Lipid transfer from plants to arbuscular mycorrhiza fungi

Arbuscular mycorrhiza (AM) symbioses contribute to global carbon cycles as plant hosts divert up to 20% of photosynthate to the obligate biotrophic fungi. Previous studies suggested carbohydrates as the only form of carbon transferred to the fungi. However, de novo fatty acid (FA) synthesis has not been observed in AM fungi in absence of the plant. In a forward genetic approach, we identified two Lotus japonicus mutants defective in AM-specific paralogs of lipid biosynthesis genes (KASI and GPAT6). These mutants perturb fungal development and accumulation of emblematic fungal 16:1ω5 FAs. Using isotopolog profiling we demonstrate that 13C patterns of fungal FAs recapitulate those of wild-type hosts, indicating cross-kingdom lipid transfer from plants to fungi. This transfer of labelled FAs was not observed for the AM-specific lipid biosynthesis mutants. Thus, growth and development of beneficial AM fungi is not only fueled by sugars but depends on lipid transfer from plant hosts. DOI: http://dx.doi.org/10.7554/eLife.29107.001


Introduction
Arbuscular mycorrhiza (AM) is a widespread symbiosis between most land plants and fungi of the Glomeromycota (Smith and Read, 2008). The fungi provide mineral nutrients to the plant. These nutrients are taken up from the soil and released inside root cortex cells at highly branched hyphal structures, the arbuscules (Javot et al., 2007). For efficient soil exploration, arbuscular mycorrhiza fungi (AMF) develop extended extraradical hyphal networks. Their growth requires a large amount of energy and carbon building blocks, which are transported mostly as lipid droplets and glycogen to the growing hyphal tips (Bago et al., 2002(Bago et al., , 2003. AMF are obligate biotrophs, as they depend on carbon supply by their host (Smith and Read, 2008). In the past, detailed 13 C-labeled tracerbased NMR studies demonstrated that hexose sugars are a major vehicle for carbon transfer from plants to fungi (Shachar-Hill et al., 1995). In addition, a fungal hexose transporter, with high transport activity for glucose is required for arbuscule development and quantitative root colonization as shown by host induced gene silencing (Helber et al., 2011), indicating the importance of hexose transfer for intra-radical fungal development.
AMF store carbon mainly in the form of lipids (Trépanier et al., 2005). The predominant storage form is triacylglycerol (TAG) and the major proportion of FAs found in AMF is composed of 16:0 (palmitic acid), and of 16:1w5 (palmitvaccenic acid). The latter is specific to AM fungi and certain demands of arbscocytes for metabolites including lipids. The importance of plant lipid biosynthesis for arbuscule development has been demonstrated by Medicago truncatula mutants in AM-specific paralogs of two lipid biosynthesis genes FatM and REDUCED ARBUSCULAR MYCORRHIZA2 (RAM2) Bravo et al., 2017). FatM encodes an ACP-thioesterase, which terminates fatty acid chain elongation in the plastid by cleaving the ACP off the acyl group releasing free FAs and soluble ACP (Jones et al., 1995). RAM2 encodes a glycerol 3-phosphate acyl transferase (GPAT) and is most similar to Arabidopsis GPAT6. In Arabidopsis, GPAT6 acetylates the sn-2 position of glycerol-3-phosphate with an FA and cleaves the phosphate from lysophosphatidic acid, thereby producing sn-2-monoacylglycerol (ßMAG, Yang et al., 2010). Mutations in both FatM and RAM2 impair arbuscule branching Bravo et al., 2017). In addition, arbuscule branching requires a complex of two half ABC transporters STR and STR2 (Zhang et al., 2010;Gutjahr et al., 2012). The substrate of STR/STR2 is unknown but other members of the ABCG transporter family are implicated in lipid transport (Wittenburg and Carey, 2002;Wang et al., 2011;Fabre et al., 2016;Hwang et al., 2016;Lee et al., 2016). Therefore, and due to its localization in the peri-arbuscular membrane (Zhang et al., 2010) it was speculated that the STR/STR2 complex may transport lipids towards arbuscules (Gutjahr et al., 2012;Bravo et al., 2017). Transcriptional activation of RAM2 and STR is controlled by the GRAS transcription factor REDUCED ARBUSCULAR MYCORRHIZA1 (RAM1) Park et al., 2015;Pimprikar et al., 2016) and also in ram1 mutants, arbuscule branching is impaired (Park et al., 2015;Xue et al., 2015;Pimprikar et al., 2016). Thus, RAM1, FatM, RAM2 and STR/STR2 appear to form an AM-specific operational unit for lipid biosynthesis and transport in arbuscocytes. Consistently, they were found to be absent from genomes of plants that have lost the ability to form AM (Delaux et al., 2014;Favre et al., 2014;Bravo et al., 2016).
Here, we analyzed two Lotus japonicus mutants identified in a forward genetic screen, which are impaired in arbuscule branching (Groth et al., 2013). Positional cloning combined with genome resequencing revealed mutations in a novel AM-specific b-keto-acyl ACP synthase I (KASI) gene and in the L. japonicus ortholog of M. truncatula RAM2. KASI likely acts upstream of RAM2 in producing 16:0 FAs. The identity of the genes and the phenotypes led us to hypothesize that AMF may depend on delivery of 16:0 FAs from the plant host. Using a combination of microscopic mutant characterization, lipidomics and isotopolog profiling of 16:0 and 16:1w5 FAs in roots and extraradical fungal mycelium, we provide strong evidence for requirement of both genes for AM-specific lipid biosynthesis and cross-kingdom lipid transfer from plants to AMF.

