounds by plant roots, which are recognized through bacterial NodD receptors and induce the biosynthesis of bacterial lipo-chitooligosaccharides or Nod-factors. The production of flavonoids and the expression of chalcone synthase (the first committed enzyme of flavonoid biosynthesis) and isoflavone reductase (conversion of flavanones to isoflavones) is triggered by N deficiency of the plant [20]. NodD belongs to the family of LysR-type transcriptional regulators that mediate the expression of nodulation (
Unlike the AM symbiosis, the rhizobium-legume (RL) symbiosis is highly specific, and each rhizobial strain establishes a symbiosis with only a limited number of host plants and vice versa [24]. The ability of rhizobial species to recognize and interpret specific flavonoid signals produced by compatible host plants through NodD is in part responsible for the host specificity in RL interactions [25]. There is also a high level of specificity at the N-fixing stage in the RL symbiosis. Bacterial strains can form N-fixing root nodules on one plant genotype (Nod+/Fix+) and nodulate other plant genotypes, but the formed nodules of this plant are unable to fix N (Nod+/Fix−). This specificity is caused by the nodule-specific cysteine-rich (NCR) peptides NFS1 and NFS2 of the plant, which induce bacterial cell death, and early nodule senescence dependent on the rhizobial strain and the genetic background of the host. It has been suggested that NCR peptides possess prosymbiotic and antisymbiotic properties and that they play a role in fine-tuning the activity of rhizobia for optimum symbiotic performance [26].
Parallel to the change in root morphology, which includes cortical cell division and differentiation into nodule primordia, rhizobia are directed into the cortex. Rhizobia can enter roots through nod-dependent infection pockets formed during root curling via tubular infection threads (ITs) or cracks in the root surface. In addition, rhizobia can also gain entry via intercellular spaces through a nod-factor-independent process [27]. Necessary for most infections in legumes, however, is root hair curling, which involves root hairs that are tightly bending and entrap bacteria in a “shepherds crook” structure [28]. This deformation of root hairs is typically only induced by the release of Nod factors from bacteria closely attached to root hair tips. In some legumes, the Nod factor (NodRm-1 in
In legumes, two types of root nodules can be distinguished. Indeterminate nodules develop after Nod factor perception as a result of periclinal cell divisions in the pericycle followed by inner cortical cell proliferation. Indeterminate nodules are characterized by a persistent meristem and the development of distinct zones within the root nodule: meristem, infection zone, interzone, fixation zone, and senescence zone. By contrast, determinate nodules have a defined lifespan and lose their central meristem. Determinate nodules develop by cell divisions in the outer root cortex, but the cells lose their meristematic activity when the nodule matures [31]. The bacteria are taken up by a process similar to endocytosis of the plasma membrane where bacteria proliferate into N-fixing bacteroids and form a symbiosome, an organelle-like structure consisting of 1–10 bacteroids enclosed by a plant-derived peribacteroid membrane or symbiosome membrane (SYM) and the symbiosome space that is located between the bacteroids and the SYM [32].
2.3 The common symbiosis signaling pathway
AM or RL symbiosis play a critical role for the nutrient supply of their host, and low Pi or N supply conditions have been shown to stimulate the release of strigolactones or flavonoids by host plants to recruit AM fungi or rhizobia. AM fungi and rhizobia respond to these signals with the release of Myc or Nod factors, respectively, which are composed of sulfated or non-sulfated lipo-chitooligosaccharides [33]. The perception and interpretation of Myc or Nod factors by the host plant plays a critical role in the establishment of both root symbioses. Compared to the AM symbiosis, which evolved around 450 to 480 million years ago, the mutualistic RL symbiosis is much younger and evolved approximately 58 million years ago [34]. The similarities in the signaling pathways of the AM and RL symbiosis has led to the assumption that the RL symbiosis evolved via the adoption of a signaling pathway that had previously been established for the successful colonization of plants by AM fungi. Similarly, the same signaling pathway can also be found in ectomycorrhizal associations that evolved also much later than the AM symbiosis [35, 36]. The common symbiotic signaling pathway (CSSP) is a conserved molecular signaling pathway that plays a key role in the establishment of the AM and RL symbiosis and acts downstream of Myc and Nod factor perception and upstream of the activation of processes required for the root colonization by specific root symbionts. Mutations in the CSSP prevent both fungal and bacterial entry into the host root [37].
The first component of the CSSP are heteromers of plasma membrane-localized lysin motif-type receptor-like kinases, such as the Nod factor receptors NFR1/NFR5 in
Downstream of Myc or Nod factor perception, the symbiosis receptor-like kinase SYMRK is indispensable for the development of the AM or rhizobial symbiosis. In
After the CSSP, specific signaling pathways regulate the development of the AM or RL symbiosis. In the AM symbiosis, molecular signaling coincides with the initiation of a PPA in plant cells to accommodate the invading fungus [50]. Subsequent fungal infection involves hyphal elongation and cortical root colonization and arbuscule formation. Arbuscule formation is regulated by a complex consisting of CCaMK, CYCLOPS, and DELLA proteins, which induce the essential GRAS gene
By contrast, in the RL symbiosis, several nuclear-associated transcriptional regulators are essential for the expression of Nod-factor-induced genes and the initiation of nodulation, including nodule inception (NIN) [53], an ERF family protein (ERN) [54], and two GRAS family proteins, nodulation signaling pathway 1 (NSP1) and NSP2 [55, 56]. DELLA proteins promote nodule development and infection thread formation during root nodule symbiosis by promoting CCaMK-IPD3/CYCLOPS complex formation and increasing IPD3/CYCLOPS phosphorylation. DELLAs can also form a protein complex with NSP2 and NSP1 and bridge a protein complex containing IPD3/CYCLOPS and NSP2. It has been suggested that the combination of transcription factors such as NSP2 and NSP1 and CCaMK-IDP3 may act in tandem to control the expression of early nodulin genes [57]. First, the phosphorylated form of CYCLOPS (IPD3 in
3. Nutrient uptake and transport across the mycorrhizal interface
3.1 Phosphate uptake and transport
The total phosphate (P) contents in soils can be high, but a large percentage of this P is not plant available. In addition to organic forms of P, inorganic phosphate (Pi) readily binds with iron, aluminum, and manganese when the pH in the soil is acidic or binds with calcium or calcium carbonate when the soil is alkaline and then becomes plant unavailable [59]. Due to the low soil concentrations, P is often a growth-limiting nutrient for plants (accounts for 0.2% of dry weight). In addition, due to the low P mobility in soils, plant P uptake leads rapidly to the development of depletion zones around the roots that further limit plant P uptake to the slow rate of diffusion. The ability of AM fungi to grow with their ERM beyond these depletion zones combined with their efficient P uptake systems is the main basis for their positive impact on P uptake and plant growth. Plants and fungi absorb P as negatively charged P ions (H2PO4−). To take up P against the concentration gradient, high-affinity transporter proteins from the Pht1 family are required, which transport P into cells via a proton gradient generated by a plasma membrane H+-ATPase [60].
During the development of arbuscules, the colonized cell undergoes a reorganization and starts to enclose newly formed hyphal branches of the arbuscule by a novel symbiosis-specific membrane, the periarbuscular membrane (PAM), which is an extension of the plant plasma membrane. The PAM plays a vital role in the nutrient exchange between the symbiotic partners and is composed of a variety of transport proteins specifically designed to facilitate the nutrient uptake from the symbiotic interface (Figure 3). The most extensively studied membrane proteins in the PAM are inorganic phosphate (Pi) transporters of the PHT1 gene family, such as MtPT4, LjPT4, and OsPT11 that were characterized in
The PAM also contains P transporters that are essential for AM development but are not critical for symbiotic Pi uptake. For example, OsPT11 and OsPT13 are both critical for AM development in rice, and mutations in both transporters interfere with intraradical fungal development and growth of arbuscules, but only OsPT11 plays an active role in symbiotic Pi uptake. It has been suggested that OsPT13 could play a role as a Pi sensor at the PAM that regulates the development of arbuscules and thereby maximizes their symbiotic transport activity [64]. Similarly, AsPT1 and AsPT4, two AM-induced Pi transporters of
3.2 Nitrogen uptake and transport
Nitrogen (N) is a major driver for crop yield, and its availability significantly impacts agricultural productivity. Since N can constitute in plant tissues between 1 and 5% of the total dry matter, plants require N in large quantities, and N is the nutrient that most often limits plant growth [66]. In soils, N is present in inorganic forms, such as nitrate (NO3−) or ammonium (NH4+), and in organic form, such as urea, free amino acids, and short peptides. The availability of these N pools, however, varies considerably due to soil heterogeneity and dynamic microbial conversions of these different N forms (e.g. nitrification and denitrification) [67]. In most aerobic soils, NO3− is the primary type of N, whereas NH4+ can be the dominant form of N in acidic and/or anaerobic soils [68]. Plants can take up NH4+, NO3−, and organic N, but due to the strong competition with microorganisms for organic N uptake, they take up NH4+ and NO3− in larger quantities [69]. NO3− is very mobile in soils and readily leached, while NH4+ adsorbs onto the cation exchange complex of many soils and is only slowly released. Because plants have to also compete for NH4+ with soil microorganisms, which use NH4+ not only as an N source but also as an energy source and convert NH4+ into NO3− via nitrification, NO3− is a major N source for most higher plants [70].
