TY - JOUR
AU1 - Horst, Robin J.
AU2 - Doehlemann, Gunther
AU3 - Wahl, Ramon
AU4 - Hofmann, Joݶrg
AU5 - Schmiedl, Alfred
AU6 - Kahmann, Regine
AU7 - Kaݶmper, Joݶrg
AU8 - Sonnewald, Uwe
AU9 - Voll, Lars M.
AB - Abstract The basidiomycete Ustilago maydis is the causal agent of corn smut disease and induces tumor formation during biotrophic growth in its host maize (Zea mays). We have conducted a combined metabolome and transcriptome survey of infected leaves between 1 d post infection (dpi) and 8 dpi, representing infected leaf primordia and fully developed tumors, respectively. At 4 and 8 dpi, we observed a substantial increase in contents of the nitrogen-rich amino acids glutamine and asparagine, while the activities of enzymes involved in primary nitrogen assimilation and the content of ammonia and nitrate were reduced by 50% in tumors compared with mock controls. Employing stable isotope labeling, we could demonstrate that U. maydis-induced tumors show a reduced assimilation of soil-derived 15NO3 ™ and represent strong sinks for nitrogen. Specific labeling of the free amino acid pool of systemic source leaves with [15N]urea revealed an increased import of organic nitrogen from systemic leaves to tumor tissue, indicating that organic nitrogen provision supports the formation of U. maydis-induced tumors. In turn, amino acid export from systemic source leaves was doubled in infected plants. The analysis of the phloem amino acid pool revealed that glutamine and asparagine are not transported to the tumor tissue, although these two amino acids were found to accumulate within the tumor. Photosynthesis was increased and senescence was delayed in systemic source leaves upon tumor development on infected plants, indicating that the elevated sink demand for nitrogen could determine photosynthetic rates in source leaves. Plant pathogens have evolved different strategies to colonize their plant hosts. While necrotrophic pathogens rapidly kill plant tissue, usually by the secretion of highly efficient toxins and cell wall-degrading enzymes (van Kan, 2006), and thrive on the dead plant material, biotrophic pathogens strictly rely on living tissue to survive and complete their life cycle (Divon and Fluhr, 2007). Ustilago maydis, the causal agent of corn smut disease, is a biotrophic basidiomycete parasitizing maize (Zea mays) and its natural ancestor teosinte. It can induce the formation of tumors on all aerial organs (Banuett, 1995), resulting in stunted growth and yield losses (Martinez-Espinoza et al., 2002). U. maydis shows a dimorphic lifestyle (Kahmann and Kaݶmper, 2004): while haploid sporidia are not infectious and grow saprophytically in a yeast-like manner, filamentous growth is initiated upon mating of two compatible sporidia on the plant surface. Filamentous hyphae form appressoria and directly penetrate host cells. Immediately upon host entry, the biotrophic interaction with intracellular fungal proliferation is initiated. About 4 d after penetration, the formation of hypertrophic host cells and concomitant tumor development are induced, while the fungal hyphae start proliferating in the apoplastic spaces that develop as a consequence of cell wall degradation and induced host cell enlargement (Doehlemann et al., 2008a, 2008b). In infections by smut fungi, the plant plasma membrane gets invaginated and encases the growing hyphae (Doehlemann et al., 2009). This generates the so-called biotrophic interface, a compartment where fungal secretion leads to the formation of a vesicular matrix that comprises the enlarged contact zone typically found for members of the Ustilaginomycetes (Bauer et al., 1997; Begerow et al., 2006). The hyphae of Ustilago species often grow along the vasculature (Doehlemann et al., 2008b, 2009) that contains high concentrations of assimilates and nutrients (Lohaus et al., 1998, 2000). In general, infection sites of biotrophic fungi represent strong local metabolic sinks that drain nutrients from the host environment. Evidence obtained for the rust fungus Uromyces fabae suggests that nutrients are mainly taken up as hexoses (generated by secreted fungal invertase) and amino acids (Hahn et al., 1997; Voegele et al., 2001; Struck et al., 2002, 2004). Very recently, a novel high-affinity U. maydis Suc transporter, Srt1, was characterized that is required for full virulence (R. Wahl, K. Wippel, J. Kaݶmper, and N. Sauer, unpublished data). Although U. maydis can infect all aerial parts of the plant, it has a high specificity for meristematic tissues (Wenzler and Meins, 1987), which represent sink organs and are dependent on the import of assimilates from source organs (i.e. germinating seeds or fully developed leaves in adult plants). The tumors that develop in infected leaves often span the entire leaf blade. Such leaf infections first hamper the establishment of C4 photosynthesis, which results in reduced CO2 assimilation upon tumor initiation (Horst et al., 2008). During tumor development, a further reduction in overall photosynthetic capacity of infected leaves is observed. Consequently, soluble carbohydrate accumulation in tumors is similar to that in young sink leaves (Doehlemann et al., 2008a; Horst et al., 2008). The role of nitrogen metabolism in plant-pathogen interactions has not been investigated very intensely to date. There have been conflicting reports on whether plant-pathogenic fungi encounter nitrogen limitation in planta. Amino acid uptake transporters (Hahn et al., 1997; Struck et al., 2002, 2004; Divon et al., 2005; Takahara et al., 2009) and genes for the biosynthesis of major (Gln synthetase [GS]; Stephenson et al., 1997) and minor (Namiki et al., 2001; Both et al., 2005; Takahara et al., 2009) amino acids are induced during early plant colonization by most (hemi)biotrophs, indicating uptake and metabolization of organic nitrogen in planta by the intruder. Nitrate-nonutilizing mutants of various fungal (hemi)biotrophs, such as U. maydis and Magnaporthe grisea (Lau and Hamer, 1996; R.J. Horst, G. Doehlemann, R. Wahl, J. Hofmann, A. Schmiedl, R. Kahmann, J. Kaݶmper, U. Sonnewald, and L.M. Voll, unpublished data), did not exhibit any reduction in pathogenicity, indicating that nitrate is not essential for these pathogens in planta. U. maydis exhibits the genetic equipment to synthesize all amino acids starting from inorganic nitrate (McCann and Snetselaar, 2008). Therefore, it should be able to use any nitrogen source that is available in maize leaves. While nitrate reductase knockout mutants are fully pathogenic on maize leaves (R.J. Horst, G. Doehlemann, R. Wahl, J. Hofmann, A. Schmiedl, R. Kahmann, J. Kaݶmper, U. Sonnewald, and L.M. Voll, unpublished data), nitrogen-auxotrophic mutants of U. maydis are reportedly unable to complete their infection cycle (Holliday, 1961). Similarly, a His-auxotrophic mutant of the hemibiotroph M. grisea (Sweigard et al., 1998) and an Arg-auxotrophic mutant of the hemibiotroph Fusarium oxysporum (Namiki et al., 2001) also exhibit reduced virulence, indicating the necessity for the biosynthesis of minor amino acids that are not readily available in planta. In addition, the loss of AreA/NiT2 transcription factor homologs that coordinate the utilization of nitrogen sources via nitrogen catabolite repression in filamentous fungi (Marzluf, 1997) resulted in attenuated pathogenicity in the respective mutants of F. oxysporum, Cladosporium fulvum, and Colletotrichum lindemuthianum (Pellier et al., 2003; Divon et al., 2006; Thomma et al., 2006). This indicates that virulence genes are regulated by AreA-like transcription factors. Is there physiological evidence for nitrogen limitation of fungal pathogens in planta? On the one hand, overfertilization of plants with nitrogen can lead to an increased susceptibility to fungal pathogens (Jensen and Munk, 1997; Hoffland et al., 2000; Agrios, 2005). For instance, the infection index of field-grown maize with U. maydis correlates with the amount and the timing of nitrogen application (Kostandi and Soliman, 1991). On the other hand, plants grown under nitrogen limitation often show increased susceptibility to pathogen infection, most likely caused by reduced general fitness (Snoeijers et al., 2000; Solomon et al., 2003). On the physiological level, free amino acid concentrations in the leaf apoplastic fluids of maize are up to 1.3 mm in maize, compared with apoplastic Suc contents of up to 2.6 mm (Lohaus et al., 2000). In addition, apoplastic amino acid concentrations even increased upon infection of tomato (Solanum lycopersicum) leaves with C. fulvum (Solomon and Oliver, 2001). In pea (Pisum sativum) leaves infected by powdery mildew, the transfer rate of radiolabeled Gln into fungal mycelium was found to be as high as 50% of the transfer rate of Glc (Clark and Hall, 1998). This indicates a similar capacity for sugar and amino acid uptake into haustoria. In summary, these observations suggest that nitrogen provision to apoplast-resident pathogens is not limited. However, nitrogen limitation for limited time periods cannot be excluded (e.g. during early pathogenic development on the host surface, when fungal cells depend on their own carbon and nitrogen reserves; for summary, see Solomon et al., 2003). In maize, nitrogen uptake in the roots preferentially occurs in the form of nitrate, which is then transported to the leaves, where it is reduced and assimilated into organic forms (Oaks, 