Results
Two L. japonicus arbuscule-branching mutants are defective in lipidbiosynthesis genes We previously identified two L. japonicus mutants disorganized arbuscules (dis-1, SL0154-N) and SL0181-N (red) deficient in arbuscule branching (Groth et al., 2013) (Figure 1A-B). Both mutants also suffered from a reduction in root length colonization and blocked the formation of lipid-containing vesicles of the fungus Rhizophagus irregularis ( Figure 1C-D). We identified the causative mutations with a combination of classical mapping and next generation sequencing (see Materials and methods). DIS encodes a b-keto-acyl ACP synthase I (KASI, Figure 1-figure supplements 1A-C and 2). KASI enzymes catalyze successive condensation reactions during fatty acyl chain elongation from C4:0-ACP to C16:0-ACP . SL0181-N carries one mutation (ram2-1) in the L. japonicus orthologue of the previously identified Medicago truncatula REDUCED ARBUSCU-LAR MYCORRHIZA2 (RAM2, Figure 1-figure supplements 3 and 4). Arabidopsis GPAT6 has been shown to produce ß-MAG with a preference for 16:0 FAs (Yang et al., 2012). Therefore, we hypothesized that DIS and RAM2 act in the same biosynthetic pathway.
We identified additional allelic dis mutants by TILLING (Figure 1-figure supplement 1E, Supplementary file 1) (Perry et al., 2003) and a ram2 mutant caused by a LORE1 insertion in the RAM2 gene (Figure 1-figure supplement 3B) (Małolepszy et al., 2016). Among the allelic dis mutants we chose dis-4 for further investigation because it suffers from a glycine replacement at the border of a conserved ß-sheet ( Figure 1-figure supplement 2), which likely affects protein folding (Perry et al., 2009). Both allelic mutants dis-4 and ram2-2 phenocopied dis-1 and ram2-1, respectively. Furthermore, transgenic complementation of both dis-1 and ram2-1 with the wild-type versions of the mutated genes restored arbuscule-branching and wild-type-like levels of root length colonization and vesicle formation ( Figure 1A-B). Taken together this confirmed identification of both causal mutations.  The following figure supplements are available for figure 1: . To analyze the spatial activity pattern of the DIS and RAM2 promoters during colonization we fused 1.5 kb for DIS and 2.275 kb for RAM2 upstream of the translational start site to the uidA gene. Consistent with a role of both genes in arbuscule development GUS activity was predominantly detected in arbuscocytes (arbuscule-containing cells) in both wild-type and the corresponding mutant roots (Figure 2-figure supplement 1A-B).
To correlate promoter activity with the precise stage of arbuscule development we used nuclear localized YFP as a reporter. To visualize the fungus, the promoter:reporter cassette was co-transformed with a second expression cassette containing secreted mCherry fused to the SbtM1 promoter. This promoter drives expression in colonized cells, in cells neighboring apoplastically growing hyphae and in cells forming pre-penetration apparatuus (PPAs, cytoplasmic aggregations that assemble in cortex cells prior to arbuscule development) (Genre et al., 2008;Takeda et al., 2009Takeda et al., , 2012. When expressed under the control of the SbtM1 promoter, secreted mCherry accumulates in the apoplast surrounding fungal structures and PPAs, thereby revealing the silhouette of these structures (Figure 2A-B, Videos 1-2). Nuclear localized YFP fluorescence indicated activity of both promoters in cells containing PPAs (c, Videos 1-2) and containing sparsely branched (d) or mature (e) arbuscules. Furthermore, we rarely detected YFP fluorescence in non-colonized cells in direct neighborhood of arbuscocytes, which were possibly preparing for PPA formation (a). However, YFP signal was absent from cells containing collapsed arbuscules (f), indicating that the promoters were active during arbuscule development and growth but inactive during arbuscule degeneration (Figure 2A -B). RAM2 promoter activity was strictly correlated with arbuscocytes, while the DIS promoter showed additional activity in cortical cells of non-colonized root segments (Figure 2A To examine, whether arbuscocyte-specific expression of DIS and RAM2 is sufficient for fungal development we complemented the dis-1 and ram2-1 mutants with the corresponding wild-type genes fused to the arbuscocyte-specific PT4 promoter (Volpe et al., 2013). This restored arbusculebranching, vesicle formation as well as root length colonization in the mutants ( Figure 2C-F), showing that arbuscocyte-specific expression of DIS and RAM2 suffices to support AM development. Thus, expression of lipid biosynthesis genes in arbuscocytes is not only important for arbuscule branching but also for vesicle formation and quantitative colonization.
The KASI family comprises three members in L. japonicus Growth and development of dis and ram2 mutants are not visibly affected (Figure 3-figure supplement 2), although they carry defects in important lipid biosynthesis genes. RAM2 is specific to AMcompetent plants Delaux et al., 2014;Favre et al., 2014;Bravo et al., 2016) and activated in an AM-dependent manner (Figure 2, Figure 3-figure supplement 1A) (Gobbato et al., , 2013. Plants contain an additional GPAT6 paralog, which likely fulfills the housekeeping function ( Figure 1-figure supplement 4, Yang et al., 2012;Delaux et al., 2015). To understand whether the same applies to DIS we searched the L. japonicus genome for additional KASI genes. We detected three paralogs KASI, DIS and DIS-LIKE ( . Phylogenetic analysis revealed a split of seed plant KASI proteins into two different clades, called KASI and DIS ( Figure 3). Members of the KASI clade, are presumably involved in housekeeping functions as this clade contains the product of the KASI single copy gene in Arabidopsis (Wu and Xue, 2010). Members of the DIS clade are found specifically in AM-host dicotyledons and in a gymnosperm ( Figure 3). As confirmed by synteny analysis (Figure 3figure supplement 3), DIS is absent from all eight analyzed non-host dicotyledon genomes, a phylogenetic pattern similar to other symbiosis genes (Delaux et al., 2014;Favre et al., 2014;Bravo et al., 2016). The occurrence of DIS in Lupinus species, which lost AM competence but still form root nodule symbiosis, may be a relic from the AM competent ancestor. An apparently, Lotusspecific, and thus recent duplication of the DIS gene resulted in an 87% identical copy (DIS-LIKE) located directly adjacent to DIS in a tail-to-tail orientation (

DIS functions like a canonical KASI in planta
We examined whether DIS can substitute the phylogenetically related housekeeping KASI. To this end we transgenically complemented an Arabidopsis kasI mutant (Wu and Xue, 2010) with Lotus DIS driven by the Arabidopsis KASI promoter. Arabidopsis kasI exhibits an altered FA profile and reduced rosette growth (Wu and Xue, 2010). Complementation with DIS restored both wild-typelike rosette growth and FA accumulation. The kasI phenotypes persisted when the dis-1 mutant allele was transformed as a negative control ( Figure 4C-E). In the reverse cross-species complementation AtKASI driven by the DIS promoter restored colonization, arbuscule branching and vesicle  The following figure supplement is available for figure 2:  Video 4. Scan through confocal z-stack of Figure 2Ab illustrating DIS promoter activity exclusively in the cortex. DOI: 10.7554/eLife.29107.013 Video 5. Scan through confocal z-stack of Figure 2Ba illustrating correlation of RAM2 promoter activity with arbuscocytes. DOI: 10.7554/eLife.29107.014 Video 6. Scan through confocal z-stack of Figure 2Bb illustrating absence of RAM2 promoter activity from non-colonized cells.  Phylogenetic trees were generated by neighbor-joining implemented in MEGA5 (Tamura et al., 2011). Partial gap Figure 3 continued on next page The AM-specific increase in 16:0 and 16:1v5 FA containing lipids is abolished in the dis mutant To characterize the role of DIS in determining the lipid composition of non-colonized and colonized roots we quantified triacylglycerols (TAGs), diacylglycerols (DAGs), galactolipids and phospholipids in wild-type and dis-1. The lipid profile of colonized roots contains both plant and fungal lipids, however using the fungal marker FA 16:1w5 and previous data on fungus-specific lipids (Wewer et al., 2014), many fungal lipids can be clearly distinguished from plant lipids. The lipid profile of non-colonized roots was not affected by the dis-1 mutation. However, the strong and significant increase of 16:0 and 16:1 (most probably fungus-specific 16:1w5) containing TAGs, which is characteristic for colonization of wild-type roots (Wewer et al., 2014) was abolished in dis-1 ( Figure  . Moreover, the AM-dependent transcriptional activation of DIS and KASIII, the latter of which is a single copy gene in L. japonicus and produces precursors for DIS-activity by catalyzing FA chain elongation from C2 to C4, was absent from ram1 mutants ( Figure 6). In contrast, induction of the single copy gene KASII, which elongates fatty acyl chains from C16 to C18 was not hampered by RAM1 deficiency. Thus, RAM1 may play an important role in the regulation of lipid biosynthesis in arbuscocytes, since it also mediates expression of RAM2 and STR Park et al., 2015;Pimprikar et al., 2016;Luginbuehl et al., 2017). We hypothesized that RAM1, DIS, RAM2 and STR form a specific operational unit for lipid biosynthesis and transport in arbuscocytes. Therefore, we directly compared their impact on the AM-specific root lipid profile and measured galactolipids, phospholipids, TAGs and also total and free fatty acids in colonized roots of ram1, dis, ram2, str mutants and wild-type in parallel. Consistent with our previous observation in dis-1, galactolipid accumulation was similar in colonized roots of wild-type and all mutants (Figure 5-figure supplement 3C-D). In contrast, total 16:0 FAs (FAMEs) as well as 16:1 and 18:1 (likely 18:1w7 FA of fungal origin) FAs were strongly reduced in all colonized mutants compared to the corresponding wild-type. Free FAs showed a similar pattern except for 18:1 FAs   Figure 5F). This suggests that RAM2 acts downstream of DIS in a biosynthetic pathway and uses the 16:0 FAs synthesized by DIS in arbuscocytes as substrates. In the absence of functional RAM2 the FA products of DIS, are probably redirected into phospholipid biosynthesis and storage lipid biosynthesis via PA and PC  leading to the observed higher accumulation of 16:0 FA containing lipid species in ram2 mutants. This higher accumulation of specific lipids did not correlate with colonization levels in ram2 mutants (Figure 5-figure supplement 4) confirming that reduced colonization levels are not the primary cause for altered lipid profiles in the colonized mutant roots. Instead, defective AM-specific lipid biosynthesis in the mutants more likely impairs fungal development.