The ERM of fungi can take up NH4+ and NO3−, but due to its higher energy efficiency, AM fungi typically prefer the uptake of NH4+ over NO3− [71]. AM fungi have high-affinity and low-affinity uptake systems for NH4+. Fungal high-affinity uptake systems for NH4 have lower
Labeling, enzymatic measurements, and gene expression data suggest that N that is taken up by the AM fungus is first assimilated and converted to the amino acid arginine in hyphae of the ERM, then transferred via polyphosphates (polyP) to the intraradical mycelium (IRM), and in the IRM, arginine is converted back to NH4+ via the urea cycle before it is released into the AM interface [71, 74, 80]. In several plant species, NH4+ transporters of the AMT2 family are specifically expressed during AM symbiosis and are located in the PAM [81, 82, 83]. In
LjAMT2;2, an NH4+ transporter in the PAM of
3.3 Potassium uptake and transport
Potassium (K) is a necessary macronutrient that plays a key role in enzyme activation, osmotic regulation, plant cell turgor generation, cell expansion, control of membrane electric potential, and pH homeostasis [66]. Plants have evolved a variety of transporters that differ in their structure and their transport mechanisms for the uptake of K from the soil, including voltage-gated K-channels, the carrier-like families KT/HAK/KUP, HKT uniporters and symporters, and cation-proton antiporters [for review see 88]. AM fungi have also been shown to have a positive impact on the K nutrition of their host plant, but the molecular mechanisms of fungal K transport are not well understood [89, 90]. The AM symbiosis triggers transcriptional responses in
3.4 Water uptake and transport
In addition to elemental nutrients, water is essential to drive plant growth and nutrient uptake. It is long known that AM fungi can have a positive impact on plant-water relations and can significantly improve the tolerance of plants to drought [94]. The positive impact of AM fungi on drought tolerance has been attributed to a variety of effects, including effects on stomatal conductance, an increase in water use efficiency, reductions of the oxidative damage under drought stress, modifications in the contents of plant hormones, such as strigolactones, jasmonic acid, and abscisic acid, improvements in plant water status by effects on hydraulic conductivity, and the activation of functional proteins, such as aquaporins [95]. For example, the AM symbiosis induced strigolactone biosynthesis under drought conditions and conferred drought tolerance in lettuce and tomatoes [96, 97]. Using a two-compartment system, it has been estimated that fungal water transport from the hyphal compartment can account for more than 30% of the water transpired by AM host plants. In addition, AM fungal hyphae were able to transport water along hyphae outside of hyphal cell membranes [98]. It has also been suggested that AM fungi increase the water uptake of plants by their positive effect on the expression of plant aquaporins [99, 100]. Aquaporins are membrane proteins that facilitate the transport of water and small solutes following an osmotic gradient. In
4. Carbon transport in root symbioses
4.1 Carbon transport in the arbuscular mycorrhizal symbiosis
The fact that AM fungi are obligate biotrophs and cannot complete their life cycle without the carbon supply from their host and the observation that host plants suppress the AM colonization of their root system when nutrients are readily available has led to the overall assumption that the host plant is in control of the symbiosis [102]. However, this phytocentric view disregards the long co-evolution of both partners in the AM symbiosis (~450 million years) that allowed both partners to improve their bargaining power in the symbiosis and contributed to the evolutionary stability of mutualism in the AM symbiosis [103, 104]. In CMNs, in which multiple host plants are interconnected and share the same mycorrhizal network, AM fungi preferentially allocate nutrient resources to host plants that provide more carbon benefits [105]. The carbon supply of the host is an important trigger for nutrient uptake and transport by the AM fungus [74, 106, 107]. Similarly, host plants are simultaneously colonized by communities of AM fungi that compete with their nutrient benefits for carbon from the mycorrhizal host. Despite the fact that different AM fungi can colonize the same root on a very small spatial scale, host plants are able to distinguish between AM fungi and preferentially allocate carbon resources to AM fungi that provide higher nutrient benefits [103]. This requires that host plants can fine-tune their carbon flux to different AM fungi on a very small spatial scale and at each individual AM interface. However, our current understanding of these processes is still very limited, particularly considering that the host plant exchanges carbon with the fungus for a variety of AM benefits.
In plants, sugar transporters are classified into monosaccharide transporters (MSTs), sucrose uptake transporters (SUTs), and SWEETs (Sugars Will Eventually be Exported Transporters). Both MSTs and SUTs contain 12 transmembrane α-helices, while SWEETs are characterized by seven transmembrane domains [108]. Plant MSTs show high expression levels in AM roots, and it has been suggested that MSTs could play an important role in funneling host plant carbon to the mycorrhizal interface [108, 109]. For example, the promoter of the
While SUTs and monosaccharide transporters are symporters and require energy for the transmembrane transport of sugars, SWEETs are uniporters that can facilitate transmembrane transport in two directions and promote the diffusion of sugars along a concentration gradient. In soybeans, 52 different SWEET genes were identified [113]. Members of the SWEET transporter family show a distinct expression profile in plants and are involved in a variety of different physiological processes in plants, such as phloem transport, grain filling, floral transition, and the abiotic and biotic stress response of plants [114, 115]. In potato plants, the SWEETs
Based on earlier findings, glucose seemed to be the most likely form in which the fungus takes up carbon from the AM interface [121]. The increased activities of an apoplastic acid invertase and sucrose synthase in AM roots, which could facilitate the conversion of sucrose into the glucose and fructose in the interfacial apoplast or in the cortical cytoplasm, seemed to confirm this view [122]. This is also consistent with the expression of the fungal monosaccharide transporter
AM fungi store carbon mainly in the form of lipids, and here, in particular, in the form of triacylglycerol and fatty acids (FAs). It has long been assumed that AM fungi use plant-derived sugars as precursors for lipid biosynthesis, and that the fungus synthesizes FAs exclusively in the intraradical mycelium [124]. However, there is growing evidence that AM fungi are FA auxotrophs, and that the plant must transfer FAs to the fungus to sustain the AM symbiosis [125, 126]. In plants,
4.2 Carbon transport in the symbiosis of legumes and rhizobia
Biological nitrogen fixation (BNF) by rhizobia is an energetically costly process. At least 16 molecules of ATP and 8 low potential electrons are necessary to convert N2 into NH3 [135]. Plants must provide rhizobia with a constant flow of energy in the form of reduced carbon compounds to maintain BNF activity. Root nodules constitute only a small fraction of the total biomass of a legume plant, but they can consume more than 25% of the total photosynthates of the plant. Sucrose is the main transport sugar that is translocated through the phloem to root nodules and to the other sink organs of the plant. However, how carbon is funneled to the root nodules and how this process is regulated is still largely unknown. For example, the nodule-specific sucrose transporter
The symbiosome membrane (SYM) is the site of nutrient exchange between plants and rhizobia and is energized through the activities of H+-ATPases that pump protons into the symbiosome space and provide both the plant and bacteroids with the necessary proton motive force to take up nutrients from the symbiosome space [137]. Among 197 proteins that were identified in the SYM of soybeans, were proteins involved in metabolism, protein folding and degradation, membrane trafficking, and solute transport, such as putative transporters for sulfate, calcium, hydrogen ions, peptide/dicarboxylate, and nitrate [138]. Mutations that interfere with dicarboxylate transport across the SYM interrupt N2 fixation, and it has been suggested that C4-dicarboxylates are the primary carbon source for bacteroids in active root nodules. The SYM has a well-characterized dicarboxylate transport system (Dct) encoded by the three gene loci
Bacteroids transfer N primarily in the form of NH4+ to the plant but also secrete significant amounts of the amino acids aspartate and alanine [140]. NH3, the product of BNF, is either transferred via passive diffusion across the bacteroid membrane or through the nodulin 26 channel [141]. Nodulin 26 is a member of the aquaporin superfamily but also shows an ammonia permease activity that is favored over its aquaporin activity [141]. Due to the low pH in the symbiosome space, NH3 is protonated here to NH4+ and then taken up by the host via a cation channel that is permeable to NH4+ [142].
4.3 Regulation of nodulation and mycorrhizal colonization
Due to the high carbon costs of both root symbioses, plants are under high selective pressure to tightly control nodulation and AM colonization. N and P deficiency in plants stimulates the colonization of plants by rhizobial or AM fungal partners, while a high availability of N or P, or the inability of partners to provide benefits to the host plant, promotes the premature senescence of symbiotic organs [143, 144]. The interaction between the partners in the RL symbiosis is based on carbon-nitrogen trade-offs. Since the plant cannot determine the BNF efficiency of rhizobia during the recognition and root entry stages, the plant needs to sanction low-benefit rhizobia later [145, 146]. Legumes have control over the carbon supply and can influence the success of their symbiotic partners. In natural soils, non-fixing rhizobia strains are rare, but intermediate fixers are common. When the plant can choose between an intermediate fixer and a more effective strain, the plant will “sanction” the intermediate fixer by limiting its carbon supply, what results in smaller nodules with fewer viable bacteria. By contrast, when the only alternative is a non-fixing rhizobia strain, plants will not sanction intermediate fixers [147]. Environmental variation can help to explain why low- and high-benefit rhizobia still coexist. In an N-rich environment, the host might be less strict, thus allowing low-benefit strains to proliferate [148]. Low-benefit rhizobia might also be able to escape host plant sanctions by forming mixed nodules with high mutualistic rhizobia strains [149].