1994). Apart from the presence of several systematic studies on nitrogen remobilization in maize leaves (Hirel et al., 2005; Gallais et al., 2006, 2007; Martin et al., 2006), the analysis of mutants of cytosolic GSs (gs1-3 and gs1-4) has identified Gln as the major route of nitrogen export to growing ears, which represent a strong sink for nitrogen (Martin et al., 2006). This work provides a systematic study of the dynamics in nitrogen metabolism during the interaction of maize with U. maydis. We address (1) the impact of U. maydis-induced tumor formation on local nitrogen metabolism, (2) its effect on nitrogen allocation in infected shoots, and (3) the impact of tumor presence on the performance of systemic source leaves. RESULTS Metabolome Analysis of Developing Tumors We have conducted a combined transcriptome and metabolome analysis of infected leaf tissue at different time points after infection. Based on this data set, we previously described that U. maydis achieves a swift suppression of defense-related genes during the interaction and that photosynthetic gene expression is progressively reduced in infected leaves (Doehlemann et al., 2008a). In this report, we focus on the insights obtained from the corresponding metabolome data set. Targeted metabolite analysis was performed for major carbohydrates, amino acids, antioxidants, phosphorylated intermediates, and organic acids at 12 h, 24 h, 4 d, 4.5 d, and 8 d after leaf infection with U. maydis in three independent experiments. Since our analysis was performed on infected leaf material, representing both host and fungal tissue, a prerequisite was to estimate the contribution of fungal cells to total extracted tissue. Assuming that the amount of fungal cells increases during infection, samples taken at 8 d post infection (dpi) were analyzed to examine the maximal portion of U. maydis in infected leaf tissue. While quantification of fungal genomic DNA by real-time PCR (see Supplemental Materials and Methods S1) indicated approximately equal amounts of fungal and host genome copies in the samples (data not shown), volume analysis of fluorescently labeled fungal and host cells in three-dimensional reconstructions of confocal image stacks revealed that only 2.3% of the total sample volume was of fungal origin (for a representative three-dimensional reconstruction, see Supplemental Movie S1). Comparing the data sets, the volume-nucleus ratio of the multinucleate fungal cells appears to be overestimated by real-time PCR analysis. As total fungal cell volume, but not the number of fungal nuclei, is relevant for estimating the pathogen's contribution to metabolite contents of infected leaf tissue, we conclude that the amount of fungal material in the analyzed samples is largely negligible with respect to the conducted metabolite analysis. A principal component analysis of all surveyed infection stages revealed that two major principal components coincide with leaf development (PC1, 40.7%) and tumor development (PC2, 24.5%; Fig. 1, A and B Figure 1. Open in new tabDownload slide Principal component analysis of metabolite data from developing U. maydis-induced tumors between 0.5 dpi (leaf primordia) and 8 dpi (fully developed tumors). Metabolite data from infected and control leaves were obtained (n = 9–12) from three independent experiments, and the mean values were analyzed with the Markerview software as described in “Materials and Methods” using the autoscale option for scaling. A, Principal component analysis of metabolite data from all time points (12 h, 24 h, 2 d, 4 d, 4.5 d, and 8 dpi). Plotted is PC2 (24.5%) against PC1 (40.7%). PC1 correlates with leaf development in mock control leaves, while PC2 discriminates tumor formation at late infection time points. B, Loadings of the individual metabolites on PC1 and PC2 from all time points analyzed. C, Principal component analysis of metabolite data from late infection time points 4 and 8 dpi. PC1 correlates with tumor formation, whereas PC2 discriminates the time of day that the samples were taken. D, Metabolite loadings of PC1 plotted against metabolite loadings of PC2 for the data depicted in C. AA, Amino acid; Asc, ascorbate; Cit, citrate; F6P, Fru-6-P; Frc, Fru; Fum, fumarate; G1P, Glc-1-P; G6P, Glc-6-P; gEC, γ-glutamylcysteine; GSH, glutathione; Icit, isocitrate; 2OG, 2-oxoglutarate; PEP, phosphoenolpyruvate; 3PG, 3-phosphoglycerate; 6PG, 6-phosphogluconate; Pyr, pyruvate; Ru15BP, ribulose-1,5-bisP; Shik, shikimate; Succ, succinate; T6P, trehalose-6-P; aToc, α-tocopherol; gToc, γ-tocopherol; Toc, total tocopherol. Figure 1. Open in new tabDownload slide Principal component analysis of metabolite data from developing U. maydis-induced tumors between 0.5 dpi (leaf primordia) and 8 dpi (fully developed tumors). Metabolite data from infected and control leaves were obtained (n = 9–12) from three independent experiments, and the mean values were analyzed with the Markerview software as described in “Materials and Methods” using the autoscale option for scaling. A, Principal component analysis of metabolite data from all time points (12 h, 24 h, 2 d, 4 d, 4.5 d, and 8 dpi). Plotted is PC2 (24.5%) against PC1 (40.7%). PC1 correlates with leaf development in mock control leaves, while PC2 discriminates tumor formation at late infection time points. B, Loadings of the individual metabolites on PC1 and PC2 from all time points analyzed. C, Principal component analysis of metabolite data from late infection time points 4 and 8 dpi. PC1 correlates with tumor formation, whereas PC2 discriminates the time of day that the samples were taken. D, Metabolite loadings of PC1 plotted against metabolite loadings of PC2 for the data depicted in C. AA, Amino acid; Asc, ascorbate; Cit, citrate; F6P, Fru-6-P; Frc, Fru; Fum, fumarate; G1P, Glc-1-P; G6P, Glc-6-P; gEC, γ-glutamylcysteine; GSH, glutathione; Icit, isocitrate; 2OG, 2-oxoglutarate; PEP, phosphoenolpyruvate; 3PG, 3-phosphoglycerate; 6PG, 6-phosphogluconate; Pyr, pyruvate; Ru15BP, ribulose-1,5-bisP; Shik, shikimate; Succ, succinate; T6P, trehalose-6-P; aToc, α-tocopherol; gToc, γ-tocopherol; Toc, total tocopherol. ). Metabolites related to (C4) photosynthesis (i.e. pyruvate, phosphoenolpyruvate, malate, and 3-phosphoglycerate) had the strongest loading on PC1. These metabolites accumulate upon the establishment of photosynthesis in the developing leaf, which is not observed in infected leaves (Fig. 2C Figure 2. Open in new tabDownload slide Metabolite analysis of U. maydis-induced leaf tumors. Time courses are shown for metabolite contents in developing leaf tumors (gray) and control leaves (black) at 1, 2, 4, and 8 dpi of 7-d-old maize plants. Samples were taken 1 h before the end of the light period. A, Contents of amino acids. B, Contents of carbohydrates. C, Contents of phosphorylated intermediates and organic acids. The shaded areas represent se (n = 9–12). Figure 2. Open in new tabDownload slide Metabolite analysis of U. maydis-induced leaf tumors. Time courses are shown for metabolite contents in developing leaf tumors (gray) and control leaves (black) at 1, 2, 4, and 8 dpi of 7-d-old maize plants. Samples were taken 1 h before the end of the light period. A, Contents of amino acids. B, Contents of carbohydrates. C, Contents of phosphorylated intermediates and organic acids. The shaded areas represent se (n = 9–12). ). For PC2, no distinct group of metabolites with particularly high loading could be defined. To this end, a more refined principal component analysis was performed, including only those time points at which tumor development had considerably progressed (4, 4.5, and 8 dpi; Fig. 1C). Here, the two major principal components correlated with U. maydis infection (PC1, 54.3%) and the time of day at which the material was harvested (PC2, 18.6%): 4- and 8-dpi samples were taken at the end of the light period, and 4.5-dpi samples were taken after the dark period. This analysis showed that the amino acids Gln, Phe, Tyr, His, and Thr as well as hexose phosphates strongly load onto PC1 (Fig. 1D). These metabolites remained constantly high in tumors, while their contents dropped during development of control leaves (Fig. 2A). Furthermore, a significant increase of total amino acids (i.e. Asn, Pro, Val, and Ile) and soluble sugars (Glc, Fru, and Suc) was observed during tumor development between 4 and 8 dpi (Fig. 2) that positively loaded on PC2 (Fig. 1D). Organic Nitrogen Accumulates in Tumors Measurement of free amino acid contents in maize leaves infected with U. maydis showed that the total free amino acid pool in tumors is elevated during the entire infection process (Fig. 2A), reaching 13.6 ± 0.6 μmol g™1 fresh weight in tumors at 8 dpi compared with 10.4 ± 0.04 μmol g™1 fresh weight in mock-infected leaves at 8 dpi. The contents of nearly all proteinogenous amino acids decreased during normal leaf development, except for Ala and Cys, which accumulate in mature leaves and Asp, Glu, and Pro that exhibit constant levels (Fig. 2A). In contrast to the situation in mock-infected leaves, the contents of most free amino acids remained high or increased progressively during tumor development in infected leaves. Amino acids with a high nitrogen-carbon ratio were particularly abundant in tumors at 8 dpi. At this time point, the content of Asn was increased more than 3-fold compared with 4 dpi, while Arg contents rose steadily throughout the