The abundance of 16:0 ß-monoacyl-glycerol is reduced in all mutants
The first step in TAG and phospholipid production after FA biosynthesis is the esterification of FAs with glycerol by GPATs in the plastid or endoplasmic reticulum to produce a-MAGs (sn1/3-MAGs, Li-Beisson et al., 2010). RAM2 is predicted to produce a different type of glycerolipid ß-MAG (sn2-MAG) with a preference towards 16:0 and 18:1 FAs (Yang et al., 2010;Wang et al., 2012;Yang et al., 2012). To examine the role of RAM2 in MAG biosynthesis, we quantified a-MAG and ß-MAG species in colonized roots of wild-type and all mutants. The abundance of ß-MAGs was generally lower than that of a-MAGs (Figure 7). The amount of most a-MAG species did not differ among the genotypes. Only the fungus-specific 16:1 and 18:1w7 a-MAGs were reduced in all mutants reflecting the lower fungal biomass ( Figure 7A). Fungus-specific ß-MAGs with 16:1 and 18:1w7 acyl groups were not detected and most ß-MAG molecular species accumulated to similar levels in all genotypes. Exclusively the levels of 16:0 ß-MAGs were significantly lower in all mutants as compared to the corresponding wild-type roots ( Figure 7B). This supports a role of RAM2 in 16:0 ß-MAG synthesis during AM and a role of DIS in providing 16:0 FA precursors for RAM2 activity. A low accumulation, of 16:0 ß-MAGs in ram1 mutants is consistent with RAM1's role in regulating the FA and lipid biosynthesis genes ( Figure 6) Pimprikar et al., 2016). In str 16:0 ß-MAGs likely did not accumulate because of reduced RAM2 expression in str roots due to low root length colonization and/or a regulatory feedback loop (Bravo et al., 2017). DIS, RAM2 and STR are required for transfer of 13 C label from plant to fungus In plants, ß-MAGs serve as precursors for cutin polymers at the surface of aerial organs (Yang et al., 2012;Yeats et al., 2012). For their use in membrane or storage lipid biosynthesis they first need to be isomerized to a-MAGs . The recruitment of a GPAT6 (RAM2) instead of a a-MAG-producing GPAT for AM-specific lipid synthesis supports the idea that RAM2-products are destined for something else than membrane biosynthesis of the host cell. Since AM fungal genomes lack genes encoding cytosolic FA synthase subunits (Wewer et al., 2014;Ropars et al., 2016;       Tang et al., 2016) we hypothesized that 16:0 ß-MAGs synthesized by DIS-and RAM2 are predominantly delivered to the fungus. To test this hypothesis, we examined lipid transfer by FA isotopolog profiling. Isotopologs are molecules that differ only in their isotopic composition. For isotopolog profiling an organism is fed with a heavy isotope labelled precursor metabolite. Subsequently the labelled isotopolog composition of metabolic products is analyzed. The resulting characteristic isotopolog pattern yields information about metabolic pathways and fluxes .
We could not detect fungus-specific 16:1w5 ß-MAGs in colonized roots ( Figure 7B). Therefore, we reasoned that either a downstream metabolite of ß-MAG is transported to the fungus, or alternatively, ß-MAG is rapidly metabolized in the fungus prior to desaturation of the 16:0 acyl residue. Since the transported FA groups can be used by the fungus for synthesizing a number of different lipids, we focused on total 16:0 FA methyl esters (FAMEs, subsequently called FAs for simplicity) and 16:1w1 FAMEs as markers for lipid transfer. We fed L. japonicus wild-type, dis-1, ram2-1 and str with [U-13 C 6 ]glucose and then measured the isotopolog composition of 16:0 FAs and 16:1w5 FAs in L. japonicus roots and in associated extraradical fungal mycelium with spores. To generate sufficient hyphal material for our measurements the fungus was pre-grown on split Petri dishes in presence of a carrot hairy root system as nurse plant (Figure 8-figure supplement 1). Once the fungal mycelium had covered the plate, L. japonicus seedlings were added to the plate on the side opposing the carrot root. During the whole experiment, the fungus was simultaneously supported by the carrot hairy root and the L. japonicus seedling. Once the L. japonicus roots had been colonized, labelled glucose was added to the side containing L. japonicus. After an additional week, FAs were esterified and extracted from colonized L. japonicus roots and from the associated extraradical mycelium and the total amount of 13 C labelled 16:0 and 16:1w5 FAs as well as their isotopolog composition was determined. In L. japonicus wild-type 13 C-labeled 16:0 and 16:1w5 FAs were detected in colonized