Arbuscules have only a short lifespan and are only functional for 2–3 days, before they become senescent and collapse [150]. This short life cycle seems like a waste of limited resources but allows plants to regulate their AM colonization. Plants can also induce a premature arbuscular degeneration (PAD) [84]. PAD has been discussed as one mechanism by which host plants can sanction low-benefit AM fungi or are able to reduce the AM colonization under high P conditions [79, 151]. Host plants can distinguish between high- and low-benefit AM fungi and allocate carbon resources accordingly [103, 130]. However, low-benefit AM fungi are able to persist in natural environments, and host plants tolerate the infection by low-benefit AM strains, to reduce their dependency on a single AM fungus for nutrient uptake.
However, plants not only control the colonization with low-benefit rhizobia but also limit nodule formation with high-benefit partners by the long-distance (systemic) autoregulation of nodulation (AON) pathway [152]. In response to rhizobial infection, a subset of genes encoding CLAVATA3/Embryo Surrounding Region (CLE) peptides are activated [153]. CLE peptides consist of 12–13 amino acids, secreted as signaling peptides from the C-terminal region of preproproteins. It has been reported that AON-related CLE peptides from the root negatively affect the number of nodules by inhibiting a leucine-rich repeat receptor-like-kinase (LRR-RLK) in the shoot, known as SUPER NUMERIC NODULES (
A prior AM colonization of one root half in a split-root system significantly reduces the AM colonization of the second root half, and there is evidence that the systemic autoregulation of mycorrhization (AOM) has similarities to the AON pathway [161, 162]. For example, hypernodulating mutants such as sunn, nark, har1, and sym29, also show a hypermycorrhizal colonization phenotype. However, whether other AON genes or mobile signals (CLE) are also involved in AOM is not yet known. However, the fact that prior nodulation in split-root studies can systemically suppress AM colonization and vice versa suggests that the same shoot-derived inhibitor is involved in AON and AOM.
5. Tripartite interactions of legumes
Our current understanding of the RL or AM symbiosis is mainly based on single plant/single symbiont studies, but field grown legumes form tripartite interactions, and are simultaneously colonized by both AM fungi and rhizobia [110, 163]. The inoculation with both root symbionts can lead to synergistic benefits, and plants can gain more from tripartite interactions than from single inoculations with either symbiont [163, 164, 165]. The rhizobial nitrogenase complex requires 16 ATP to fix one N2 molecule, and consequently rhizobia require an adequate P supply for efficient BNF. Nodules act as strong P sinks in legume root systems to provide sufficient P resources for optimum BNF [110, 166]. Nonmycorrhizal soybean plants have lower nodule numbers and weights and show particularly under low P supply lower N fixation rates [163, 167]. The positive effect of the AM symbiosis on the P uptake of the plant has therefore been discussed as the primary reason for the stimulation of BNF in AM legumes [163]. In addition, AM fungi can also supply the plant with other microelements that are essential for N2 fixation, including zinc, iron, manganese, and molybdenum [168, 169].
However, antagonistic responses have also been described, and the prior inoculation with either rhizobia or AM fungi can also suppress the root colonization by the other partner [170]. Whether the plant shows antagonistic or synergistic growth responses after dual inoculation depends on the environmental context [164], and the compatibility between symbiotic partners [165, 171]. As long as the root symbionts provide complementary rewards to the host plant, and the benefits outweigh the costs of these interactions, synergistic growth responses are more likely [172]. Rhizobia and AM fungi, however, are also competitors for the same resource from the host plant, and since both interactions are costly, the plant must be able to allocate carbon resources to both root symbionts according to their benefits. For example, an AM fungal partner is a stronger competitor for host plant carbon when it is able to provide N to the host, or when the plant is grown under high N but low P availabilities [110]. Our current understanding of the molecular mechanisms that control the carbon allocation from the host plant to individual root symbionts is very limited. Considering, the role that host plant carbon plays as an important trigger for symbiotic functioning, a better understanding of these processes is critical, because it may be key to improve the resource exchange between plants and symbionts and ultimately enhance productivity of agronomically important legumes [74, 105, 173, 174].
References
- 1.
Turner TR, James EK, Poole PS. The plant microbiome. Genome Biology. 2013; 14 :209. DOI: 10.1186/gb-2013-14-6-209 - 2.
Herridge DF, Peoples MB, Boddey RM. Global inputs of biological nitrogen fixation in agricultural systems. Plant and Soil. 2008; 311 :1-18. DOI: 10.1007/s11104-008-9668-3 - 3.
Smith SE, Read DJ. Mycorrhizal Symbiosis. 3rd ed. New York: Academic Press; 2008. p. 787. DOI: 10.1016/B978-0-12-370526-6.X5001-6 - 4.
Parniske M. Arbuscular mycorrhiza: The mother of plant root endosymbioses. Nature Reviews Microbiology. 2008; 6 :763-775. DOI: 10.1038/nrmicro1987 - 5.
Strullu-Derrien C, Selosse M-A, Kenrick P, Martin FM. The origin and evolution of mycorrhizal symbioses: From palaeomycology to phylogenomics. New Phytologist. 2018; 220 :1012-1030. DOI: 10.1111/nph.15076 - 6.
Wang B, Qiu Y-L. Phylogenetic distribution and evolution of mycorrhizae in land plants. Mycorrhiza. 2006; 16 :299-363. DOI: 10.1007/s00572-005-0033-6 - 7.
Ryan MH, Graham JH. Is there a role for arbuscular mycorrhizal fungi in production agriculture? Plant and Soil. 2002; 244 :263-271. DOI: 10.1023/A:1020207631893 - 8.
Cameron DD. Arbuscular mycorrhizal fungi as (agro)ecosystem engineers. Plant and Soil. 2010; 333 :1-5. DOI: 10.1007/s11104-010-0361-y - 9.
Smith SE, Jakobsen I, Grønlund M, Smith FA. Roles of arbuscular mycorrhizas in plant phosphorus nutrition: Interactions between pathways of phosphorus uptake in arbuscular mycorrhizal roots have important implications for understanding and manipulating plant phosphorus acquisition. Plant Physiology. 2011; 156 :1050-1057. DOI: 10.1104/pp.111.174581 - 10.
Smith SE, Smith FA, Jakobsen I. Functional diversity in arbuscular mycorrhizal (AM) symbioses: The contribution of the mycorrhizal P uptake pathway is not correlated with mycorrhizal responses in growth or total P uptake. New Phytologist. 2004; 162 :511-524. DOI: 10.1111/j.1469-8137.2004.01039.x - 11.
Babikova Z, Gilbert L, Bruce TJA, Birkett M, Caulfield JC, Woodcock C, et al. Underground signals carried through common mycelial networks warn neighbouring plants of aphid attack. Ecology Letters. 2013; 16 :835-843. DOI: 10.1111/ele.12115 - 12.
Gorzelak MA, Asay AK, Pickles BJ, Simard SW. Inter-plant communication through mycorrhizal networks mediates complex adaptive behaviour in plant communities. AoB Plants. 2015:plv050. DOI: 10.1093/aobpla/plv050 - 13.
Figueiredo A, Boy J, Guggenberger G. Common mycorrhizae network: A review of the theories and mechanisms behind underground interactions. Frontiers in Fungal Biology. 2021; 2 :735299. DOI: 10.3389/ffunb.2021.735299 - 14.
Akiyama K, Matsuzaki KI, Hayashi H. Plant sesquiterpenes induce hyphal branching in arbuscular mycorrhizal fungi. Nature. 2005; 435 :824-827. DOI: 10.1038/nature03608 - 15.
Besserer A, Puech-Pagès V, Kiefer P, Gomez-Roldan V, Jauneau A, Roy S, et al. Strigolactones stimulate arbuscular mycorrhizal fungi by activating mitochondria. PLOS Biology. 2006; 4 :1239-1247. DOI: 10.1371/journal.pbio.0040226 - 16.
Bücking H, Abubaker J, Govindarajulu M, Tala M, Pfeffer PE, Nagahashi G, et al. Root exudates stimulate the uptake and metabolism of organic carbon in germinating spores of Glomus intraradices . New Phytologist. 2008;180 :684-695. DOI: 10.1111/j.1469-8137.2008.02590.x - 17.
Mostofa MG, Li W, Nguyen KH, Fujita M, Tran L-SP. Strigolactones in plant adaptation to abiotic stresses: An emerging avenue of plant research. Plant, Cell & Environment. 2018; 41 :2227-2243. DOI: 10.1111/pce.13364 - 18.
Das D, Paries M, Hobecker K, Gigl M, Dawid C, Lam H-M, et al. Phosphate starvation response transcription factors enable arbuscular mycorrhiza symbiosis. Nature Communications. 2022; 13 :477. DOI: 10.1038/s41467-022-27976-8 - 19.