infection process and Gln contents remained constantly high at all time points analyzed (Fig. 2A). The comparison of the amino acid pool composition in tumors with fully developed control leaves (source) and very young leaves (sink) revealed that the tumor tissue strongly resembles juvenile sink leaves in this respect. The amino acid pool composition of sink leaves and tumors significantly differed from that of fully developed source leaves (Supplemental Fig. S1). Primary Nitrogen Assimilation Is Down-Regulated in Tumors To resolve whether the elevated organic nitrogen supply in tumors derives (1) from increased local primary nitrogen assimilation or (2) from stimulated import of amino acids from noninfected systemic leaves, we assessed transcript levels and activities of enzymes directly involved in primary nitrogen assimilation as well as the content of inorganic nitrogen forms in tumors. Analysis of the complementary microarray data set (Doehlemann et al., 2008a) showed transcript levels for all enzymes involved in primary nitrogen assimilation as down-regulated in tumors between 4- and 13-fold at 8 dpi compared with mock-infected leaves (Fig. 3A Figure 3. Open in new tabDownload slide Transcript and metabolite data mapped onto the primary nitrogen assimilation pathway of maize. A, Overview of the primary nitrogen assimilation pathway. Metabolite data are shown from control leaves (black bars) and infected leaves (white bars) at 4 dpi (left) and 8 dpi (right). Error bars represent se (n = 9–12). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). The fold changes in transcript abundance of the respective genes at 4 dpi (top) and 8 dpi (bottom) are presented next to the arrows connecting the metabolites. AsnS2/3, Asn synthetase isoform 2/3; Asp-AT, Asp aminotransferase; Fd-GOGAT, ferredoxin-dependent Glu synthase; Fd-NiR, ferredoxin-dependent nitrite reductase; FW, fresh weight; GS2, plastidic GS; NAR1S, nitrate reductase; Nrt1.1, nitrate transporter. B, Activities of enzymes involved in nitrogen assimilation. Left, maximal nitrate reductase activity (in vivo inhibitory proteins are removed by addition of EDTA to the reaction buffer); middle, selective nitrate reductase activity (reflects the in vivo active nitrate reductase); right, GS activity. Error bars represent se (n = 6). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). Figure 3. Open in new tabDownload slide Transcript and metabolite data mapped onto the primary nitrogen assimilation pathway of maize. A, Overview of the primary nitrogen assimilation pathway. Metabolite data are shown from control leaves (black bars) and infected leaves (white bars) at 4 dpi (left) and 8 dpi (right). Error bars represent se (n = 9–12). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). The fold changes in transcript abundance of the respective genes at 4 dpi (top) and 8 dpi (bottom) are presented next to the arrows connecting the metabolites. AsnS2/3, Asn synthetase isoform 2/3; Asp-AT, Asp aminotransferase; Fd-GOGAT, ferredoxin-dependent Glu synthase; Fd-NiR, ferredoxin-dependent nitrite reductase; FW, fresh weight; GS2, plastidic GS; NAR1S, nitrate reductase; Nrt1.1, nitrate transporter. B, Activities of enzymes involved in nitrogen assimilation. Left, maximal nitrate reductase activity (in vivo inhibitory proteins are removed by addition of EDTA to the reaction buffer); middle, selective nitrate reductase activity (reflects the in vivo active nitrate reductase); right, GS activity. Error bars represent se (n = 6). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). ). Except for nitrate reductase (Nar1S), all the other genes were already down-regulated early during tumor development (4 dpi). Consistently, these transcriptional changes correlate with substantial reductions in the extractable enzyme activity of nitrate reductase (maximal and selective activity) as well as total GS in tumors at 4 and 8 dpi (Fig. 3B). Since all four cytosolic GS isoforms represented on the maize Genechip (gs1-1, gs1-2, gs1-4, and gs1-5) were not transcriptionally regulated upon infection with U. maydis, this drop in activity can be attributed to the plastidic GS2, which is involved in primary nitrogen assimilation in young leaves (Becker et al., 2000; Martin et al., 2006). Similarly, the contents of the inorganic nitrogen compounds nitrate and ammonium were also reduced in tumors, indicating a reduced availability of inorganic nitrogen (Fig. 3A). Despite the apparent reduction of the capacity for inorganic nitrogen assimilation in tumors, Asp aminotransferase (Asp-AT), an indicator of high nitrogen availability (Lam et al., 1996), and two isoforms of Asn synthetase (AsnS) were induced at the transcriptional level compared with controls at 4 and 8 dpi (Fig. 3A). This indicates stimulated transformation of organic nitrogen into Asn. Consequently, the contents of Glu and Asp remained unchanged, while Gln and Asn accumulated (see above; Fig. 3A). Taken together, we observed diminished availability of inorganic nitrogen and a reduced capacity for primary nitrogen assimilation in tumors on the one hand and elevated organic nitrogen content on the other. This discrepancy suggests that the primary nitrogen assimilation is not solely responsible for the accumulation of organic nitrogen in tumors. Uptake and Distribution of Nitrate from the Soil Since nitrate assimilation in young maize plants occurs predominantly in leaves (Oaks, 1992, 1994), we aimed at gathering direct experimental evidence demonstrating a reduction of nitrate assimilation in tumors. At 8 dpi, U. maydis-infected as well as mock control plants were watered with 15NO3 ™, and 15N uptake into tumor tissue was quantified during a 48-h time course. This experiment showed a reduced incorporation of 15N into the total nitrogen pool in tumor tissue relative to control leaves (Fig. 4A Figure 4. Open in new tabDownload slide Incorporation kinetics of nitrogen originating from 15NO3 ™ into different pools of nitrogen-containing compounds. Plants were watered with 40 mL of 20 mm K15NO3 (containing a molar ratio of 15N/14N of 0.2) at 8 dpi, and samples were taken at the time points indicated. Black lines represent control plants, and gray lines represent infected plants. A to C, Incorporation of 15N into the total nitrogen pool (A), into the pool of free amino acids (AA; B), and into protein-bound amino acids (C) in percentage of total nitrogen. The shaded areas represent se (n = 4). D, Allocation of 15N derived from soil nitrate to tumors. The allocation of 15N to fourth leaves of infected plants bearing tumors (right) or healthy control leaves (left) at 48 h after treatment with 15NO3 ™ relative to the total amount of 15N retrieved in all aerial organs is shown. Error bars represent se (n = 4). Figure 4. Open in new tabDownload slide Incorporation kinetics of nitrogen originating from 15NO3 ™ into different pools of nitrogen-containing compounds. Plants were watered with 40 mL of 20 mm K15NO3 (containing a molar ratio of 15N/14N of 0.2) at 8 dpi, and samples were taken at the time points indicated. Black lines represent control plants, and gray lines represent infected plants. A to C, Incorporation of 15N into the total nitrogen pool (A), into the pool of free amino acids (AA; B), and into protein-bound amino acids (C) in percentage of total nitrogen. The shaded areas represent se (n = 4). D, Allocation of 15N derived from soil nitrate to tumors. The allocation of 15N to fourth leaves of infected plants bearing tumors (right) or healthy control leaves (left) at 48 h after treatment with 15NO3 ™ relative to the total amount of 15N retrieved in all aerial organs is shown. Error bars represent se (n = 4). ). However, saturation of the nitrogen pool with 15N was not reached in both conditions. In contrast, 15N incorporation into the free amino acid pool reached saturation as early as 10 h after treatment with 15NO3 ™ in control plants and remained at this level throughout the experiment (Fig. 4B). Incorporation of 15N into the free amino acid pool of tumor tissue was substantially reduced and did not reach saturation during the entire experiment. This is in line with our observation that the contents of most free amino acids increased 2- to 5-fold during the first 12 h after 15NO3 ™ application in control leaves, while the free amino acid pools remained fairly constant in tumors (Supplemental Fig. S2). In tumors, the level of 15N in the free amino acid pool dropped during the dark period, which was not observed in control leaves. Incorporation of 15N into proteins followed a linear rate in control leaves and in tumors, but the 15N incorporation into proteins was reduced in infected leaves (Fig. 4C), which could be attributed to the decreased level of overall 15N labeling in tumors. To directly assess the rate of protein biosynthesis in fully developed tumors, we determined the incorporation of [35S]Met into the protein fraction in tumors and control leaves at 8 dpi. In control leaves, the ratio of the recovery of 35S in the protein fraction relative to 35S in the free amino acid pool (0.14 ± 0.04) was significantly lower than in tumors (0.5 ± 0.1). This suggests a higher rate of amino acid incorporation into proteins in tumors compared with healthy leaves. Analysis of protein biosynthesis-related transcripts suggests that cytosolic protein biosynthesis of tumor cells is up-regulated while plastidic protein