Host plants determine the isotopolog pattern of fungal FAs
Remarkably, the isotopolog profile of 16:0 FAs was close to identical between colonized L. japonicus roots and the connected extraradical mycelium, for 11 independent samples of wild-type Gifu ( Figure 8C-D, Figure 8-figure supplement 4) and for 5 independent samples of wild-type MG20 (Figure 8-figure supplement 2C-D). Moreover, the isotopolog profile of fungus-specific 16:1w5 FAs mirrored the profile of 16:0 FAs ( Figure 8C, Figure 8-figure supplements 2,4). Pattern conservation between root and associated extraradical mycelium occurred independently of pattern variation among individual samples. Since the fungus does not incorporate 13 C into the analyzed FAs in the absence of the plant ( Figure 8A and colonized carrot, L. japonicus wild-type, dis-1, ram2-1 roots and in the extraradical mycelium of R. irregularis. P values were generated by ANOVA using the Dunnett Test for multiple comparisons to L. japonicus wild-type (n = 29 (16:0 control roots); n = 33 (16:0 root AM); n = 39 (16:0 extraradical mycelium); n = 33 (16:1w5 root AM); n = 39 (16:1w5 extraradical mycelium), ***p<0.001, Figure 8 continued on next page japonicus seedlings ( Figure 8D, Figure 8-figure supplement 1). In these root organ cultures, sugar uptake from the medium does not compete with photosynthesis, as in whole seedlings. Additionally, the carrot roots explore a larger surface of the Petri dish, increasing access to substances in the nutrient medium. Consequently, and likely because of increased uptake of labelled glucose from the medium, the isotopolog pattern of carrot ROCs differed from Lotus and was shifted towards more highly labeled 16:0 FA isotopologs. This fingerprint was again recapitulated in the extraradical fungal mycelium as well as in fungus-specific 16:1w5 FAs inside and outside the root for 10 independent samples ( Figure 8C, Figure 8-figure supplement 4). These data provide strong support for direct transfer of a 16:0 FA containing lipid from plants to AMF (Figure 9).