Genre A, Chabaud M, Timmers T, Bonfante P, Barker DG. Arbuscular mycorrhizal fungi elicit a novel intracellular apparatus in Medicago truncatula root epidermal cells before infection. Molecular Plant Microbe Interactions. 2005; 17 :3489-3499. DOI: 10.1105/tpc.105.035410 - 20.
Coronado C, Zuanazzi J, Sallaud C, Quirion JC, Esnault R, Husson HP, et al. Alfalfa root flavonoid production is nitrogen regulated. Plant Physiology. 1995; 108 :533-542. DOI: 10.1104/pp.108.2.533 - 21.
Giraud E, Moulin L, Vallenet D, Barbe V, Cytryn E, Avarre J-C, et al. Legumes symbioses: Absence of nod genes in photosynthetic Bradyrhizobia. Science. 2007;316 :1307-1312. DOI: 10.1126/science.1139548 - 22.
Madsen EB, Madsen LH, Radutoiu S, Olbryt M, Rakwalska M, Szczyglowski K, et al. A receptor kinase gene of the LysM type is involved in legume perception of rhizobial signals. Nature. 2003; 425 :637-640. DOI: 10.1038/nature02045 - 23.
Radutoiu S, Madsen LH, Madsen EB, Felle HH, Umehara Y, Grønlund M, et al. Plant recognition of symbiotic bacteria requires two LysM receptor-like kinases. Nature. 2003; 425 :585-592. DOI: 10.1038/nature02039 - 24.
Fisher RF, Long SR. Rhizobium–plant signal exchange. Nature. 1992; 357 :655-660. DOI: 10.1038/357655a0 - 25.
Liu C-W, Murray J. The role of flavonoids in nodulation host-range specificity: An update. Plants. 2016; 5 :33. DOI: 10.3390/plants5030033 - 26.
Wang Q , Yang S, Liu J, Terecskei K, Ábrahám E, Gombár A, et al. Host-secreted antimicrobial peptide enforces symbiotic selectivity in Medicago truncatula. Proceedings of the National Academy of Sciences, USA. 2017; 114 :6854-6859. DOI: 10.1073/pnas.1700715114 - 27.
Roy S, Liu W, Nandety RS, Crook A, Mysore KS, Pislariu CI, et al. Celebrating 20 years of genetic discoveries in legume nodulation and symbiotic nitrogen fixation. The Plant Cell. 2020; 32 :15-41. DOI: 10.1105/tpc.19.00279 - 28.
Downie JA. The roles of extracellular proteins, polysaccharides and signals in the interactions of rhizobia with legume roots. FEMS Microbiology Reviews. 2010; 34 :150-170. DOI: 10.1111/j.1574-6976.2009.00205.x - 29.
Truchet G, Roche P, Lerouge P, Vasse J, Camut S, de Billy F, et al. Sulphated lipo-oligosaccharide signals of Rhizobium meliloti elicit root nodule organogenesis in alfalfa. Nature. 1991;351 :670-673. DOI: 10.1038/351670a0 - 30.
Harris JM, Wais R, Long SR. Rhizobium-induced calcium spiking in Lotus japonicus . Molecular Plant Microbe Interactions. 2003;16 :335-341. DOI: 10.1094/MPMI.2003.16.4.335 - 31.
Popp C, Ott T. Regulation of signal transduction and bacterial infection during root nodule symbiosis. Current Opinion in Plant Biology. 2011; 14 :458-467. DOI: 10.1016/j.pbi.2011.03.016 - 32.
Udvardi MK, Day DA. Metabolite transport across symbiotic membranes of legume nodules. Annual Review of Plant Physiology and Plant Molecular Biology. 1997; 48 :493-523. DOI: 10.1146/annurev.arplant.48.1.493 - 33.
Maillet F, Poinsot V, André O, Puech-Pagès V, Haouy A, Gueunier M, et al. Fungal lipochitooligosaccharide symbiotic signals in arbuscular mycorrhiza. Nature. 2011; 469 :58-63. DOI: 10.1038/nature09622 - 34.
Sprent JI. Evolving ideas of legume evolution and diversity: A taxonomic perspective on the occurrence of nodulation. New Phytologist. 2007; 174 :11-25. DOI: 10.1111/j.1469-8137.2007.02015.x - 35.
Brundrett MC, Tedersoo L. Evolutionary history of mycorrhizal symbioses and global host plant diversity. New Phytologist. 2018; 220 :1108-1115. DOI: 10.1111/nph.14976 - 36.
Cope KR, Bascaules A, Irving TB, Venkateshwaran M, Maeda J, Garcia K, et al. The ectomycorrhizal fungus Laccaria bicolor produces lipochitooligosaccharides and uses the common symbiosis pathway to colonizePopulus roots. The Plant Cell. 2019;31 :2386-2410. DOI: 10.1105/tpc.18.00676 - 37.
Kistner C, Winzer T, Pitzschke A, Mulder L, Sato S, Kaneko T, et al. Seven Lotus japonicus genes required for transcriptional reprogramming of the root during fungal and bacterial symbiosis. The Plant Cell. 2005;17 :2217-2229. DOI: 10.1105/tpc.105.032714 - 38.
Broghammer A, Krusell L, Blaise M, Sauer J, Sullivan JT, Maolanon N, et al. Legume receptors perceive the rhizobial lipochitin oligosaccharide signal molecules by direct binding. Proceedings of the National Academy of Sciences USA. 2012; 109 :13859-13864. DOI: 10.1073/pnas.1205171109 - 39.
Moling S, Pietraszewska-Bogiel A, Postma M, Fedorova E, Hink MA, Limpens E, et al. Nod factor receptors form heteromeric complexes and are essential for intracellular infection in Medicago nodules. The Plant Cell. 2014;26 :4188-4199. DOI: 10.1105/tpc.114.129502 - 40.
He J, Zhang C, Dai H, Liu H, Zhang X, Yang J, et al. A LysM receptor heteromer mediates perception of arbuscular mycorrhizal symbiotic signal in rice. Molecular Plant. 2019; 12 :1561-1576. DOI: 10.1016/j.molp.2019.10.015 - 41.
Miyata K, Kozaki T, Kouzai Y, Ozawa K, Ishii K, Asamizu E, et al. The bifunctional plant receptor, OsCERK1, regulates both chitin-triggered immunity and arbuscular mycorrhizal symbiosis in rice. Plant Cell Physiology. 2014; 55 :1864-1872. DOI: 10.1093/pcp/pcu129 - 42.
Antolín-Llovera M, Ried Martina K, Parniske M. Cleavage of the SYMBIOSIS RECEPTOR-LIKE KINASE ectodomain promotes complex formation with nod factor receptor 5. Current Biology. 2014; 24 :422-427. DOI: 10.1016/j.cub.2013.12.053 - 43.
Feng Y, Wu P, Liu C, Peng L, Wang T, Wang C, et al. Suppression of LjBAK1-mediated immunity by SymRK promotes rhizobial infection in Lotus japonicus . Molecular Plant. 2021;14 :1935-1950. DOI: 10.1016/j.molp.2021.07.016 - 44.
Charpentier M, Bredemeier R, Wanner G, Takeda N, Schleiff E, Parniske M. Lotus japonicus CASTOR and POLLUX are ion channels essential for perinuclear calcium spiking in legume root endosymbiosis. The Plant Cell. 2008;20 :3467-3479. DOI: 10.1105/tpc.108.063255 - 45.
Chen C, Fan C, Gao M, Zhu H. Antiquity and function of CASTOR and POLLUX, the twin ion channel-encoding genes key to the evolution of root symbioses in plants. Plant Physiology. 2008; 149 :306-317. DOI: 10.1104/pp.108.131540 - 46.
Groth M, Takeda N, Perry J, Uchida H, Dräxl S, Brachmann A, et al. NENA, a Lotus japonicus homolog of Sec13, is required for rhizodermal infection by arbuscular mycorrhiza fungi and rhizobia but dispensable for cortical endosymbiotic development. The Plant Cell. 2010;22 :2509-2526. DOI: 10.1105/tpc.109.069807 - 47.
Kanamori N, Madsen LH, Radutoiu S, Frantescu M, Quistgaard EMH, Miwa H, et al. A nucleoporin is required for induction of Ca2+ spiking in legume nodule development and essential for rhizobial and fungal symbiosis. Proceedings of the National Academy of Sciences, USA. 2006; 103 :359-364. DOI: 10.1073/pnas.0508883103 - 48.
Singh S, Parniske M. Activation of calcium- and calmodulin-dependent protein kinase (CCaMK), the central regulator of plant root endosymbiosis. Current Opinion in Plant Biology. 2012; 15 :444-453. DOI: 10.1016/j.pbi.2012.04.002 - 49.
Singh S, Katzer K, Lambert J, Cerri M, Parniske M. CYCLOPS, a DNA-binding transcriptional activator, orchestrates symbiotic root nodule development. Cell Host & Microbe. 2014; 15 :139-152. DOI: 10.1016/j.chom.2014.01.011 - 50.
Gutjahr C, Parniske M. Cell and developmental biology of arbuscular mycorrhiza symbiosis. Annual Review in Cell Developmental Biology. 2013; 29 :593-617. DOI: 10.1146/annurev-cellbio-101512-122413 - 51.