biosynthesis is down-regulated (Supplemental Fig. S3). In summary, our data suggest that the evident accumulation of organic nitrogen in tumors is not entirely fueled by local primary nitrogen assimilation but most likely relies on the import of reduced nitrogen compounds from systemic, noninfected leaves. The observed drop of 15N labeling in the free amino acid pool of tumors during the night might even reflect the contribution of organic nitrogen import from systemic plant organs. Tumors Represent Strong Sinks for N After labeling with 15NO3 ™, we observed a reduced 15N uptake rate of systemic leaves in infected plants compared with control plants (data not shown). This indicates that, despite their diminished capacity for nitrogen assimilation, tumors represent a strong sink for nitrogen at the whole plant level. To verify this assumption, we calculated the systemic allocation of 15N in infected plants bearing tumors on leaf 4 (see “Materials and Methods” and final figure). At 9 dpi, tumor tissue constituted approximately 40% of the total shoot weight, whereas the corresponding leaf of a healthy plant amounted to maximum 15% of total shoot weight. On the one hand, this increase can be attributed to the reduced total shoot biomass of the infected plants compared with healthy plants; on the other hand, tumors exhibited a strongly increased total weight compared with normal leaf tissue: leaf segments carrying tumors had four to five times more biomass than healthy leaves of the same segment length. Consequently, when regarding the distribution of nitrogen among the entire shoot, the allocation of nitrogen to tumors was two to three times increased compared with the corresponding leaf of a mock-infected plant (Fig. 4D), even though primary nitrogen assimilation was reduced in tumors. We also assessed the influence of tumor development on assimilate supply to and metabolism in upper systemic sink leaves, but only a few changes were observed relative to controls (Table I Table I. Contents of selected amino acids and sugars from young, upper systemic sink leaves with no infection symptoms Sugars comprise Glc, Fru, and Suc. se values are indicated (n = 10–12), and statistically significant differences are marked by asterisks (Welch-Satterthwaite t test; P < 0.05). Sample . Total Amino Acids . Asn . Asp . Gln . Glu . Sugars . μmol g™1 fresh wt Control 13.8 ± 1.1 236 ± 26 1.5 ± 0.2 282 ± 21 3.0 ± 0.2 34.3 ± 2.8 Infected 11.3 ± 0.7 134 ± 19* 0.8 ± 0.1* 156 ± 19* 2.8 ± 0.2 27.2 ± 1.6* Sample . Total Amino Acids . Asn . Asp . Gln . Glu . Sugars . μmol g™1 fresh wt Control 13.8 ± 1.1 236 ± 26 1.5 ± 0.2 282 ± 21 3.0 ± 0.2 34.3 ± 2.8 Infected 11.3 ± 0.7 134 ± 19* 0.8 ± 0.1* 156 ± 19* 2.8 ± 0.2 27.2 ± 1.6* Open in new tab Table I. Contents of selected amino acids and sugars from young, upper systemic sink leaves with no infection symptoms Sugars comprise Glc, Fru, and Suc. se values are indicated (n = 10–12), and statistically significant differences are marked by asterisks (Welch-Satterthwaite t test; P < 0.05). Sample . Total Amino Acids . Asn . Asp . Gln . Glu . Sugars . μmol g™1 fresh wt Control 13.8 ± 1.1 236 ± 26 1.5 ± 0.2 282 ± 21 3.0 ± 0.2 34.3 ± 2.8 Infected 11.3 ± 0.7 134 ± 19* 0.8 ± 0.1* 156 ± 19* 2.8 ± 0.2 27.2 ± 1.6* Sample . Total Amino Acids . Asn . Asp . Gln . Glu . Sugars . μmol g™1 fresh wt Control 13.8 ± 1.1 236 ± 26 1.5 ± 0.2 282 ± 21 3.0 ± 0.2 34.3 ± 2.8 Infected 11.3 ± 0.7 134 ± 19* 0.8 ± 0.1* 156 ± 19* 2.8 ± 0.2 27.2 ± 1.6* Open in new tab ; Supplemental Fig. S4). Nevertheless, contents of total soluble carbohydrates were reduced by approximately 20%, while contents of Asn, Asp, Arg, Pro, and Gln were substantially lowered between 40% and 50% in upper sink leaves of infected plants compared with the same leaves of mock-infected plants. The reduced accumulation of carbon and, especially, nitrogen assimilates supports the hypothesis that import of assimilates into upper systemic leaves is reduced upon the establishment of the tumor as a strong additional sink organ. Reallocation of Organic Nitrogen from Systemic Leaves As suggested by our previous results, we next investigated whether the export of organic nitrogen compounds from systemic source leaves toward U. maydis-induced tumors was increased. The organic nitrogen pool of the source leaf below the tumors (leaf 3 when leaf 4 was infected; see final figure) was labeled by [15N]urea at 8 dpi. Thirty hours after treatment, the reallocation of 15N between partitions of the maize shoot was analyzed comparing (1) infected and corresponding control leaves (leaf 4), (2) the two leaves below the labeled leaf (leaves 1 and 2), and (3) the younger (upper) systemic leaves above the infection site (for illustration, see final figure). Export of organic nitrogen to the roots was not assessed. The recovery of total exported nitrogen in tumors was increased approximately 3-fold compared with corresponding control leaves from mock-infected plants, indicating an increased import of organic nitrogen from lower source leaves into the tumors (Fig. 5A Figure 5. Open in new tabDownload slide Incorporation of nitrogen after application of [15N]urea to lower systemic source leaves at 8 dpi. Leaf 3 (no infection symptoms) was treated with 100 μL of 200 mm [15N]urea, and the entire shoot was sampled at 30 h after treatment in partitions as described in the text and below. A, Distribution of nitrogen exported from the labeled leaf to the rest of the shoot. Values were corrected against the 15N enrichment in leaf 3, which was determined prior to sample preparation of the other shoot parts. Black represents infected leaf or corresponding leaf from control plants (leaf 4), dark gray represents young, upper systemic leaves, and light gray represents lower systemic leaves (leaves 1 and 2). B, Accumulation of 15N in amino acid (AA) pools of infected leaves (gray bars) and control leaves (black bars) 30 h after labeling. Error bars represent se (n = 4). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). FW, Fresh weight. Figure 5. Open in new tabDownload slide Incorporation of nitrogen after application of [15N]urea to lower systemic source leaves at 8 dpi. Leaf 3 (no infection symptoms) was treated with 100 μL of 200 mm [15N]urea, and the entire shoot was sampled at 30 h after treatment in partitions as described in the text and below. A, Distribution of nitrogen exported from the labeled leaf to the rest of the shoot. Values were corrected against the 15N enrichment in leaf 3, which was determined prior to sample preparation of the other shoot parts. Black represents infected leaf or corresponding leaf from control plants (leaf 4), dark gray represents young, upper systemic leaves, and light gray represents lower systemic leaves (leaves 1 and 2). B, Accumulation of 15N in amino acid (AA) pools of infected leaves (gray bars) and control leaves (black bars) 30 h after labeling. Error bars represent se (n = 4). Statistically significant changes are indicated with asterisks (Welch-Satterthwaite t test; P < 0.05). FW, Fresh weight. ). In turn, less of the exported nitrogen was recovered in upper systemic leaves of infected plants. However, the allocation of nitrogen from leaf 3 to the two older leaves was not altered upon infection. An analysis of the total pool size of 15N-labeled amino acids revealed that tumors accumulated nearly five times more labeled amino acids than the corresponding leaves from control plants (Fig. 5B) on a fresh weight basis. Considering the elevated total fresh weight of the tumors compared with control leaves, tumors accumulate 10 times more free amino acids compared with corresponding control leaves (data not shown). Furthermore, healthy leaves mainly accumulated [15N]Glu (Fig. 5B) and [15N]Ala (data not shown), indicating that 15N label is finally retrieved in amino acids whose pools are subject to a high turnover in photosynthetically active maize leaves. In contrast, tumors accumulated mainly [15N]Asn as well as [15N]Gln and [15N]Glu (Fig. 3B), which likely relates to high rates of overall amino acid import. Taken together, these data suggest that tumors rely on the import of organic nitrogen from noninfected, systemic source leaves. This, in turn, implies a higher export rate of these compounds from systemic leaves. Export of Assimilates from Systemic Leaves Increases upon Infection To test whether lower source leaves from infected plants (with tumors on leaf 4) export more amino acids than the corresponding leaves from control plants, phloem exudates were collected from leaf 3. Exudates were collected from leaves pretreated with urea 1 d prior to sampling to simulate the conditions of the [15N]urea-labeling experiment (high nitrogen availability). To rule out artifacts caused by this treatment, exudates were also collected from nontreated leaves (normal nitrogen availability). Under both experimental conditions, the amino acid exudation rate of leaf 3 from infected plants was about 2-fold increased compared with the exudation rate of leaf 3 from control plants (Table II Table II. Phloem exudation rate and amino acid composition of phloem exudate collected from leaf 3 of plants infected with U. maydis (leaf 4 harbored tumors) or from control plants at 9 dpi The experiment was conducted under normal (no urea treatment; left two columns) and high nitrogen availability (leaves treated with 200 mm urea; right two columns) conditions. se