Discussion
Here we identified DIS and RAM2, two AM-specific paralogs of the lipid biosynthesis genes KASI and GPAT6 using forward genetics in Lotus japonicus. The dis and ram2 mutants enabled us to demonstrate lipid transfer from plants to AMF using isotopolog profiling.
During AM symbiosis, an array of lipid biosynthesis genes is induced in arbuscocytes (Gaude et al., 2012a(Gaude et al., , 2012b, indicating a large demand for lipids in these cells. Indeed, two genes encoding lipid biosynthesis enzymes, the thioesterase FatM and the GPAT6 RAM2, have previously been shown to be required for arbuscule branching in M. truncatula Bravo et al., 2017;Jiang et al., 2017). Both enzymes have a substrate preference for 16:0 FAs (Salas and Ohlrogge, 2002;Yang et al., 2012;Bravo et al., 2017) and, consistent with this, we and others observed that colonized ram2 mutant roots over-accumulate 16:0 FA containing phospholipids and TAGs (Figure 7, [Bravo et al., 2017]), indicating re-channeling of superfluous 16:0 FAs in the absence of RAM2 function and placing RAM2 downstream of FatM (Figure 9).
Our discovery of DIS, a novel and AM-specific KASI gene, now provides evidence for the enzyme which synthesizes these 16:0 FAs in arbuscocytes. The arbuscule phenotype, as well as the lipid profile of colonized dis mutants is very similar to fatm and ram2 mutants except for the accumulation of 16:0 FA-containing lipids in ram2 (Figure 1, Figure 5 and all figure supplements), consistent with the predicted function. Together, this strongly suggests that DIS, FatM and RAM2 act in the same lipid biosynthesis pathway, which is specifically and cell-autonomously induced when a resting root cortex cell differentiates into an arbuscocyte (Figure 2A-B, Figure 9, [Bravo et al., 2017]). Interestingly, DIS was exclusively found in genomes of AM-competent dicotyledons and a gymnosperm (Figure 3). This implies that DIS has been lost at the split of the mono-from dicotyledons. Despite the Figure 8 continued **p<0.01, *p<0.05). (C) Relative fraction of 13 C isotopologs for 16:0 FAs of three replicates of carrot, L. japonicus WT Gifu, dis-1, ram2-1 in control roots (upper panel) and AM roots and each of the associated R. irregularis extraradical mycelia with spores (middle panel) and 16:1w5 FAs in AM roots and extraradical mycelia with spores (lower panel). Individual bars and double bars indicate individual samples. Values from roots are indicated by 'R' and from fungal extraradical mycelia with spores by 'M'. For carrot and L. japonicus WT the 13 C labelling pattern of 16:0 and 16:1w5 FAs in the plant is recapitulated in the fungal extraradical mycelium. Extraradical mycelium associated with dis-1 and ram2-1 does not mirror these patterns. Compare bars for AM roots and extraradical mycelium side by side. Black numbers indicate 13 C o. e. for individual samples. Colors indicate 13 C-isotopologs carrying one, two, three, etc. 13 C-atoms (M + 1, M + 2, M + 3, etc.). (D) Schematic and simplified illustration of carbon flow and 12 C vs. 13 C-carbon contribution to plant lipid metabolism and transport to the fungus in the two-compartment cultivation setup used for isotope labelling. Carbohydrate metabolism and transport is omitted for simplicity. ERM, extraradical mycelium. DOI: 10.7554/eLife.29107.037 The following source data and figure supplements are available for figure 8: Source data 1. Raw data for isotopolog profiles in Figure 8 and  Bravo et al., 2017). These are transported Figure 9 continued on next page phylogenetic divergence, DIS and the single copy housekeeping KASI gene of Arabidopsis are interchangeable ( Figure 5). Therefore, the specificity of DIS to function in AM symbiosis is probably encoded in its promoter (Figure 2). In monocotyledons, the promoter of the housekeeping KASI gene may have acquired additional regulatory elements, sufficient for arbuscocyte-specific activation, thus making DIS dispensable. We provide several pieces of complementary evidence that lipids synthesized by DIS and RAM2 in the arbuscocyte are transferred from plants to AMF and are required for fungal development. We fed host plants with [U-13 C 6 ]glucose and subsequently determined the isotopolog profile of freshly synthetized 16:0 and 16:1w5 FAs in roots and associated fungal extraradical mycelia (Figure 8). This showed that: (1) AMF were unable to incorporate 13 C into FAs when fed with [U-13 C 6 ]glucose in absence of the host plant.
(2) When associated with a wild-type host, the fungal extraradical mycelium accumulated 13 C labelled 16:0 FAs and the isotopolog profile of these 16:0 FAs was almost identical with the host profile. (3) The 16:0 FA isotopolog fingerprint differed strongly between two different wild-type plant systems (Lotus seedling and carrot hairy root) but for each of them the fungal mycelium recapitulated the isotopolog profile. Therefore clearly, the plant dominates the profile of the fungus, because it is impossible that the fungus by itself generates the same FA isotopolog pattern as the plant -especially in the absence of cytosolic FA synthase. Therefore, this result provides compelling evidence for interkingdom transfer of 16:0 FAs from plants to AMF. (4) In agreement, the isotopolog profile of fungus-specific 16:1 w5 FAs inside and outside the root also resembled the plant 16:0 FA profile. (5) Colonized dis and ram2 mutant roots resembled the 16:0 FA isotopolog profile of L. japonicus wild-type roots. However, the 16:0 FA profile of the fungal extraradical mycelium and the 16:1w5 FA profile inside the roots showed a very different pattern, consistent with very low transport of labelled FAs to the fungus when associated with the mutants. (6) DIS and RAM2 are specifically required for the synthesis of 16:0 ß-MAG (Figure 7) and the predominant FA chain length found in AM fungi is precisely 16. (7) dis and ram2 roots do not allow the formation of lipid-containing fungal vesicles and accumulate very low levels of fungal signature lipids ( Figure 5 and figure supplements). Together this strongly supports the idea that DIS and RAM2 are required to provide lipids for transfer to the fungus. Consequently, in the mutants, the fungus is deprived of lipids.
The L. japonicus mutants were originally identified due to their defective arbuscule branching (Groth et al., 2013). The promoters of DIS and RAM2 are active in arbusocytes and already during PPA formation, the earliest visible stage of arbuscocyte development. Together with the stunted arbuscule phenotype of dis, ram2 and fatm mutants (Figure 1 [ Bravo et al., 2017]) this suggests that plant lipids are needed for arbuscule growth, probably to provide material for the extensive plasma-membrane of the highly branched fungal structure. It also indicates that the arbuscule dictates development of the AMF as a whole, since lipid uptake at the arbuscule is required for vesicle formation, full exploration of the root and development of extraradical mycelia and spores. Defective arbuscule development was also observed for the different and phylogenetically distantly related AMF Gigaspora rosea (Groth et al., 2013), which similar to R. irregularis lacks genes encoding cytosolic FA synthase from their genomes (Wewer et al., 2014;Tang et al., 2016). Hence the dependence on plant lipids delivered at the arbuscule is likely a common phenomenon among AMF and a hallmark of AMF obligate biotrophy.
Despite the obvious central importance of lipid uptake by the arbuscule, the fungus can initially colonize the mutant roots with a low amount of intraradical hyphae and stunted arbuscules (Figure 1, Figure 5-figure supplement 4). The construction of membranes for this initial colonization may be supported by the large amounts of lipids stored in AMF spores. This would be consistent with the frequent observation that in wild-type roots, at initial stages of root colonization, AMF form Figure 9 continued from the plant cell to the fungus. The PAM-localized ABCG transporter STR/STR2 is a hypothetical candidate for lipid transport across the PAM. Desaturation of 16:0 FAs by fungal enzymes (Wewer et al., 2014) leads to accumulation of lipids containing specific 16:1w5 FAs. Mal-CoA, Malonyl-Coenzyme A; FA, fatty acid; KAS, b-keto-acyl ACP synthase; GPAT, Glycerol-3-phosphate acyl transferase; PAM, periarbuscular membrane; LPA, lysophosphatic acid; MAG, monoacylglycerol; DAG, diacylglycerol; TAG, triacylglycerol; PA, phosphatidic acid; PC, phosphatidylcholine; PE, phosphatidylethanolamine; PS, phosphatidylserine; CDP-DAG, cytidine diphosphate diacylglycerol; PG, phosphatidylglycerol; PI, phosphatidylinositol. DOI: 10.7554/eLife.29107.043 arbuscules immediately after reaching the inner cortex and before colonizing longer distances, possibly as a strategy to accquire lipids quickly after the reserves in the spore have been depleted. Alternatively, it is possible that plant housekeeping enzymes provide lipids to intraradical hyphae before arbuscule formation. Activity of the housekeeping KASI may also be responsible for slightly higher colonization levels observed for dis in some experiments as compared to other mutants.
It has recently been reported that photosynthetic wild-type nurse plants can restore arbusculebranching in Medicago ram2 and str mutants (Jiang et al., 2017;Luginbuehl et al., 2017), suggesting that lipids can be supplied to arbuscules via the extraradical hyphal network and intraradical hyphae through this route support arbuscule fine-branching. Based on four observations, we favor an alternative szenario, in which lipids need to be provided cell-autonomously by the arbuscocyte to support arbuscule fine-branching. However, we cannot exclude that our observations differ from the reported observations due to growth conditions or plant species. (1) Presence of nurse carrot hairy roots did not restore arbuscule branching in dis, ram2 and str (Figure 8-figure supplement 1C-F).
(2) dis and ram2 were found in a forward genetics screen based on their stunted arbuscule phenotype. In this screen, the fungal inoculum was provided via chive nurse plants (Groth et al., 2013). (3) Map-based cloning of Lotus dis, ram2 and str (Kojima et al., 2014) was performed with segregating mutant populations grown in the same pot, in which the wild-type and heterozygeous siblings acted as nurse plants on the homozygeous mutants. In this system, the stunted arbuscule phenotype was easily observable. (4) Arbuscule branching in a rice str mutant was not restored by wild type nurse plants (Gutjahr et al., 2012).
It still remains to be shown, which types of lipids are transported from the plant arbuscocyte to the fungal arbuscule and how. RAM2 is the most downstream acting enzyme in arbuscocyte-specific lipid biosynthesis known to date (Figure 9). It is predicted to synthesize ß-MAG and we and others have shown that 16:0 ß-MAGs are indeed reduced in colonized roots of dis, fatm and ram2 mutants, providing evidence that this is likely the case (Figure 7, [Bravo et al., 2017]). Although, we cannot exclude that a downstream metabolite of 16:0 ß-MAG is transported to the fungus, 16:0 ß-MAG as transport vehicle for 16:0 FAs to the fungus is a good candidate because conceptually this molecule may bear certain advantages. It has been shown in Arabidopsis that ß-MAGs are not used for plant storage or membrane lipid biosynthesis but rather as pre-cursors for cuticle formation (Li et al., 2007). The production of ß-MAGs could therefore, be a way, to withdraw FAs from the plants own metabolism to make them available to the fungus. In addition, ß-MAGs are small and amphiphilic and could diffuse across the short distance of the hydrophilic apoplastic space between plant and fungal membrane. At the newly growing arbuscule branches the distance between the plant and fungal membrane is indeed very small and has been measured to be 80-100 nm on TEM images of high-pressure freeze-substituted samples (Bonfante, 2001). However, we could not detect fungusspecific 16:1w5 ß-MAGs in colonized roots. This could mean that the fungus metabolizes them before desaturation of the 16:0 FAs to synthesize membrane and storage lipids. Alternatively, ß-MAGs may not be taken up by the fungus. ß-MAGs are known to isomerize to a-MAGs in acid or basic conditions (Iqbal and Hussain, 2009). It is therefore, possible that they isomerize in the acidic periarbuscular space (Guttenberger, 2000) before being taken up by the arbuscule.
How are MAGs transported across the peri-arbuscular membrane? Good candidates for MAG transporters are the ABCG half transporters STR and STR2. Similar ABCG transporters have been implicated genetically in cuticle formation, which also requires ß-MAGs (Pighin et al., 2004;Panikashvili et al., 2011;Yeats et al., 2012). The half ABCG transporters STR and STR2 are both independently required for arbuscule branching and they need to interact to form a full transporter (Zhang et al., 2010). We found that colonized roots of a L. japonicus str mutant, did not allow the formation of fungal vesicles and had the same lipid profile as dis and ram2 ( Figure 5 and figure supplements). Furthermore, our 13 C labelling experiment demonstrated that str mutants do not transfer lipids to the fungus (Figure 8-figure supplement 2). Although these are encouraging indications, strong evidence for the role of STR in lipid transport across the periarbuscular membrane is still lacking and the substrate of STR remains to be determined. Therefore, currently, it cannot be excluded that mutation of str has an indirect effect on lipid transport and alternative mechanisms for example lipid translocation via vesicle fission and fusion are possible. Nevertheless, also in AMF, several ABC transporter genes are expressed in planta (Tisserant et al., 2012;Tang et al., 2016). They are not characterized, but if lipid transport via ABC transporters instead of other mechanisms would play a role, some of them could be involved in uptake of lipids into the fungal cytoplasm.
We found that mutants in the GRAS gene RAM1 are impaired in AM-specific lipid accumulation in colonized roots and in AM-mediated activation of DIS and the single copy gene KASIII (Figure 6), in addition to FatM, RAM2 and STR Park et al., 2015;Pimprikar et al., 2016;Luginbuehl et al., 2017). This suggests that plants have evolved an AM-specific regulatory module for lipid production in arbuscocytes and delivery to the fungus. It remains to be shown, whether RAM1 regulates lipid biosynthesis genes directly and how this occurs mechanistically.
Our finding that plants transfer lipids to AMF completely changes the previous view that the fungus receives only sugars from the plant (Pfeffer et al., 1999;Trépanier et al., 2005). It will now be interesting to determine the relative contributions of sugar and lipid transfer to AMF, and whether this may be a determinant of variation in root length colonization and extraradical mycelium formation depending on the plant-fungal genotype combination (Sawers et al., 2017). An interesting question refers to why AMF have lost the genes encoding cytosolic FA synthase to depend on the lipid biosynthesis machinery of the host. FA biosynthesis consumes more energy than biosynthesis of carbohydrates and organic carbon provided by the plant needs to be transported in fungal hyphae over long distances from the inside of the root to the extremities of the extraradical mycelium. Therefore, it is conceivable that supply of plant lipids to the fungus plus fungal lipid transport is more energy efficient for the symbiosis as a whole than fungal carbohydrate transport plus fungal lipid biosynthesis. Hence, inter-organismic lipid transfer followed by loss of fungal FA biosynthesis genes may have been selected for during evolution because it likely optimized the symbiosis for most rapid proliferation of extraradical mycelium, thus ensuring efficient mineral nutrient acquisition from the soil for supporting the plant host. Lipid transfer across kingdoms has also been observed in human parasites or symbiotic bacteria of insects (Caffaro and Boothroyd, 2011;Elwell et al., 2011;Herren et al., 2014). It will be interesting to learn whether this is a more widespread phenomenon among biotrophic inter-organismic interactions.