Pimprikar P, Carbonnel S, Paries M, Katzer K, Klingl V, Bohmer Monica J, et al. A CCaMK-CYCLOPS-DELLA complex activates transcription of RAM1 to regulate arbuscule branching. Current Biology. 2016; 26 :987-998. DOI: 10.1016/j.cub.2016.01.069 - 52.
Yu N, Luo D, Zhang X, Liu J, Wang W, Jin Y, et al. A DELLA protein complex controls the arbuscular mycorrhizal symbiosis in plants. Cell Research. 2014; 24 :130-133. DOI: 10.1038/cr.2013.167 - 53.
Marsh JF, Rakocevic A, Mitra RM, Brocard L, Sun J, Eschstruth A, et al. Medicago truncatula NIN is essential for rhizobial-independent nodule organogenesis induced by autoactive calcium/calmodulin-dependent protein kinase. Plant Physiology. 2007;144 :324-335. DOI: 10.1104/pp.106.093021 - 54.
Andriankaja A, Boisson-Dernier A, Frances L, Sauviac L, Jauneau A, Barker DG, et al. AP2-ERF transcription factors mediate nod factor dependent Mt ENOD11 activation in root hairs via a novel cis-regulatory motif. The Plant Cell. 2007; 19 :2866-2885. DOI: 10.1105/tpc.107.052944 - 55.
Kaló P, Gleason C, Edwards A, Marsh J, Mitra RM, Hirsch S, et al. Nodulation signaling in legumes requires NSP2, a member of the GRAS family of transcriptional regulators. Science. 2005; 308 :1786-1789. DOI: 10.1126/science.1110951 - 56.
Smit P, Raedts J, Portyanko V, Debelle F, Gough C, Bisseling T, et al. NSP1 of the GRAS protein family is essential for rhizobial nod factor-induced transcription. Science. 2005; 308 :1789-1791. DOI: 10.1126/science.1111025 - 57.
Jin Y, Liu H, Luo D, Yu N, Dong W, Wang C, et al. DELLA proteins are common components of symbiotic rhizobial and mycorrhizal signalling pathways. Nature Communications. 2016; 7 :12433. DOI: 10.1038/ncomms12433 - 58.
Hirsch S, Kim J, Muñoz A, Heckmann AB, Downie JA, Oldroyd GE. GRAS proteins form a DNA binding complex to induce gene expression during nodulation signaling in Medicago truncatula . The Plant Cell. 2009;21 :545-557. DOI: 10.1105/tpc.108.064501 - 59.
Schachtman DP, Reid RJ, Ayling SM. Phosphorus uptake by plants: From soil to cell. Plant Physiology. 1998; 116 :447-453. DOI: 10.1104/pp.116.2.447 - 60.
Bucher M. Functional biology of plant phosphate uptake at root and mycorrhiza interfaces. New Phytologist. 2007; 173 :11-26. DOI: 10.1111/j.1469-8137.2006.01935.x - 61.
Paszkowski U, Kroken S, Roux C, Briggs SP. Rice phosphate transporters include an evolutionarily divergent gene specifically activated in arbuscular mycorrhizal symbiosis. Proceedings of the National Academy of Sciences, USA. 2002; 99 :13324-13329. DOI: 10.1073/pnas.202474599 - 62.
Volpe V, Giovannetti M, Sun X-G, Fiorilli V, Bonfante P. The phosphate transporters LjPT4 and MtPT4 mediate early root responses to phosphate status in non mycorrhizal roots. Plant, Cell & Environment. 2016; 39 :660-671. DOI: 10.1111/pce.12659 - 63.
Harrison MJ, Dewbre GR, Liu J. A phosphate transporter from Medicago truncatula involved in the acquisition of phosphate released by arbuscular mycorrhizal fungi. The Plant Cell. 2002;14 :2413-2429. DOI: 10.1105/tpc.004861 - 64.
Yang S-Y, Grønlund M, Jakobsen I, Grotemeyer MS, Rentsch D, Miyao A, et al. Nonredundant regulation of rice arbuscular mycorrhizal symbiosis by two members of the PHOSPHATE TRANSPORTER1 gene family. The Plant Cell. 2012; 24 :4236-4251. DOI: 10.1105/tpc.112.104901 - 65.
Xie XA, Huang W, Liu FC, Tang NW, Liu Y, Lin H, et al. Functional analysis of the novel mycorrhiza-specific phosphate transporter AsPT1 and PHT1 family from Astragalus sinicus during the arbuscular mycorrhizal symbiosis. New Phytologist. 2013;198 :836-852. DOI: 10.1111/nph.12188 - 66.
Hawkesford MJ, Cakmak I, Coskun D, De Kok LJ, Lambers H, Schjoerring JK, et al. Chapter 6 - functions of macronutrients. In: Rengel Z, Cakmak I, White PJ, editors. Marschner's Mineral Nutrition of Plants. San Diego: Academic Press; 2023. pp. 201-281 - 67.
Bloom AJ. The increasing importance of distinguishing among plant nitrogen sources. Current Opinion in Plant Biology. 2015; 25 :10-16. DOI: 10.1016/j.pbi.2015.03.002 - 68.
Miller AJ, Cramer MD. Root nitrogen acquisition and assimilation. Plant and Soil. 2004; 274 :1-36. DOI: 10.1007/s11104-004-0965-1 - 69.
Kuzyakov Y, Xu X. Competition between roots and microorganisms for nitrogen: Mechanisms and ecological relevance. New Phytologist. 2013; 198 :656-669. DOI: 10.1111/nph.12235 - 70.
Rengel Z, Cakmak I, White PJ. Marschner's Mineral Nutrition of Plants. San Diego: Academic Press; 2023. p. 795p - 71.
Bücking H, Kafle A. Role of arbuscular mycorrhizal fungi in the nitrogen uptake of plants: Current knowledge and research gaps. Agronomy. 2015; 5 :587-612. DOI: 10.3390/agronomy5040587 - 72.
Pérez-Tienda J, Valderas A, Camañes G, García-Agustín P, Ferrol N. Kinetics of NH4+ uptake by the arbuscular mycorrhizal fungus Rhizophagus irregularis . Mycorrhiza. 2012;22 :485-491. DOI: 10.1007/s00572-012-0452-0 - 73.
Tian C, Kasiborski B, Koul R, Lammers PJ, Bücking H, Shachar-Hill Y. Regulation of the nitrogen transfer pathway in the arbuscular mycorrhizal symbiosis: Gene characterization and the coordination of expression with nitrogen flux. Plant Physiology. 2010; 153 :1175-1187. DOI: 10.1104/pp.110.156430 - 74.
Fellbaum CR, Gachomo EW, Beesetty Y, Choudhari S, Strahan GD, Pfeffer PE, et al. Carbon availability triggers fungal nitrogen uptake and transport in the arbuscular mycorrhizal symbiosis. Proceedings of the National Academy of Sciences, USA. 2012; 109 :2666-2671. DOI: 10.1073/pnas.1118650109 - 75.
Cooper TG, Sumrada RA. What is the function of nitrogen catabolite repression in Saccharomyces cerevisiae ? Journal of Bacteriology. 1983;155 :623-627. DOI: 10.1128/jb.155.2.623-627.1983 - 76.
Smith SE, Smith FA. Roles of arbuscular mycorrhizas in plant nutrition and growth: New paradigms from cellular to ecosystem scales. Annual Review Plant Biology. 2011; 62 :227-250. DOI: 10.1146/annurev-arplant-042110-103846 - 77.
Mensah JA, Koch AM, Antunes PM, Hart MM, Kiers ET, Bücking H. High functional diversity within arbuscular mycorrhizal fungal species is associated with differences in phosphate and nitrogen uptake and fungal phosphate metabolism. Mycorrhiza. 2015; 25 :533-546. DOI: 10.1007/s00572-015-0631-x - 78.
Javot H, Penmetsa RV, Terzaghi N, Cook DR, Harrison MJ. A Medicago truncatula phosphate transporter indispensable for the arbuscular mycorrhizal symbiosis. Proceedings of the National Academy of Sciences, USA. 2007;104 :1720-1725. DOI: 10.1073/pnas.060813610 - 79.
Javot H, Penmetsa RV, Breuillin F, Bhattarai KK, Noar RD, Gomez SK, et al. Medicago truncatula Mtpt4 mutants reveal a role for nitrogen in the regulation of arbuscule degeneration in arbuscular mycorrhizal symbiosis. Plant Journal. 2011;68 :954-965. DOI: 10.1111/j.1365-313X.2011.04746.x - 80.
Govindarajulu M, Pfeffer PE, Jin HR, Abubaker J, Douds DD, Allen JW. Nitrogen transfer in the arbuscular mycorrhizal symbiosis. Nature. 2005; 435 :819-823. DOI: 10.1038/nature03610 - 81.
Kobae Y, Tamura Y, Takai S, Banba M, Hata S. Localized expression of arbuscular mycorrhiza-inducible ammonium transporters in soybean. Plant and Cell Physiology. 2010; 51 :1411-1415. DOI: 10.1093/pcp/pcq099 - 82.
Koegel S, Lahmidi NA, Arnould C, Chatagnier O, Walder F, Ineichen K, et al. The family of ammonium transporters (AMT) in Sorghum bicolor : Two AMT members are induced locally, but not systemically in roots colonized by arbuscular mycorrhizal fungi. New Phytologist. 2013;198 :853-865. DOI: 10.1111/nph.12199 - 83.