values (n = 6) are indicated, and statistically significant changes upon infection are marked by asterisks (Welch-Satterthwaite t test; P < 0.05). Amino Acid . Normal Nitrogen Availability . High Nitrogen Availability . Control . Infected . Control . Infected . Amino acid exudation rate (nmol g™1 fresh wt h™1) 26 ± 5 47 ± 7* 36 ± 6 83 ± 17* % total amino acids Asp 9.5 ± 0.5 8.2 ± 0.5 9 ± 0.4 9 ± 2 Glu 20 ± 2 19 ± 2 13 ± 1 16 ± 1 Asn 0.9 ± 0.1 1.2 ± 0.1 0.9 ± 0.1 1.1 ± 0.1 Ser 11 ± 1 11 ± 1 15.6 ± 0.8 14 ± 1 Gln 2.1 ± 0.2 4.4 ± 0.9* 3.5 ± 0.3 4.9 ± 0.8 Gly 14 ± 1 8.9 ± 0.5* 13 ± 1 11.1 ± 0.9 His 0.7 ± 0.1 0.7 ± 0.2 0.9 ± 0.1 0.5 ± 0.1* Thr 2.6 ± 0.4 4.3 ± 0.7 2.8 ± 0.3 2.4 ± 0.4 Arg 5 ± 0.3 3.5 ± 0.5* 5.4 ± 0.2 3.1 ± 0.3* Ala 12 ± 2 24 ± 2* 10 ± 2 25 ± 3* Pro 1.7 ± 0.2 1 ± 0.1* 1.4 ± 0.2 0.9 ± 0.1* Tyr 2.1 ± 0.2 1.4 ± 0.1* 2.6 ± 0.2 1.2 ± 0.2* Val 5 ± 0.6 2.5 ± 0.3* 5.2 ± 0.3 2.2 ± 0.3* Met 0.7 ± 0.2 0.34 ± 0.05 1 ± 0.1 0.27 ± 0.02* Ile 3.5 ± 0.6 1.7 ± 0.3* 3.9 ± 0.3 1.3 ± 0.3* Lys 3.4 ± 0.4 3.9 ± 0.9 4.3 ± 0.2 2.7 ± 0.5* Leu 3.8 ± 0.5 2.1 ± 0.3* 4.4 ± 0.4 2 ± 0.5* Phe 2.1 ± 0.3 1.4 ± 0.2 2.1 ± 0.2 1.1 ± 0.2* Amino Acid . Normal Nitrogen Availability . High Nitrogen Availability . Control . Infected . Control . Infected . Amino acid exudation rate (nmol g™1 fresh wt h™1) 26 ± 5 47 ± 7* 36 ± 6 83 ± 17* % total amino acids Asp 9.5 ± 0.5 8.2 ± 0.5 9 ± 0.4 9 ± 2 Glu 20 ± 2 19 ± 2 13 ± 1 16 ± 1 Asn 0.9 ± 0.1 1.2 ± 0.1 0.9 ± 0.1 1.1 ± 0.1 Ser 11 ± 1 11 ± 1 15.6 ± 0.8 14 ± 1 Gln 2.1 ± 0.2 4.4 ± 0.9* 3.5 ± 0.3 4.9 ± 0.8 Gly 14 ± 1 8.9 ± 0.5* 13 ± 1 11.1 ± 0.9 His 0.7 ± 0.1 0.7 ± 0.2 0.9 ± 0.1 0.5 ± 0.1* Thr 2.6 ± 0.4 4.3 ± 0.7 2.8 ± 0.3 2.4 ± 0.4 Arg 5 ± 0.3 3.5 ± 0.5* 5.4 ± 0.2 3.1 ± 0.3* Ala 12 ± 2 24 ± 2* 10 ± 2 25 ± 3* Pro 1.7 ± 0.2 1 ± 0.1* 1.4 ± 0.2 0.9 ± 0.1* Tyr 2.1 ± 0.2 1.4 ± 0.1* 2.6 ± 0.2 1.2 ± 0.2* Val 5 ± 0.6 2.5 ± 0.3* 5.2 ± 0.3 2.2 ± 0.3* Met 0.7 ± 0.2 0.34 ± 0.05 1 ± 0.1 0.27 ± 0.02* Ile 3.5 ± 0.6 1.7 ± 0.3* 3.9 ± 0.3 1.3 ± 0.3* Lys 3.4 ± 0.4 3.9 ± 0.9 4.3 ± 0.2 2.7 ± 0.5* Leu 3.8 ± 0.5 2.1 ± 0.3* 4.4 ± 0.4 2 ± 0.5* Phe 2.1 ± 0.3 1.4 ± 0.2 2.1 ± 0.2 1.1 ± 0.2* Open in new tab Table II. Phloem exudation rate and amino acid composition of phloem exudate collected from leaf 3 of plants infected with U. maydis (leaf 4 harbored tumors) or from control plants at 9 dpi The experiment was conducted under normal (no urea treatment; left two columns) and high nitrogen availability (leaves treated with 200 mm urea; right two columns) conditions. se values (n = 6) are indicated, and statistically significant changes upon infection are marked by asterisks (Welch-Satterthwaite t test; P < 0.05). Amino Acid . Normal Nitrogen Availability . High Nitrogen Availability . Control . Infected . Control . Infected . Amino acid exudation rate (nmol g™1 fresh wt h™1) 26 ± 5 47 ± 7* 36 ± 6 83 ± 17* % total amino acids Asp 9.5 ± 0.5 8.2 ± 0.5 9 ± 0.4 9 ± 2 Glu 20 ± 2 19 ± 2 13 ± 1 16 ± 1 Asn 0.9 ± 0.1 1.2 ± 0.1 0.9 ± 0.1 1.1 ± 0.1 Ser 11 ± 1 11 ± 1 15.6 ± 0.8 14 ± 1 Gln 2.1 ± 0.2 4.4 ± 0.9* 3.5 ± 0.3 4.9 ± 0.8 Gly 14 ± 1 8.9 ± 0.5* 13 ± 1 11.1 ± 0.9 His 0.7 ± 0.1 0.7 ± 0.2 0.9 ± 0.1 0.5 ± 0.1* Thr 2.6 ± 0.4 4.3 ± 0.7 2.8 ± 0.3 2.4 ± 0.4 Arg 5 ± 0.3 3.5 ± 0.5* 5.4 ± 0.2 3.1 ± 0.3* Ala 12 ± 2 24 ± 2* 10 ± 2 25 ± 3* Pro 1.7 ± 0.2 1 ± 0.1* 1.4 ± 0.2 0.9 ± 0.1* Tyr 2.1 ± 0.2 1.4 ± 0.1* 2.6 ± 0.2 1.2 ± 0.2* Val 5 ± 0.6 2.5 ± 0.3* 5.2 ± 0.3 2.2 ± 0.3* Met 0.7 ± 0.2 0.34 ± 0.05 1 ± 0.1 0.27 ± 0.02* Ile 3.5 ± 0.6 1.7 ± 0.3* 3.9 ± 0.3 1.3 ± 0.3* Lys 3.4 ± 0.4 3.9 ± 0.9 4.3 ± 0.2 2.7 ± 0.5* Leu 3.8 ± 0.5 2.1 ± 0.3* 4.4 ± 0.4 2 ± 0.5* Phe 2.1 ± 0.3 1.4 ± 0.2 2.1 ± 0.2 1.1 ± 0.2* Amino Acid . Normal Nitrogen Availability . High Nitrogen Availability . Control . Infected . Control . Infected . Amino acid exudation rate (nmol g™1 fresh wt h™1) 26 ± 5 47 ± 7* 36 ± 6 83 ± 17* % total amino acids Asp 9.5 ± 0.5 8.2 ± 0.5 9 ± 0.4 9 ± 2 Glu 20 ± 2 19 ± 2 13 ± 1 16 ± 1 Asn 0.9 ± 0.1 1.2 ± 0.1 0.9 ± 0.1 1.1 ± 0.1 Ser 11 ± 1 11 ± 1 15.6 ± 0.8 14 ± 1 Gln 2.1 ± 0.2 4.4 ± 0.9* 3.5 ± 0.3 4.9 ± 0.8 Gly 14 ± 1 8.9 ± 0.5* 13 ± 1 11.1 ± 0.9 His 0.7 ± 0.1 0.7 ± 0.2 0.9 ± 0.1 0.5 ± 0.1* Thr 2.6 ± 0.4 4.3 ± 0.7 2.8 ± 0.3 2.4 ± 0.4 Arg 5 ± 0.3 3.5 ± 0.5* 5.4 ± 0.2 3.1 ± 0.3* Ala 12 ± 2 24 ± 2* 10 ± 2 25 ± 3* Pro 1.7 ± 0.2 1 ± 0.1* 1.4 ± 0.2 0.9 ± 0.1* Tyr 2.1 ± 0.2 1.4 ± 0.1* 2.6 ± 0.2 1.2 ± 0.2* Val 5 ± 0.6 2.5 ± 0.3* 5.2 ± 0.3 2.2 ± 0.3* Met 0.7 ± 0.2 0.34 ± 0.05 1 ± 0.1 0.27 ± 0.02* Ile 3.5 ± 0.6 1.7 ± 0.3* 3.9 ± 0.3 1.3 ± 0.3* Lys 3.4 ± 0.4 3.9 ± 0.9 4.3 ± 0.2 2.7 ± 0.5* Leu 3.8 ± 0.5 2.1 ± 0.3* 4.4 ± 0.4 2 ± 0.5* Phe 2.1 ± 0.3 1.4 ± 0.2 2.1 ± 0.2 1.1 ± 0.2* Open in new tab ). Treatment with urea resulted in a proportional increase of amino acid exudation rate in both infected and control plants. Under both nitrogen regimes, a slight shift was observed in the amino acid composition of the phloem exudates from leaf 3 of infected plants compared with controls. Exudates of systemic leaves of infected plants contained more Ala and less minor amino acids compared with the controls (Table II). Under regular nitrogen availability, leaf exudates from infected plants also contained more Gln and less Gly compared with exudates from control plants. The amino acid composition of phloem exudates differed strongly from those of leaf and tumor extracts (for comparison, see Supplemental Fig. S1). This indicates that amino acids are specifically loaded into the phloem and that the free amino acid pool in the phloem does not reflect the amino acid composition in source or sink organs. Phloem-Mobile Minerals Accumulate in Tumors To further investigate whether phloem transport from source leaves to U. maydis-induced tumors is increased compared with noninfected tissue, we assessed the mineral composition of tumors. It is known that the accumulation of mainly phloem-mobile minerals (e.g. potassium, phosphorus, and magnesium) is a consequence of increased phloem flow, since these minerals are basically not transported in the xylem sap (Marschner, 1997). Compared with control leaves, the potassium and phosphorus contents in tumors at 8 dpi were 1.8- and 3.1-fold increased, respectively, while the magnesium content was slightly decreased (Table III Table III. Contents of mainly xylem-mobile (iron and calcium) and mainly phloem-mobile (magnesium, phosphorus, and potassium) minerals in tumors and control leaves at 8 dpi se values are indicated (n = 4), and statistically significant changes in contents are marked by asterisks (Welch-Satterthwaite t test; * P < 0.05, ** P < 0.005). Sample . Iron . Calcium . Magnesium . Phosphorus . Potassium . mg g™1 dry wt Control 0.060 ± 0.004 18.1 ± 0.8 1.8 ± 0.1 3.8 ± 0.2 31 ± 1 Tumor 0.037 ± 0.004* 2.7 ± 0.2** 1.4 ± 0.1* 11.8 ± 0.5** 54 ± 3** Sample . Iron . Calcium . Magnesium . Phosphorus . Potassium . mg g™1 dry wt Control 0.060 ± 0.004 18.1 ± 0.8 1.8 ± 0.1 3.8 ± 0.2 31 ± 1 Tumor 0.037 ± 0.004* 2.7 ± 0.2** 1.4 ± 0.1* 11.8 ± 0.5** 54 ± 3** Open in new tab Table III. Contents of mainly xylem-mobile (iron and calcium) and mainly phloem-mobile (magnesium, phosphorus, and potassium) minerals in tumors and control leaves at 8 dpi se values are indicated (n = 4), and statistically significant changes in contents are marked by asterisks (Welch-Satterthwaite t test; * P < 0.05, ** P < 0.005). Sample . Iron . Calcium . Magnesium . Phosphorus . Potassium . mg g™1 dry wt Control 0.060 ± 0.004 18.1 ± 0.8 1.8 ± 0.1 3.8 ± 0.2 31 ± 1 Tumor 0.037 ± 0.004* 2.7 ± 0.2** 1.4 ± 0.1* 11.8 ± 0.5** 54 ± 3** Sample . Iron . Calcium . Magnesium . Phosphorus . Potassium . mg g™1 dry wt Control 0.060 ± 0.004 18.1 ± 0.8 1.8 ± 0.1 3.8 ± 0.2 31 ± 1 Tumor 0.037 ± 0.004* 2.7 ± 0.2** 1.4 ± 0.1* 11.8 ± 0.5** 54 ± 3** Open in new tab ). In contrast, contents of the predominantly xylem-mobile minerals iron and calcium were decreased in tumors by 40% and 75%, respectively. These data suggest an increased phloem flow and a decreased xylem flow into tumors. Photosynthetic Capacity Is Higher in Systemic Leaves of Infected Plants The increased export of nitrogen assimilates from lower systemic leaves of infected plants should be fueled by an increased CO2 assimilation rate, since photosynthesis provides the carbon backbones for amino acid biosynthesis. Thus, we determined the photosynthetic CO2 assimilation rate (A) and the electron transport rate (ETR) from leaf 3 at different time points after infection with U. maydis at ambient (400 μE m™2 s™1) and saturating (2,200 μE m™2 s™1) light intensity. Most obvious at saturating light intensity, the photosynthetic capacity of leaf 3 was significantly higher in U. maydis-infected plants compared with mock controls (Fig. 6 Figure 6. Open in new tabDownload slide Photosynthetic performance and delay of senescence in lower systemic source leaves of plants infected with U. maydis. A and B, Photosynthetic parameters from leaf 3 were determined in ambient (400 μE m™2 s™1; A) and saturating (2,200 μE m™2 s™1; B) light intensities at different time points after infection, when leaves 4 and 5 of infected plants harbored tumors. Circles, CO2 assimilation rate; triangles, ETR; black symbols, control plants; white symbols, infected plants. Error bars represent se (n = 6). C, Leaf 3 of control plants (left) and from plants infected with U. maydis (right) at 13 dpi. Figure 6. Open in new tabDownload slide Photosynthetic performance and delay of senescence in lower systemic source leaves of plants infected with U. maydis. A