Plant growth and inoculation with AM fungi
Lotus japonicus ecotype  and ecotype MG-20 wild-type and str mutant (kindly provided by Tomoko Kojima (NARO, Tochigi, Japan) seeds were scarified and surface sterilized with 1% NaClO. Imbibed seeds were germinated on 0.8% Bacto Agar (Difco) at 24˚C for 10-14 days. Seedlings were cultivated in pots containing sand/vermiculite (2/1 vol.) as substrate. For colonization with Rhizophagus irregularis roots were inoculated with 500 spores (SYMPLANTA, Munich, Germany or Agronutrition, Toulouse, France) per plant. Plants were harvested 5 weeks post inoculation (wpi); except for dis-1 complementation in Figure 1A, which was harvested at 4 wpi. Arabidopsis thaliana seeds of Col-0 wild-type, kasI mutant in the Col-0 background and the transgenically complemented kasI mutant were surface sterilized with 70% EtOH +0.05% Tween 20% and 100% EtOH, germinated on MS-Medium for 48 hr at 4˚C in the dark followed by 5-6 days at 22˚C (8 hr light/dark).

Identification of DIS by map-based cloning and next generation sequencing
The L. japonicus dis mutant (line SL0154, [Groth et al., 2013]) resulting from an EMS mutagenesis program (Perry et al., 2003(Perry et al., , 2009) was backcrossed to ecotype Gifu wild-type and outcrossed to the polymorphic mapping parent ecotype MG-20. The dis locus segregated as a recessive monogenic trait and was previously found to be linked to marker TM2249 on chromosome 4 (Groth et al., 2013). We confirmed the monogenic segregation as 26 of 110 individuals originating from the cross to MG-20 (c 2 : P(3:1)=0.74) and 32 of 119 individuals originating from the cross to Gifu (c 2 : P(3:1) =0.63) exhibited the mutant phenotype. To identify SL0154-specific mutations linked to the dis locus, we employed a genome re-sequencing strategy. Nuclear DNA of Gifu wild-type and the SL0154 mutant was subjected to paired end sequencing (2 Â 100 bp) of a 300-500 bp insert library, on an Illumina Hi-Seq 2000 instrument resulting in between 16.7 and 19.5 Gigabases per sample, equivalent to roughly 35-41 fold coverage assuming a genome size of 470 Megabases. Reads were mapped to the reference genome of MG-20 v2.5  and single nucleotide polymorphisms identified using CLC genomics workbench (CLC bio, Aarhus, Denmark). SL0154-specific SNPs were identified by subtracting Gifu/MG-20 from SL0154/MG-20 polymorphisms. 19 potentially EMS induced (11x G->A, 8x C->T) SNPs called consistently in all mapped reads from SL0514 but not in Gifu were identified between the markers TM0046/TM1545, the initial dis target region (Figure 1-figure supplement 1A. In a screen for recombination events flanking the dis locus, 63 mutants out of 254 total F2 individuals of a cross MG-20 x SL0154 were genotyped with markers flanking the dis locus (Figure 1-figure supplement 1B). Interrogating recombinant individuals with additional markers in the region narrowed down the target interval between TM2249 and BM2170 (2 cM according to markers; ca. 650 kb). In this interval, 3 SL0154-specific SNPs with typical EMS signature (G to A transition) remained, of which one was predicted to be located in exon 3 of CM0004.1640.r2 (reference position 40381558 in L. japonicus genome version 2.5; http://www. kazusa.or.jp/lotus/), a gene annotated as ketoacyl-(acyl carrier protein) synthase. This co-segregation together with phenotyping of one additional mutant allele obtained through TILLING (Supplementary file 1, [Perry et al., 2003[Perry et al., , 2009) as well as transgenic complementation ( Figure 1A)) confirmed the identification of the mutation causing the dis phenotype of the SL0514 line. The two remaining mutations in the target region were located in a predicted intron of chr4. CM0004.1570.r2.a, a cyclin-like F-box protein (reference position: 40356684) and in a predicted intergenic region (reference position: 40364479). Untranslated regions of DIS and DIS-LIKE were determined using the Ambion FirstChoice RLM RACE kit according to manufacturer's instructions (http://www.ambion.de/). DIS sequence information can be found under the NCBI accession number KX880396.