Guether M, Neuhauser B, Balestrini R, Dynowski M, Ludewig U, Bonfante P. A mycorrhizal-specific ammonium transporter from Lotus japonicus acquires nitrogen released by arbuscular mycorrhizal fungi. Plant Physiology. 2009;150 :73-83. DOI: 10.1104/pp.109.136390 - 84.
Breuillin-Sessoms F, Floss DS, Gomez SK, Pumplin N, Ding Y, Levesque-Tremblay V, et al. Suppression of arbuscule degeneration in Medicago truncatula phosphate transporter 4 mutants is dependent on the ammonium transporter 2 family protein AMT2;3. The Plant Cell. 2015;27 :1352-1366. DOI: 10.1105/tpc.114.131144 - 85.
Hui J, An X, Li Z, Neuhäuser B, Ludewig U, Wu X, et al. The mycorrhiza-specific ammonium transporter ZmAMT3;1 mediates mycorrhiza-dependent nitrogen uptake in maize roots. The Plant Cell. 2022; 34 :4066-4087. DOI: 10.1093/plcell/koac225 - 86.
Wang S, Chen A, Xie K, Yang X, Luo Z, Chen J, et al. Functional analysis of the OsNPF4.5 nitrate transporter reveals a conserved mycorrhizal pathway of nitrogen acquisition in plants. Proceedings of the National Academy of Science, USA. 2020; 117 :16649-16659. DOI: 10.1073/pnas.2000926117 - 87.
Guether M, Volpe V, Balestrini R, Requena N, Wipf D, Bonfante P. LjLHT1.2 - a mycorrhiza-inducible plant amino acid transporter from Lotus japonicus . Biology and Fertility of Soils. 2011;47 :925-936. DOI: 10.1007/s00374-011-0596-7 - 88.
Ragel P, Raddatz N, Leidi EO, Quintero FJ, Pardo JM. Regulation of K+ nutrition in plants. Frontiers in Plant Science. 2019; 2019 :10. DOI: 10.3389/fpls.2019.00281 - 89.
Garcia K, Ané J-M. Polymorphic responses of Medicago truncatula accessions to potassium deprivation. Plant Signaling & Behavior. 2017;12 :e1307494. DOI: 10.1080/15592324.2017.1307494 - 90.
Garcia K, Chasman D, Roy S, Ané J-M. Physiological responses and gene co-expression network of mycorrhizal roots under K deprivation. Plant Physiology. 2017; 173 :1811-1823. DOI: 10.1104/pp.16.01959 - 91.
Padmanaban S, Chanroj S, Kwak JM, Li X, Ward JM, Sze H. Participation of endomembrane cation/H+ exchanger AtCHX20 in osmoregulation of guard cells. Plant Physiology. 2007; 144 :82-93. DOI: 10.1104/pp.106.092155 - 92.
Guether M, Balestrini R, Hannah M, He J, Udvardi MK, Bonfante P. Genome-wide reprogramming of regulatory networks, transport, cell wall and membrane biogenesis during arbuscular mycorrhizal symbiosis in Lotus japonicus . New Phytologist. 2009;182 :200-212. DOI: 10.1111/j.1469-8137.2008.02725.x - 93.
Liu J, Liu J, Liu J, Cui M, Huang Y, Tian Y, et al. The potassium transporter SlHAK10 is involved in mycorrhizal potassium uptake. Plant Physiology. 2019; 180 :465-479. DOI: 10.1104/pp.18.01533 - 94.
Augé RM. Water relations, drought and vesicular-arbuscular mycorrhizal symbiosis. Mycorrhiza. 2001; 11 :3-42. DOI: 10.1007/s005720100097 - 95.
Bahadur A, Batool A, Nasir F, Jiang S, Mingsen Q , Zhang Q , et al. Mechanistic insights into arbuscular mycorrhizal fungi-mediated drought stress tolerance in plants. International Journal of Molecular Sciences. 2019; 20 :4199. DOI: 10.3390/ijms20174199 - 96.
Ruiz-Lozano JM, Aroca R, Zamarreño ÁM, Molina S, Andreo-Jiménez B, Porcel R, et al. Arbuscular mycorrhizal symbiosis induces strigolactone biosynthesis under drought and improves drought tolerance in lettuce and tomato. Plant, Cell & Environment. 2016; 39 :441-452. DOI: 10.1111/pce.12631 - 97.
Visentin I, Vitali M, Ferrero M, Zhang Y, Ruyter-Spira C, Novák O, et al. Low levels of strigolactones in roots as a component of the systemic signal of drought stress in tomato. New Phytologist. 2016; 212 (4):954-963. DOI: 10.1111/nph.14190 - 98.
Kakouridis A, Hagen JA, Kan MP, Mambelli S, Feldman LJ, Herman DJ, et al. Routes to roots: Direct evidence of water transport by arbuscular mycorrhizal fungi to host plants. New Phytologist. 2022; 236 :210-221. DOI: 10.1111/nph.18281 - 99.
Quiroga G, Erice G, Ding L, Chaumont F, Aroca R, Ruiz-Lozano JM. The arbuscular mycorrhizal symbiosis regulates aquaporins activity and improves root cell water permeability in maize plants subjected to water stress. Plant, Cell & Environment. 2019; 42 :2274-2290. DOI: 10.1111/pce.13551 - 100.
Ruiz-Lozano JM, del Mar AM, Bárzana G, Vernieri P, Aroca R. Exogenous ABA accentuates the differences in root hydraulic properties between mycorrhizal and non mycorrhizal maize plants through regulation of PIP aquaporins. Plant Molecular Biology. 2009; 70 :565-579. DOI: 10.1007/s11103-009-9492-z - 101.
Giovannetti M, Balestrini R, Volpe V, Guether M, Straub D, Costa A, et al. Two putative-aquaporin genes are differentially expressed during arbuscular mycorrhizal symbiosis in Lotus japonicus . BMC Plant Biology. 2012;12 :14. DOI: 10.1186/1471-2229-12-186 - 102.
Smith SE, Smith FA. Fresh perspectives on the roles of arbuscular mycorrhizal fungi in plant nutrition and growth. Mycologia. 2012; 104 :1-13. DOI: 10.3852/11-229 - 103.
Kiers ET, Duhamel M, Beesetty Y, Mensah JA, Franken O, Verbruggen E, et al. Reciprocal rewards stabilize cooperation in the mycorrhizal symbiosis. Science. 2011; 333 :880-882. DOI: 10.1126/science.1208473 - 104.
Bücking H, Mensah JA, Fellbaum CR. Common mycorrhizal networks and their effect on the bargaining power of the fungal partner in the arbuscular mycorrhizal symbiosis. Communicative & Integrative Biology. 2016; 9 :e1107684. DOI: 10.1080/19420889.2015.1107684 - 105.
Fellbaum CR, Mensah JA, Cloos AJ, Strahan GD, Pfeffer PE, Kiers ET, et al. Fungal nutrient allocation in common mycelia networks is regulated by the carbon source strength of individual host plants. New Phytologist. 2014; 203 :645-656. DOI: 10.1111/nph.12827 - 106.
Bücking H, Shachar-Hill Y. Phosphate uptake, transport and transfer by the arbuscular mycorrhizal fungus Glomus intraradices is stimulated by increased carbohydrate availability. New Phytologist. 2005;165 :899-912. DOI: 10.1111/j.1469-8137.2004.01274.x - 107.
Hammer EC, Pallon J, Wallander H, Olsson PA. Tit for tat? A mycorrhizal fungus accumulates phosphorus under low plant carbon availability. FEMS Microbiology Ecology. 2011; 76 :236-244. DOI: 10.1111/j.1574-6941.2011.01043.x - 108.
Harrison MJ. A sugar transporter from Medicago truncatula : Altered expression pattern in roots during vesicular-arbuscular (VA) mycorrhizal associations. The Plant Journal. 1996;9 :491-503. DOI: 10.1046/j.1365-313x.1996.09040491.x - 109.
Gaude N, Bortfeld S, Duensing N, Lohse M, Krajinski F. Arbuscule-containing and non-colonized cortical cells of mycorrhizal roots undergo extensive and specific reprogramming during arbuscular mycorrhizal development. Plant Journal. 2012; 69 :510-528. DOI: 10.1111/j.1365-313X.2011.04810.x - 110.
Kafle A, Garcia K, Wang X, Pfeffer PE, Strahan GD, Bücking H. Nutrient demand and fungal access to resources control the carbon allocation to the symbiotic partners in tripartite interactions of Medicago truncatula . Plant, Cell & Environment. 2019;42 :270-284. DOI: 10.1111/pce.13359 - 111.
Gabriel-Neumann E, Neumann G, Leggewie G, George E. Constitutive overexpression of the sucrose transporter SoSUT1 in potato plants increases arbucular mycorrhiza fungal root colonization under high, but not under low, soil phosphorus availability. Journal of Plant Physiology. 2011; 168 :911-919. DOI: 10.1016/j.jplph.2010.11.026 - 112.
Bitterlich M, Krügel U, Boldt-Burisch K, Franken P, Kühn C. The sucrose transporter SlSUT2 from tomato interacts with brassinosteroid functioning and affects arbuscular mycorrhiza formation. Plant Journal. 2014; 78 :877-889. DOI: 10.1111/tpj.12515 - 113.