and B, Photosynthetic parameters from leaf 3 were determined in ambient (400 μE m™2 s™1; A) and saturating (2,200 μE m™2 s™1; B) light intensities at different time points after infection, when leaves 4 and 5 of infected plants harbored tumors. Circles, CO2 assimilation rate; triangles, ETR; black symbols, control plants; white symbols, infected plants. Error bars represent se (n = 6). C, Leaf 3 of control plants (left) and from plants infected with U. maydis (right) at 13 dpi. ). Both assimilation rate and ETR of leaf 3 from control plants decreased with leaf age starting between 5 and 7 dpi (i.e. between 15 and 17 d post sowing), while the reduction in photosynthetic capacity of leaf 3 was delayed by approximately 3 d in infected plants (Fig. 6, A and B). In plants that had developed mature tumors on leaf 4, both assimilation rate and ETR of leaf 3 from infected plants were increased by 20% to 25% (7 dpi), 30% (8 dpi), and approximately 60% (11 dpi) compared with the respective control leaves. The transcript levels of the senescence markers See1 and See2b (Smart et al., 1995) increased with leaf aging in leaf 3 of noninfected plants between 8 and 14 dpi, while, in comparison, the induction of these two genes was markedly reduced in leaf 3 of infected plants at 11 and 14 dpi (Supplemental Fig. S5). Furthermore, visual inspection showed that senescence-associated chlorophyll loss of the leaves was strongly delayed in infected plants (Fig. 6C), suggesting that increased export rates and maintenance of photosynthetic performance are achieved by a delay in the onset of senescence of lower source leaves of infected plants. Developing tumors have a reduced photosynthetic capacity compared with uninfected leaves of the same position (Horst et al., 2008), and infected plants are stunted (see above). Thus, the signal for the delay in senescence could be caused either by a concomitant increase in total sink strength due to tumor development or by the reduction of green, photosynthetically active biomass of infected plants, both leading to a general change in the source-to-sink balance of the entire plant. Therefore, assimilation rate and ETR of leaf 3 were determined from plants, of which all younger leaves above leaf 3 were shielded from light with aluminum foil, mimicking a drop in the source-to-sink ratio. While assimilation rate (A) and ETR in control plants dropped to 12.5 ± 1.4 and 39 ± 3 μmol m™2 s™1 at 14 dpi, respectively, photosynthetic performance remained high in infected plants (A = 19.6 ± 1.2 μmol m™2 s™1 and ETR = 59 ± 6 μmol m™2 s™1) and covered plants (A = 21 ± 0.6 μmol m™2 s™1 and ETR = 74 ± 6 μmol m™2 s™1). Covering young leaves not only reduced the source strength of the whole plant but also created a strong sink, since the covered leaves still grew, suggesting that these leaves also rely on the import of assimilates from older source leaves. Photosynthetic performance of lower source leaves remained higher than in plants with all upper leaves covered, suggesting that both the reduction in total source capacity and the occurrence of an additional strong sink organ together effectuate the retention of photosynthetic capacity in lower source leaves of maize plants carrying tumors. DISCUSSION Biotrophic plant pathogens represent strong local sinks for nutrients. While extensive work has been done on nutrient acquisition and metabolism of the individual pathogens, only a few studies have addressed the question how overall host nitrogen metabolism is affected upon infection with biotrophic fungi. In this report, we provide a systematic study of (1) the dynamics in nitrogen metabolism during the biotrophic interaction between maize and the corn smut fungus U. maydis in infected leaves and (2) nitrogen allocation in the host plant. Our results have revealed three fundamental insights into the biology of this interaction. First, U. maydis-induced tumors represent a strong sink for organic nitrogen that, second, is provided by systemic source leaves in which, third, photosynthetic capacity and amino acid export are increased, which is accompanied by a suppression of senescence. Furthermore, we show that the amino acids transported in the phloem are metabolized to amino acids with a high nitrogen-carbon ratio after the uptake into tumors. Tumor Development on Maize Leaves Establishes Nitrogen Sink Metabolism Our study has demonstrated that tumors have elevated contents of nitrogen-rich amino acids, such as Gln, Asn, and Arg, when compared with mock-infected leaves. A transient accumulation of nitrogen-rich amino acids has also been observed during the first 24 to 48 h of potato (Solanum tuberosum), maize, and barley (Hordeum vulgare) infection with Phytophthora infestans, Colletotrichum graminicola, and Blumeria graminis f. sp. hordei, respectively (Grenville-Briggs et al., 2005; R.J. Horst, G. Doehlemann, R. Wahl, J. Hofmann, A. Schmiedl, R. Kahmann, J. Kaݶmper, U. Sonnewald, and L.M. Voll, unpublished data). During early biotrophy, these changes in the free amino acid pool may indicate increased nitrogen assimilation that is either (1) required to launch defense responses or (2) reflects the demand for organic nitrogen by the parasite. Accumulation of nitrogen-rich amino acids has also been observed during late necrotrophic growth of Pseudomonas syringae in tomato (Olea et al., 2004) and C. lindemuthianum in bean (Phaseolus vulgaris) leaves (Tavernier et al., 2007). In these two studies, a reduction in primary nitrogen assimilation was accompanied by an increase in cytosolic GS1 and Glu dehydrogenase (GDH) transcript abundance. These two genes are typical senescence markers and are thought to be involved in the recycling of nitrogen that is released during protein degradation (Kamachi et al., 1991; Masclaux et al., 2000). Therefore, GS1 and GDH may facilitate the export of nitrogen from infected leaves in these two interactions, thereby decreasing nitrogen availability to the pathogens (Tavernier et al., 2007). In U. maydis-induced tumors, none of the cytosolic GS isoforms was differentially regulated, and only one GDH (Zm.17860) was slightly up-regulated (see corresponding microarray data, deposited by Doehlemann et al. [2008a], as mentioned in “Materials and Methods”). In addition, other reliable senescence markers like See1 (Cys protease) and See2 (legumain-like protease; Smart et al., 1995) were not transcriptionally up-regulated in tumors. These comparisons with other pathosystems suggest that senescence is not induced in tumors and that the nitrogen metabolism of tumor tissue differs strongly from the nitrogen metabolism observed in other plant-pathogen interactions. In addition to the accumulation of nitrogen-rich amino acids, we found an induction of Asp and Asn metabolism at the transcript level, while we could determine that primary nitrogen assimilation was reduced in tumors at the transcriptional and enzymatic as well as the physiological level. Asn usually accumulates under C limitation (Lam et al., 1996). Since carbon may become limiting to the host due to increased respiration of the infected tissue (see transcript data) and/or due to carbon uptake by the pathogen (Snoeijers et al., 2000), our results could be explained by carbon limitation in tumors. However, we have previously shown that carbon accumulates in the form of soluble carbohydrates in U. maydis-infected leaves (Doehlemann et al., 2008a; Horst et al., 2008). To consider carbon limitation as the trigger for the accumulation of Asn thus seems unlikely. Instead, we favor that the high sink strength of tumors for nitrogen could be the cause of the observed effects on the amino acid pool. It is difficult to estimate the contribution of the pathogen to tumor nitrogen metabolism, especially as only less than 3% of the total tumor volume is of fungal origin. Compared with sporidia harvested immediately after maize infection, fungal genes involved in nitrogen utilization were not induced in fully developed tumors, despite three genes involved in Trp biosynthesis (R.J. Horst, G. Doehlemann, R. Wahl, J. Hofmann, A. Schmiedl, R. Kahmann, J. Kaݶmper, U. Sonnewald, and L.M. Voll, unpublished data). However, this result may indicate that nitrogen supply to U. maydis is similar in planta and on synthetic media. Consequently, it remains elusive to what extent the hypertrophic growth of tumor cells and pathogen metabolism contribute to the massive increase in sink strength of U. maydis-triggered tumors. Nevertheless, our data provide some indication that the increased import of nitrogen into tumors might predominantly fuel protein biosynthesis of U. maydis. Plant cytosolic ribosomes produce large amounts of pathogenesis-related proteins during pathogen attack (Stintzi et al., 1993), and many of these defense genes were also strongly induced in fully developed tumors at 8 dpi (Doehlemann et al., 2008a). Although cytosolic protein biosynthesis of the host was strongly up-regulated in tumors at the transcriptional level, the photosynthetic machinery (Doehlemann et al., 2008a) and, thus, genes involved in plastidic protein biosynthesis were strongly down-regulated in tumors compared with controls. Irrespective of the transcriptional induction of cytosolic protein synthesis, we can assume that total host protein biosynthesis is diminished in tumors compared with healthy leaves, because the photosynthetic apparatus represents