Identification of RAM2 by map-based cloning and Sanger sequencing
The L. japonicus Gifu mutant reduced and degenerate arbuscules (red, line SL0181-N) resulting from an EMS mutagenesis (Perry et al., 2003(Perry et al., , 2009) was outcrossed to the ecotype MG-20 and previously reported to segregate for two mutations, one on chromosome 1 and one on chromosome 6 (Groth et al., 2013). They were separated by segregation and the mutation on chromosome 1 was previously found in the GRAS transcription factor gene REDUCED ARBUSCULAR MYCORRHIZA 1 (RAM1) (Pimprikar et al., 2016). A plant from the F2 population, which showed wild-type phenotype but was heterozygous for the candidate interval on chromosome 6 and homozygous Gifu for the candidate interval on chromosome 1 was selfed for producing an F3. The F3 generation segregated for only one mutation as 38 out of 132 individuals exhibited the mutant phenotype (c 2 : P(3:1)=0.68). A plant from the F3 population, which displayed wild-type phenotype but was heterozygous for the candidate interval on chromosome 6 was selfed for producing an F4. The F4 generation also segregated for only one mutation as 17 out of 87 individuals exhibited the mutant phenotype (c 2 : P(3:1) =0.76). To identify the mutation on chromosome 6 linked to the previously identified interval (Groth et al., 2013), we employed additional markers for fine mapping in F3 segregating and F4 mutant populations. This positioned the causative mutation between TM0082 and TM0302 (Figure 1-figure supplement 3A). Due to a suppression of recombination in this interval we could not get closer to the mutation and also next generation sequencing (see [Pimprikar et al., 2016] for the methodology) failed to identify a causative mutation. The Medicago truncatula ram2 mutant displays stunted arbuscules similar to our mutant . L. japonicus RAM2 had not been linked to any chromosome but was placed on chromosome 0, which prevented identification of a RAM2 mutation in the target interval on chromosome 6. Therefore, we sequenced the RAM2 gene by Sanger sequencing. Indeed, mutants with stunted arbuscule phenotype in the F3 and F4 generation carried an EMS mutation at base 1663 from G to A leading to amino acid change from Glycine to Glutamic acid, which co-segregated with the mutant phenotype (Figure 1-figure supplement 3B-C). An additional allelic mutant ram2-2 (Figure 1-figure supplement 3B) caused by a LORE1 retrotransposon insertion (Małolepszy et al., 2016) and transgenic complementation with the wildtype RAM2 gene confirmed that the causative mutation affects RAM2 ( Figure 1B). Untranslated regions of RAM2 were determined using the Ambion FirstChoice(R) RLM RACE kit according to manufacturer's instructions (http://www.ambion.de/). A 1345 bp long sequence upstream of ATG was available from the http://www.kazusa.or.jp/lotus/blast.html. To enable cloning a 2275 bp promoter fragment upstream of ATG of RAM2 the remaining upstream sequence of 1047 bp was determined by primer walking on TAC Lj T46c08. L. japonicus RAM2 sequence information can be found under the NCBI accession number KX823334 and the promoter sequence under the number KX823335.

Plasmid generation
Genes and promoter regions were amplified using Phusion PCR according to standard protocols and using primers indicated in Supplementary file 2. Plasmids were constructed as indicated in Supplementary file 3. For localization of DIS in L. japonicus hairy roots the LIII tricolor plasmid (Binder et al., 2014) was used. The plasmid containing 35S:RFP for localization of free RFP in Nicotiana benthamiana leaves was taken from Yano et al. (2008).

Induction of transgenic hairy roots in L. japonicus
Hypocotyls of L. japonicus were transformed with plasmids shown in Supplementary file 3 for hairy root induction using transgenic Agrobacterium rhizogenes AR1193 as described (Takeda et al., 2009).

Floral dipping and rosette growth assay of Arabidopsis thaliana
Five plants per pot were sown. One week before transformation the primary bolt was cut off to induce growth of secondary floral bolts. 5 ml LB culture of A. tumefaciens transformed with a binary vector was incubated at 28˚C, 300 rpm over night. 500 ml of the preculture was added to 250 ml LB medium with appropriate antibiotics. This culture was incubated again at 28˚C, 300 rpm over night until an OD600 of 1.5 was reached. Plants were watered and covered by plastic bags the day before the dipping to ensure high humidity. The cells were harvested by centrifugation (10 min, 5000 rpm) and resuspended in infiltration medium (0.5 x MS medium, 5% sucrose). The resuspended cell culture was transferred to a box and Silwet L-77 was added (75 ml to 250 ml medium). The floral bolts of the plants were dipped into the medium for 5 s and put back into plastic bags and left in horizontal position for one night. After that, plants were turned upright, bags were opened and mature siliques were harvested. For rosette growth assays T3 plants were used. 31 days post sowing the rosettes were photographed and then cut and dried in an oven at 65˚C for the determination of rosette dry weight.

Spatial analysis of promoter activity
For promoter:GUS analysis L. japonicus hairy roots transformed with plasmids containing the DIS and RAM2 promoter fused to the uidA gene and colonized by R. irregularis were subjected to GUS staining as described (Takeda et al., 2009). To correlate DIS and RAM2 promoter activity precisely with the stage of arbuscule development two expression cassettes were combined in the same golden gate plasmid for simultaneous visualization of arbuscule stages and promoter activity. The fungal silhouette including all stages of arbuscule development and pre-penetration apparatuus were made visible by expressing secretion peptide coupled mCherry under the control of the SbtM1 promoter region comprising 704 bp upstream of the SbtM1 gene (Takeda et al., 2009). Promoter activity was visualized using a YFP reporter fused to a nuclear localization signal (NLS).
Transient transformation of N. benthamiana leaves N. benthamiana leaves were transiently transformed by infiltration of transgenic A. tumefaciens AGL1 as described (Yano et al., 2008).

Real time qRT-PCR
For analysis of transcript levels, plant tissues were rapidly shock frozen in liquid nitrogen. RNA was extracted using the Spectrum Plant Total RNA Kit (www.sigmaaldrich.com). The RNA was treated with Invitrogen DNAse I amp. grade (www.invitrogen.com) and tested for purity by PCR. cDNA synthesis was performed with 500 ng RNA using the Superscript III kit (www.invitrogen.com). qRT-PCR was performed with GoTaq G2 DNA polymerase (Promega), 5 x colorless GoTaq Buffer (Promega) and SYBR Green I (Invitrogen S7563, 10.000x concentrated, 500 ml) -diluted to 100x in DMSO. Primers (Supplementary file 2) were designed with primer3 (58). The qPCR reaction was run on an iCycler (Biorad, www.bio-rad.com/) according to manufacturer's instructions. Thermal cycler conditions were: 95˚C 2 min, 45 cycles of 95˚C 30 s, 60˚C/62˚C 30 s and 72˚C 20 s followed by dissociation curve analysis. Expression levels were calculated according to the DDCt method (Rozen and Skaletsky, 2000). For each genotype and treatment three to four biological replicates were tested and each sample was represented by two to three technical replicates.
To collect sequences for phylogeny construction corresponding to potential DIS orthologs, Lotus DIS and KASI (outgroup) protein sequences were searched in genome and transcriptome datasets using BLASTp and tBLASTn respectively. The list of species and the databases used are indicated in Figure 3-source data 1. Hits with an e-value >10 À50 were selected for the phylogenetic analysis. Collected sequences were aligned using MAFFT (http://mafft.cbrc.jp/alignment/server/) and the alignment manually checked with Bioedit. Phylogenetic trees were generated by Neighbor-joining implemented in MEGA5 (Tamura et al., 2011). Partial gap deletion (95%) was used together with the JTT substitution model. Bootstrap values were calculated using 500 replicates.