Patil G, Valliyodan B, Deshmukh R, Prince S, Nicander B, Zhao M, et al. Soybean ( Glycine max ) SWEET gene family: Insights through comparative genomics, transcriptome profiling and whole genome re-sequence analysis. BMC Genomics. 2015;16 :520. DOI: 10.1186/s12864-015-1730-y - 114.
Gautam T, Dutta M, Jaiswal V, Zinta G, Gahlaut V, Kumar S. Emerging roles of SWEET sugar transporters in plant development and abiotic stress response. Cell. 2022; 11 :1303. DOI: 10.3390/cells11081303 - 115.
Ji J, Yang L, Fang Z, Zhang Y, Zhuang M, Lv H, et al. Plant SWEET family of sugar transporters: Structure, evolution and biological functions. Biomolecules. 2022; 12 :205. DOI: 10.3390/biom12020205 - 116.
Manck-Götzenberger J, Requena N. Arbuscular mycorrhiza symbiosis induces a major transcriptional reprogramming of the potato SWEET sugar transporter family. Frontiers in Plant Science. 2016; 2016 :7. DOI: 10.3389/fpls.2016.00487 - 117.
Tamayo E, Figueira-Galán D, Manck-Götzenberger J, Requena N. Overexpression of the potato monosaccharide trransporter StSWEET7a promotes root colonization by symbiotic and pathogenic fungi by increasing root sink strength. Frontiers in Plant Science. 2022;2022 :13. DOI: 10.3389/fpls.2022.837231 - 118.
Kryvoruchko IS, Sinharoy S, Torres-Jerez I, Sosso D, Pislariu CI, Guan D, et al. MtSWEET11, a nodule-specific sucrose transporter of Medicago truncatula . Plant Physiology. 2016;171 :554-565. DOI: 10.1104/pp.15.01910 - 119.
Sugiyama A, Saida Y, Yoshimizu M, Takanashi K, Sosso D, Frommer WB, et al. Molecular characterization of LjSWEET3, a sugar transporter in nodules of Lotus japonicus . Plant and Cell Physiology. 2016;58 :298-306. DOI: 10.1093/pcp/pcw190 - 120.
An J, Zeng T, Ji C, de Graaf S, Zheng Z, Xiao TT, et al. A Medicago truncatula SWEET transporter implicated in arbuscule maintenance during arbuscular mycorrhizal symbiosis. New Phytologist. 2019;224 :396-408. DOI: 10.1111/nph.15975 - 121.
Pfeffer PE, Douds DD, Bécard G, Shachar-Hill Y. Carbon uptake and the metabolism and transport of lipids in an arbuscular mycorrhiza. Plant Physiology. 1999; 120 :587-598. DOI: 10.1104/pp.120.2.587 - 122.
Schaarschmidt S, Kopka J, Ludwig-Müller J, Hause B. Regulation of arbuscular mycorrhization by apoplastic invertases: Enhanced invertase activity in the leaf apoplast affects the symbiotic interaction. Plant Journal. 2007; 51 :390-405. DOI: 10.1111/j.1365-313X.2007.03150.x - 123.
Helber N, Wippel K, Sauer N, Schaarschmidt S, Hause B, Requena N. A versatile monosaccharide transporter that operates in the arbuscular mycorrhizal fungus Glomus sp. is crucial for the symbiotic relationship with plants. The Plant Cell. 2011;23 :3812-3823. DOI: 10.1105/tpc.111.089813 - 124.
Trépanier M, Bécard G, Moutoglis P, Willemot C, Gagné S, Avis TJ, et al. Dependence of arbuscular-mycorrhizal fungi on their plant host for palmitic acid synthesis. Applied and Environmental Microbiology. 2005; 71 :5341-5347. DOI: 10.1128/aem.71.9.5341-5347.2005 - 125.
Luginbuehl LH, Menard GN, Kurup S, van Erp H, Radhakrishnan G, Breakspear A, et al. Fatty acids in arbuscular mycorrhizal fungi are synthesized by the host plant. Science. 2017; 356 :1175-1178. DOI: 10.1126/science.aan0081 - 126.
Keymer A, Pimprikar P, Wewer V, Huber C, Brands M, Bucerius SL, et al. Lipid transfer from plants to arbuscular mycorrhiza fungi. eLife. 2017; 6 :e29107. DOI: 10.7554/eLife.29107 - 127.
Bravo A, York T, Pumplin N, Mueller LA, Harrison MJ. Genes conserved for arbuscular mycorrhizal symbiosis identified through phylogenomics. Nature Plants. 2016; 2 :15208. DOI: 10.1038/nplants.2015.208 - 128.
Wang E, Schornack S, Marsh JF, Gobbato E, Schwessinger B, Eastmond PJ, et al. A common signaling process that promotes mycorrhizal and oomycete colonization in plants. Current Biology. 2012; 22 :2242-2246. DOI: 10.1016/j.cub.2012.09.043 - 129.
Bravo A, Brands M, Wewer V, Dörmann P, Harrison MJ. Arbuscular mycorrhiza-specific enzymes FatM and RAM2 fine-tune lipid biosynthesis to promote development of arbuscular mycorrhiza. New Phytologist. 2017; 214 :1631-1645. DOI: 10.1111/nph.14533 - 130.
Cope KR, Kafle A, Yakha JK, Pfeffer PE, Strahan GD, Garcia K, et al. Physiological and transcriptomic response of Medicago truncatula to colonization by high- or low-benefit arbuscular mycorrhizal fungi. Mycorrhiza. 2022;32 :281-303. DOI: 10.1007/s00572-022-01077-2 - 131.
Banasiak J, Jamruszka T, Murray JD, Jasiński M. A roadmap of plant membrane transporters in arbuscular mycorrhizal and legume–rhizobium symbioses. Plant Physiology. 2021; 187 :2071-2091. DOI: 10.1093/plphys/kiab280 - 132.
Zhang Q , Blaylock LA, Harrison MJ. Two Medicago truncatula half-ABC transporters are essential for arbuscule development in arbuscular mycorrhizal symbiosis. The Plant Cell. 2010;22 :1483-1497. DOI: 10.1105/tpc.110.074955 - 133.
Radhakrishnan GV, Keller J, Rich MK, Vernié T, Mbadinga Mbadinga DL, Vigneron N, et al. An ancestral signalling pathway is conserved in intracellular symbioses-forming plant lineages. Nature Plants. 2020; 6 :280-289. DOI: 10.1038/s41477-020-0613-7 - 134.
Hogekamp C, Arndt D, Pereira PA, Becker JD, Hohnjec N, Kuster H. Laser microdissection unravels cell-type-specific transcription in arbuscular mycorrhizal roots, including CAAT-box transcription factor gene expression correlating with fungal contact and spread. Plant Physiology. 2011; 157 :2023-2043. DOI: 10.1104/pp.111.186635 - 135.
Kafle A, Garcia K, Peta V, Yakha JK, Soupir A, Bücking H. Beneficial plant microbe interactions and their effect on nutrient uptake, yield, and stress resistance of soybeans. In: Kasai M, editor. Soybean: Biomass, Yield and Productivity. London: Intechopen; 2018. DOI: 10.5772/intechopen.81396 - 136.
Deng L, Zhao S, Yang G, Zhu S, Tian J, Wang X. Soybean GmSUT1 transporter participates in sucrose transport to nodules during rhizobial symbiosis. Plant Growth Regulation. 2022; 96 :119-129. DOI: 10.1007/s10725-021-00764-y - 137.
Catalano CM, Lane WS, Sherrier DJ. Biochemical characterization of symbiosome membrane proteins from Medicago truncatula root nodules. Electrophoresis. 2004;25 :519-531. DOI: 10.1002/elps.200305711 - 138.
Clarke VC, Loughlin PC, Gavrin A, Chen C, Brear EM, Day DA, et al. Proteomic analysis of the soybean symbiosome identifies new symbiotic proteins. Molecular Cell Proteomics. 2015; 14 :1301-1322. DOI: 10.1074/mcp.M114.043166 - 139.
Yurgel SN, Kahn ML. Dicarboxylate transport by rhizobia. FEMS Microbiology Reviews. 2004; 28 :489-501. DOI: 10.1016/j.femsre.2004.04.002 - 140.
White J, Prell J, James EK, Poole P. Nutrient sharing between symbionts. Plant Physiology. 2007; 144 :604-614. DOI: 10.1104/pp.107.097741 - 141.
Hwang JH, Ellingson SR, Roberts DM. Ammonia permeability of the soybean nodulin 26 channel. FEBS Letters. 2010; 584 :4339-4343. DOI: 10.1016/j.febslet.2010.09.033 - 142.
Schwember AR, Schulze J, Del Pozo A, Cabeza RA. Regulation of symbiotic nitrogen fixation in legume root nodules. Plants (Basel). 2019; 8 :333. DOI: 10.3390/plants8090333 - 143.
Lambert I, Pervent M, Le Queré A, Clément G, Tauzin M, Severac D, et al. Responses of mature symbiotic nodules to the whole-plant systemic nitrogen signaling. Journal of Experimental Botany. 2020; 71 :5039-5052. DOI: 10.1093/jxb/eraa221 - 144.