the vast majority of cellular protein in mature maize leaves, with Rubisco being up to 50% of the total leaf protein (Leegood et al., 2000). However, we have determined an increased incorporation of [35S]Met into the protein fraction of tumors. Although we cannot directly discriminate between host and pathogen, taken together, these data suggest that most organic nitrogen acquired by the tumors is directed toward fungal protein biosynthesis. Organic Nitrogen Is Rerouted to Tumors from Systemic Source Leaves Although we could demonstrate that primary nitrogen assimilation is reduced in tumors, we have also observed that nitrogen derived from soil nitrate preferentially accumulated in tumors compared with corresponding leaves of noninfected plants. Although apparently contradictory, this result can be explained, as tumors represent a large biomass fraction of the entire shoot. Second, organic nitrogen import from systemic source leaves into tumors was strongly increased compared with corresponding leaves of healthy plants, suggesting that after nitrate feeding, organic nitrogen import from systemic leaves into tumors is favored over a direct import of supplied nitrate from the soil (Fig. 7 Figure 7. Open in new tabDownload slide Model comparing the nitrogen flow in healthy and U. maydis-infected plants. The flow of inorganic nitrogen (black arrows) and amino acids (AA; gray arrows) is depicted for healthy plants (left) and U. maydis-infected plants bearing tumors (right). The thickness of the arrows indicates the flow rate. Plant development and leaf numbering correspond to the material sampled in our experiments. In addition, the inhibition of lower source leaf senescence by increased sink demand is highlighted in the right sketch. Figure 7. Open in new tabDownload slide Model comparing the nitrogen flow in healthy and U. maydis-infected plants. The flow of inorganic nitrogen (black arrows) and amino acids (AA; gray arrows) is depicted for healthy plants (left) and U. maydis-infected plants bearing tumors (right). The thickness of the arrows indicates the flow rate. Plant development and leaf numbering correspond to the material sampled in our experiments. In addition, the inhibition of lower source leaf senescence by increased sink demand is highlighted in the right sketch. ). The reallocation of nitrogen from systemic leaves into tumors defines the tumor as a sink organ for nitrogen, as was already shown for carbon (Billett and Burnett, 1978; Doehlemann et al., 2008a; Horst et al., 2008). As the increased import of organic nitrogen into tumors leads to an accumulation of nitrogen-rich amino acids, it appears extremely unlikely that U. maydis suffers from nitrogen limitation in planta, especially as hyphae can grow alongside the vascular bundles in mature tumors (Doehlemann et al., 2008b). In addition, nitrate does not seem to represent a favored nitrogen source of U. maydis in planta, as nitrate reductase mutants in the SG200 background are fully pathogenic (R.J. Horst and L.M. Voll, unpublished data). The amino acid Gln has been shown to play a major role in nitrogen mobilization to the kernels during the grain-filling period of maize cv B73 (Martin et al., 2006). Although organic nitrogen derived from systemic leaves predominantly accumulates as Asn and Gln in tumors, these amino acids constitute only a minor fraction in the phloem sap of the systemic leaves. This, together with the transcriptional induction of Asn biosynthetic genes, suggests that these amino acids are specifically synthesized in tumors and not directly transported via the phloem. Our findings are in sharp contrast to previous observations in host leaves during necrotrophic growth of P. syringae (Olea et al., 2004) and C. lindemuthianum (Tavernier et al., 2007), where organic nitrogen is mobilized and exported from the infection site to noninfected plant organs via Asn synthetase, cytosolic GS, and GDH. In addition, it was recently observed that, upon infection of spotted knapweed (Centaurea maculosa) with the root herbivore Agapeta zoegana, total nitrogen uptake was reduced and nitrogen was translocated from the root to the shoot of the plant (Newingham et al., 2007). These examples suggest that plants have evolved a way of limiting nutrient supply at the infection site. U. maydis seems to overcome nutrient limitation in infected leaves by inducing tumor formation, thereby generating a strong artificial sink that outcompetes other systemic sink tissues (Fig. 7). Photosynthesis and Organic Nitrogen Export Are Stimulated in Systemic Source Leaves upon Tumor Formation We have demonstrated that import of organic nitrogen into tumors from systemic leaves is strongly increased and that amino acid exudation from systemic source leaves is specifically elevated in infected plants compared with noninfected plants (for summary, see Fig. 7). This suggests an increased phloem flow from systemic leaves to infected leaves, as phloem-mobile minerals accumulated in tumors as well. Thus, the induction of tumor formation seems to be a very effective way of rerouting all phloem-mobile nutrients to the infection site. On the other hand, lower contents of xylem-mobile minerals were detected in tumors, which can be explained by the diminished stomatal conductance for water vapor of tumors compared with healthy leaves, which could account for a decreased mineral transport capacity toward tumors (Horst et al., 2008). Furthermore, we have observed that photosynthesis is elevated in lower systemic source leaves of infected plants and that these leaves exhibit a delay in senescence (Fig. 7). Due to the fact that shielding all younger, growing source leaves from light resulted in similar effects on lower source leaves as tumor formation, our results suggest that a strong shift in the sink-source balance of the entire plant, decreasing source and increasing sink capacity at the same time, triggers the delayed senescence of older source leaves of infected plants (Fig. 7). A delay in senescence of lower source leaves has also been observed upon infection of Ricinus communis by the plant parasite Cuscuta reflexa (Jeschke and Hilpert, 1997), which taps directly into the phloem of the host, where it acquires carbohydrates and amino acids. It is long known that the sink-source balance can influence the onset of senescence (Nooden and Guiamet, 1989), and it has previously been hypothesized that the drop of photosynthesis below a critical threshold can induce senescence (Smart, 1994; Bleecker and Patterson, 1997). In U. maydis-infected maize plants, increased demand for nitrogen and carbon by the tumors provokes a stimulation of carbon and nitrogen export in systemic source leaves, which consequently necessitates increased carbon and nitrogen assimilation. As a result, photosynthetic performance in systemic leaves of infected plants will remain above the critical threshold for a longer time than that of corresponding leaves from uninfected plants, thereby delaying senescence induction. Conflicting results on the significance of altered hexose contents for the induction of senescence have been obtained (Dai et al., 1999; Lara et al., 2004; Kocal et al., 2008). In the U. maydis-maize interaction, however, hexose contents in lower systemic source leaves did not change until the onset of leaf senescence in control plants (data not shown), indicating that hexose contents do not modulate the onset of senescence in the system studied here. In the past, transgenic approaches to increase plant productivity by manipulation of source and sink strength have resulted in the finding that biomass production and yield of many crop plants are not source limited but restricted by the target organ's sink strength for nitrogen and carbon (Herbers and Sonnewald, 1998; Okita et al., 2001). Increasing sink strength for nitrogen by seed-specific overexpression of an amino acid permease in pea (Rolletschek et al., 2005) resulted in increased seed storage protein synthesis of up to 25% and in the accumulation of nitrogen-rich amino acids (Asn, Gln, and Arg) in seeds. The uptake of ammonium from the soil and vegetative growth were also stimulated in these transgenics (Rolletschek et al., 2005), indicating the stimulation of systemic nitrogen metabolism by elevated seed sink strength for nitrogen, similar to the influence of tumor formation on nitrogen metabolism in systemic leaves reported here. Our study links the induction of senescence and source leaf productivity to elevated sink demand in infected plants. This renders the U. maydis-maize pathosystem a promising system to address (1) the role of source-sink relations for the induction of senescence and (2) how sink strength influences source metabolism. MATERIALS AND METHODS Plant and Fungal Cultivation and Infection Conditions For combined transcript and metabolite profiling experiments, maize (Zea mays ‘Early Golden Bantam’) was cultivated as described (Doehlemann et al., 2008a). For all other experiments, the same maize cultivar was grown on P-type soil (Fruݶhstorfer Erde) in phytochambers at a 14-h-light (28°C, relative humidity 50%–60%)/10-h-dark (20°C, relative humidity 80%–90%) regime including a 1-h ramping of light and temperature at the beginning and end of the light period. Light was provided at a photon flux density of 350 μmol m™2 s™1. The solopathogenic Ustilago maydis strain SG200 (Kaݶmper et al., 2006) was