Microscopy
For quantification of AM colonization in L. japonicus roots a light microscope (Leica) with a 20x magnification was used. For observation of GUS-staining in L. japonicus hairy roots an inverted microscope (Leica DMI6000 B) was used with 10x and 20x magnification. Transformed roots were screened by stereomicroscope (Leica MZ16 FA) using an mCherry fluorescent transformation marker or the pSbtM1:mCherry marker for fungal colonization (for Figure 2A and B). Confocal microscopy (Leica SP5) for WGA-AlexaFluor488 detection using 20x and 63x magnification was performed as described (Groth et al., 2010). Transgenic roots showing mCherry fluorescence signal due to SbtM1 promoter activity linked with fungal colonization were cut into pieces immediately after harvesting. The living root pieces were placed on a glass slide with a drop of water, covered by a cover slip and immediately subjected to imaging. Sequential scanning for the YFP and RFP signal was carried out simultaneously with bright field image acquisition. YFP was excited with the argon ion laser 514 nm and the emitted fluorescence was detected from 525 to 575 nm; RFP was excited with the Diode-Pumped Solid State laser at 561 nm and the emitted fluorescence was detected from 580 to 623 nm. Images were acquired using LAS AF software. Several z-optical sections were made per area of interest and assembled to a z-stack using Fiji. The z-stack movies and 3D projections were produced using the 3D viewer function in Fiji (Schindelin et al., 2012).

Extraction and purification of phospho-and glycoglycerolipids and triacylglycerols
Approximately 50-100 mg of root or leaf material was harvested, weighed and immediately frozen in liquid nitrogen to avoid lipid degradation. The frozen samples were ground to a fine powder before extraction with organic solvents. Total lipids were extracted as described previously (Wewer et al., 2011(Wewer et al., , 2014. Briefly, 1 mL chloroform/methanol/formic acid (1:1:0.1, v/v/v) was added and the sample was shaken vigorously. At this point the internal standards for TAG and fatty acid analysis were added. Phase separation was achieved after addition of 0.5 mL 1M KCl/0.2 M H 3 PO 4 and subsequent centrifugation at 4000 rpm for 5 min. The lipid-containing chloroform phase was transferred to a fresh glass tube and the sample was re-extracted twice with chloroform. The combined chloroform phases were dried under a stream of air and lipids were re-dissolved in 1 mL chloroform to yield the total lipid extract.
For phospho-and glycerolipid analysis 20 ml of the total lipid extract were mixed with 20 ml of the internal standard mix and 160 ml of methanol/chloroform/300 mM ammonium acetate (665:300:35, v/v/v) (Welti et al., 2002). For triacylglycerol analysis 500 ml of the total lipid extract were purified by solid phase extraction on Strata silica columns (1 ml bed volume; Phenomenex) as described (Wewer et al., 2011). TAGs were eluted from the silica material with chloroform, dried under a stream of air and re-dissolved in 1 mL methanol/chloroform/300 mM ammonium acetate (665:300:35, v/v/v).

Extraction and purification of free fatty acids and monoacylglycerol (MAG)
Total lipids were extracted into chloroform and dried as described above. 15-0 FA and a mixture of 15-0 a-MAG and b-MAG were added as internal standard before the extraction. Dried extracts were resuspended in 1 ml n-hexane and applied to silica columns for solid-phase extraction with a n-hexane:diethylether gradient. Free fatty acids were eluted with a mixture of 92:8 (v/v) n-hexane: diethylether as described bevore (Gasulla et al., 2013) and pure diethylether were used for elution of MAG.

Analysis of total fatty acids and free fatty acids by GC-FID
For measurement of total fatty acids, 100 ml of the total lipid extract were used. For measurement of free fatty acids, the SPE-fraction containing free fatty acids was used. Fatty acid methyl esters (FAMEs) were generated from acyl groups of total lipids and free fatty acids by addition of 1 mL 1N methanolic HCL (Sigma) to dried extracts and incubation at 80˚C for 30 min (Browse et al., 1986). Subsequently, FAMEs were extracted by addition of 1 mL n-hexane and 1 mL of 0.9% (w/v) NaCl and analyzed on a gas chromatograph with flame-ionization detector (GC-FID, Agilent 7890A PlusGC). FAMEs were separated on an SP 2380 fused silica GC column (Supelco, 30 mx 0.53 mm, 0.20 mm film) as described (Wewer et al., 2013), with a temperature -gradient starting at 100˚C, increased to 160˚C with 25˚C/min, then to 220˚C with10˚C/min and reduced to 100˚C with 25˚C/ min. FAMEs were quantified in relation to the internal standard pentadecanoic acid (15:0).

Quantification of glycerolipids by Q-TOF MS/MS
Phosphoglycerolipids (PC, PE, PG, PI, PS), glycoglycerolipids (MGDG, DGDG, SQDG) and triacylglycerol (TAG) were analyzed in positive mode by direct infusion nanospray Q-TOF MS/MS on an Agilent 6530 Q-TOF instrument as described previously Gasulla et al., 2013). A continuous flow of 1 ml/min methanol/chloroform/300 mM ammonium acetate (665:300:35, v/v/v) (Welti et al., 2002) was achieved using a nanospray infusion ion source (HPLC/chip MS 1200 with infusion chip). Data are displayed as X:Y, where X gives the number of C atoms of the fatty acid chain and Y the amount of desaturated carbo-carbon bonds inside that fatty acid chain.

Internal standards
Internal standards for phospho-and glycoglycerolipid analysis were prepared as described previously (Gasulla et al., 2013;Wewer et al., 2014). The following standards were dissolved in 20 ml of

Data availability
Lunularia cruciata: For this species, the raw RNAseq reads have been previously deposited to NCBI under the accession number SRR1027885. It is annotated with Rhizophagus irregularis (10% of sequences) as the transcriptome was partly prepared from Lunularia plant tissue colonized by the fungus Rhizophagus irregularis. The corresponding Lunularia transcriptomic assembly is available at www.polebio.lrsv.ups-tlse.fr/Luc_v1/

Statistics
All statistical analyses (Source code 1) were performed and all boxplots were generated in R (www. r-project.org).
Supervision, Funding acquisition, Investigation, Writing-original draft, Project administration, Writing-review and editing