Luginbuehl LH, Oldroyd GED. Understanding the arbuscule at the heart of endomycorrhizal symbioses in plants. Current Biology. 2017; 27 :R952-R963. DOI: 10.1016/j.cub.2017.06.042 - 145.
Westhoek A, Field E, Rehling F, Mulley G, Webb I, Poole PS, et al. Policing the legume-rhizobium symbiosis: A critical test of partner choice. Scientific Reports. 2017; 7 :1419. DOI: 10.1038/s41598-017-01634-2 - 146.
Kiers ET, Rousseau RA, West SA, Denison RF. Host sanctions and the legume-rhizobium mutualism. Nature. 2008; 425 :78-81. DOI: 10.1038/nature01931 - 147.
Westhoek A, Clark LJ, Culbert M, Dalchau N, Griffiths M, Jorrin B, et al. Conditional sanctioning in a legume-rhizobium mutualism. Proceedings of the National Academy of Sciences, USA. 2021; 2021 :118. DOI: 10.1073/pnas.2025760118 - 148.
Vuong HB, Thrall PH, Barrett LG. Host species and environmental variation can influence rhizobial community composition. Journal of Ecology. 2017; 105 :540-548. DOI: 10.1111/1365-2745.12687 - 149.
Checcucci A, Azzarello E, Bazzicalupo M, Galardini M, Lagomarsino A, Mancuso S, et al. Mixed nodule infection in Sinorhizobium meliloti–Medicago sativa symbiosis suggest the presence of cheating behavior. Frontiers in Plant Science. 2016;2016 :7. DOI: 10.3389/fpls.2016.00835 - 150.
Kobae Y, Hata S. Dynamics of periarbuscular membranes visualized with a fluorescent phosphate transporter in arbuscular mycorrhizal roots of rice. Plant and Cell Physiology. 2010; 51 :341-353. DOI: 10.1093/pcp/pcq013 - 151.
Breuillin F, Schramm J, Hajirezaei M, Ahkami A, Favre P, Druege U, et al. Phosphate systemically inhibits development of arbuscular mycorrhiza in Petunia hybrida and represses genes involved in mycorrhizal functioning. Plant Journal. 2010;64 :1002-1017. DOI: 10.1111/j.1365-313X.2010.04385.x - 152.
Suzaki T, Nishida H. Autoregulation of legume nodulation by sophisticated transcriptional regulatory networks. Molecular Plant. 2019; 12 :1179-1181. DOI: 10.1016/j.molp.2019.07.008 - 153.
Mortier V, Den Herder G, Whitford R, Van de Velde W, Rombauts S, D'Haeseleer K, et al. CLE peptides control Medicago truncatula nodulation locally and systemically. Plant Physiology. 2010;153 :222-237. DOI: 10.1104/pp.110.153718 - 154.
Schnabel E, Journet E-P, de Carvalho-Niebel F, Duc G, Frugoli J. The Medicago truncatula SUNN gene encodes a CLV1-like leucine-rich repeat receptor kinase that regulates nodule number and root length. Plant Molecular Biology. 2005;58 :809-822. DOI: 10.1007/s11103-005-8102-y - 155.
Searle IR, Men AE, Laniya TS, Buzas DM, Iturbe-Ormaetxe I, Carroll BJ, et al. Long-distance signaling in nodulation directed by a CLAVATA1-like receptor kinase. Science. 2003; 299 :109-112. DOI: 10.1126/science.1077937 - 156.
Krusell L, Madsen LH, Sato S, Aubert G, Genua A, Szczyglowski K, et al. Shoot control of root development and nodulation is mediated by a receptor-like kinase. Nature. 2002; 420 :422-426. DOI: 10.1038/nature01207 - 157.
Suzaki T, Yoro E, Kawaguchi M. Leguminous plants: Inventors of root nodules to accommodate symbiotic bacteria. International Review of Cell and Molecular Biology. 2015; 316 :111-158. DOI: 10.1016/bs.ircmb.2015.01.004 - 158.
Sasaki T, Suzaki T, Soyano T, Kojima M, Sakakibara H, Kawaguchi M. Shoot-derived cytokinins systemically regulate root nodulation. Nature Communications. 2014; 5 :4983. DOI: 10.1038/ncomms5983 - 159.
Tiwari M, Pandey V, Singh B, Yadav M, Bhatia S. Evolutionary and expression dynamics of LRR-RLKs and functional establishment of KLAVIER homolog in shoot mediated regulation of AON in chickpea symbiosis. Genomics. 2021; 113 :4313-4326. DOI: 10.1016/j.ygeno.2021.11.022 - 160.
van Noorden GE, Ross JJ, Reid JB, Rolfe BG, Mathesius U. Defective long-distance auxin transport regulation in the Medicago truncatula super numeric nodules mutant. Plant Physiology. 2006;140 :1494-1506. DOI: 10.1104/pp.105.075879 - 161.
Wang C, Reid JB, Foo E. The art of self-control - autoregulation of plant-microbe symbioses. Frontiers in Plant Science. 2018; 9 :988. DOI: 10.3389/fpls.2018.00988 - 162.
Meixner C, Vegvari G, Ludwig-Müller J, Gagnon H, Steinkellner S, Staehelin C, et al. Two defined alleles of the LRR receptor kinase GmNARK in supernodulating soybean govern differing autoregulation of mycorrhization. Physiologia Plantarum. 2007; 130 :261-270. DOI: 10.1111/j.1399-3054.2007.00903.x - 163.
Püschel D, Janouskova M, Voriskova A, Gryndlerova H, Vosatka M, Jansa J. Arbuscular mycorrhiza stimulates biological nitrogen fixation in two Medicago spp. through improved phosphorus acquisition. Frontiers in Plant Science. 2017;2017 :8. DOI: 10.3389/fpls.2017.00390 - 164.
Larimer AL, Clay K, Bever JD. Synergism and context dependency of interactions between arbuscular mycorrhizal fungi and rhizobia with a prairie legume. Ecology. 2014; 95 :1045-1054. DOI: 10.1890/13-0025.1 - 165.
Bournaud C, James EK, de Faria SM, Lebrun M, Melkonian R, Duponnois R, et al. Interdependency of efficient nodulation and arbuscular mycorrhization in Piptadenia gonoacantha , a Brazilian legume tree. Plant, Cell & Environment. 2017;41 :2008-2020. DOI: 10.1111/pce.13095 - 166.
Vadez V, Beck DP, Lasso JH, Drevon JJ. Utilization of the acetylene reduction assay to screen for tolerance of symbiotic N2 fixation to limiting P nutrition in common bean. Physiologia Plantarum. 1997; 99 :227-232. DOI: 10.1111/j.1399-3054.1997.tb05406.x - 167.
Mortimer PE, Perez-Fernandez MA, Valentine AJ. The role of arbuscular mycorrhizal colonization in the carbon and nutrient economy of the tripartite symbiosis with nodulated Phaseolus vulgaris . Soil Biology & Biochemistry. 2008;40 :1019-1027. DOI: 10.1016/j.soilbio.2007.11.014 - 168.
Chen BD, Li XL, Tao HQ , Christie P, Wong MH. The role of arbuscular mycorrhiza in zinc uptake by red clover growing in a calcareous soil spiked with various quantities of zinc. Chemosphere. 2003; 50 :839-846. DOI: 10.1016/s0045-6535(02)00228-x - 169.
Ibiang YB, Mitsumoto H, Sakamoto K. Bradyrhizobia and arbuscular mycorrhizal fungi modulate manganese, iron, phosphorus, and polyphenols in soybean ( Glycine max (L.) Merr.) under excess zinc. Environmental and Experimental Botany. 2017;137 :1-13. DOI: 10.1016/j.envexpbot.2017.01.011 - 170.
Sakamoto K, Ogiwara N, Kaji T. Involvement of autoregulation in the interaction between rhizobial nodulation and AM fungal colonization in soybean roots. Biology and Fertility of Soils. 2013; 49 :1141-1152. DOI: 10.1007/s00374-013-0804-8 - 171.
Meghvansi MK, Prasad K, Harwani D, Mahna SK. Response of soybean cultivars toward inoculation with three arbuscular mycorrhizal fungi and Bradyrhizobium japonicum in the alluvial soil. European Journal of Soil Biology. 2008;44 :316-323. DOI: 10.1016/j.ejsobi.2008.03.003 - 172.
Afkhami ME, Almeida BK, Hernandez DJ, Kiesewetter KN, Revillini DP. Tripartite mutualisms as models for understanding plant–microbial interactions. Current Opinion in Plant Biology. 2020; 56 :28-36. DOI: 10.1016/j.pbi.2020.02.003 - 173.
Konvalinková T, Jansa J. Lights off for arbuscular mycorrhiza: On its symbiotic functioning under light deprivation. Frontiers in Plant Science. 2016; 2016 :7. DOI: 10.3389/fpls.2016.00782 - 174.
Kleinert A, Venter M, Kossmann J, Valentine A. The reallocation of carbon in P deficient lupins affects biological nitrogen fixation. Journal of Plant Physiology. 2014; 171 :1619-1624. DOI: 10.1016/j.jplph.2014.07.017