cultivated on potato dextrose plates or in YEPSlight liquid medium (Tsukuda et al., 1988) at 28°C, and plant infection was conducted as described (Gillissen et al., 1992). A suspension with fungal sporidia or the same volume of water for mock controls was syringe injected into the stems of 8- to 10-d-old maize seedlings, which resulted in local infection of leaf 4 and sometimes also leaf 5. To study nitrogen allocation, only those plants showing similar tumorization were used. Gene Expression Analysis by DNA Microarray Gene expression data from U. maydis-induced tumors was obtained from the same set of material described by Doehlemann et al. (2008a), which is deposited in the Gene Expression Omnibus (http://www.ncbi.nlm.nih.gov/geo/) under the accession number GSE10023. Metabolite Quantification and Analysis Metabolite contents were determined in three independent experiments from subsets of the leaf material pools that were employed for transcriptome analysis (Doehlemann et al., 2008a), such that material of four independent samples for metabolite analysis were pooled to generate one sample pool for transcript analysis per time point. Due to the high reproducibility of the three replicate experiments with four replicate samples each, metabolite contents were computed based on all 12 analyzed samples per time point. Principal component analysis of metabolite data was performed with the MarkerView software (version 1.1.0.7; Applied Biosystems) using the autoscale algorithm for scaling. The contents of carbohydrates and free amino acids (except Trp and Cys) were determined exactly as described (Abbasi et al., 2009), while Cys contents were determined by the same HPLC-based method used for glutathione quantification by Abbasi et al. (2009). The contents of organic acids and phosphorylated intermediates were determined as follows. Maize leaf material was quenched in liquid nitrogen, ground to a fine powder, divided into aliquots, and stored at ™80°C. Powder aliquots of approximately 50 mg were homogenized in 1 mL of 1 m ice-cold perchloric acid using a precooled mortar and pestle. The remainder was reextracted with 1 mL of ice-cold 0.1 m perchloric acid. Cell debris were removed by centrifugation for 2 min at 20,000g at 4°C, and 1.8 mL of the supernatant was neutralized with two portions of 50 μL of 5 m K2CO3. Precipitated potassium chlorate was removed by centrifugation at 20,000g at 4°C, and the supernatants were divided into aliquots and stored at ™80°C. Extract aliquots of 200 μL were filtered through a 10-kD filter (AcroPrep Omega 10 K; Pall Corporation), and within 12 h, 10 μL of the filtrates was analyzed on an ICS3000 HPLC System (Dionex) connected to a QTrap 3200 Triple-Quadrupole mass spectrometer with turboV ion source (Applied Biosystems) operated in multiple reaction monitoring mode. The system was controlled by the software Chromeleon VS 6.8 and DCMS-Link VS1.1 (Dionex) in combination with Analyst 1.4.1 (Applied Biosystems). Metabolites were separated on two IonPac AS11HC columns (2 × 250 mm; Dionex) protected by an AG11HC guard column (2 × 50 mm). The elution gradient was generated with water (eluent A) and 100 mm KOH (eluent B) within a total run time of 80 min at a flow rate of 0.25 mL min™1 and a column temperature of 35°C as follows: 0 min, 4%; 0 to 1 min, 4%; 1 to 6 min, 15%; 6 to 12 min, 19%; 12 to 22 min, 20%; 22 to 24 min, 23%; 24 to 27 min, 35%; 27 to 37 min, 38%; 37 to 39 min, 45%; 39 to 44 min, 100%; 44 to 71 min, 100%; 71 to 76 min, 4%; and 76 to 80 min, 4% eluent B. Scan ranges were from mass-to-charge ratio 87 to 606 (precursor ions) and mass-to-charge ratio 59 to 385 (product ions). The electrospray ionization source parameters were ™4,500 eV at 600°C, N2 gas pressures were 20 p.s.i. (curtaingas), 30 p.s.i. (gas1), and 20 p.s.i. (gas2), and collision gas was set to medium. The dwell time for ions was 75 ms, and scan time per cycle was 3.7 s. Compound-specific parameters are listed in Supplemental Table S1. The contents of metabolites were calculated based on peak areas for precursor/product ion transitions relative to standards. Enzyme Activity Assays The selective and maximal activities of nitrate reductase and GS activity were determined as described (Gibon et al., 2004) using aliquots of the leaf powder pools that were also employed for gene expression and metabolite profiling. Determination of Photosynthetic Parameters Photosynthetic parameters from lower systemic leaves (leaf 3 when tumors developed on leaves 4 and 5) were determined between 4 to 11 dpi using a combined infrared gas exchange-chlorophyll fluorescence imaging system (GFS-3000 and MINI-Imaging-PAM Chlorophyll Fluorometer; Walz) at an actinic illumination of 400 and 2,200 μmol m™2 s™1, 28°C leaf temperature, 350 μL L™1 CO2, and 10,000 μL L™1 water at a background ambient illumination of 350 μmol m™2 s™1 photon flux density. CO2 assimilation rates (A) was calculated according to (von Caemmerer and Farquhar, 1981), and ETR was calculated as described (Horst et al., 2008). Collection of Phloem Exudates At the time points indicated, the lower systemic leaf (leaf 3) was cut with a razor blade while being submerged in 5 mm EDTA, pH 8.0, to prevent clogging of the sieve tubes by callose. Leaves were placed in 1.5 mL of 5 mm EDTA, and the exudates of the first 15 min were discarded. Then, every 30 min, the leaves were transferred to fresh EDTA solution, and the exudates were snap frozen and used for amino acid quantification as described above. Exudation rates were calculated from the linear phase of the exudation. Elemental and Mineral Analysis Determination of carbon and nitrogen (14N and 15N) was performed from finely ground and freeze-dried material with an elemental analyzer (Vario EL; Elementar Analysensysteme). Nitrogen uptake/nitrogen import into a specific tissue from the start of the labeling experiment to the time of harvest (new N) was calculated using the formula: \[\mathrm{new{\,}N}{\,}(\mathrm{g}{\,}\mathrm{g}^{{-}1}{\,}\mathrm{dry}{\,}\mathrm{weight}){=}[(^{15}\mathrm{N}_{\mathrm{tissue}}{-}^{15}\mathrm{N}_{\mathrm{natural}})/(^{15}\mathrm{N}_{\mathrm{label}}{-}^{15}\mathrm{N}_{\mathrm{natural}})]{\times}\mathrm{N}_{\mathrm{tissue}}\] where 15Ntissue is the atom % of 15N relative to total nitrogen in the tissue, 15Nnatural is the natural abundance of 15N (0.3663 atom %), 15Nlabel is the atom % of 15N used to label the plants (see below), and Ntissue is the nitrogen content of the tissue (g g™1 dry weight). Quantification of mineral nutrients was performed after dry ashing (480°C, 8 h) and dissolving the ash in 6 m HCl with 1.5% (w/v) hydroxylammonium chloride, measuring aqueous 1:10 (v/v) dilutions. Measurements were carried out by inductively coupled plasma optical emission spectroscopy (Spectro Analytical Instruments) as described (Fuehrs et al., 2008). 15N Labeling and Determination of 15N Abundance in Amino Acid Pools The incorporation of soil nitrate was determined as follows. Maize plants were watered with 40 mL of 20 mm KNO3 enriched with 20% 15NO3 ™ at 8 dpi. Samples of infected and control leaves as well as from the remaining, symptomless aerial organs were taken at 4, 7, 10, 24, and 48 h after administration of K15NO3. The plant material was ground to a fine powder and used for elemental analysis (see above) and for the determination of 15N abundance in the free and protein-bound amino acid pools. Proteins were extracted, precipitated with methanol-chloroform-water, and hydrolyzed for 16 h in 6 n HCl at 110°C. The released amino acids from the protein fraction were determined as described below. For the determination of the reallocation of reduced nitrogen from systemic leaves, 100 μL of 200 mm urea (with 0.05% Silwet L-77 as surfactant) enriched with 98% [15N]urea was spread evenly onto leaf 3 of maize plants at 8 dpi. After 30 h, samples were taken from the labeled, the infected, and the older and younger systemic leaves and prepared for elemental and amino acid analysis. Amino acids were extracted from leaf material as described above, and 14N and 15N amino acid contents were assayed using the HPLC-mass spectrometry (MS) system described for metabolite quantification. Ten microliters of the extracts was separated on a C18RP-Acclaim OA column (5 μm, 4 × 250 mm; Dionex) protected by an Acclaim OA guard column (5 μm, 4.3 × 10 mm; Dionex). The elution gradient was generated with 50 mm ammonium acetate, pH 3.5 (eluent A), water (eluent C), and acetonitrile (eluent D) within a total time of 75 min at a flow rate of 0.25 mL min™1 and a column temperature of 30°C as follows: 0 to 2 min, 5% A/95% C; 2 to 20 min, 30% A/70% C; 20 to 25 min, 30% A/70% C; 25 to 35 min, 5% A/55% C/40% D; 35 to 45 min, 5% A/5% C/90% D; 45 to 50 min, 5% A/5% C/90% D; 50 to 65 min, 5% A/95% C; and 65 to 75 min, 5% A/95% C. Ionization was performed at +5,500 eV at 500°C. N2 gas pressures were 10 p.s.i. (curtaingas), 40 p.s.i. (gas1), and 45 p.s.i. (gas2). The interface heater was on, and collision gas was set to medium. Compound-specific parameters were determined by tuning with standard solutions of 1 to 10 mm. Dwell time was set to 50 ms, while the scan time was divided into three periods of 0 to 9.1 min, 9.2 to 13 min, and 13.1 to 53 min with 0.9 s, 1.8 s, and 0.6 s per cycle, respectively. Precursor/product ion transitions that allow the calculation of the abundance of 14N and 15N of selected nitrogen atoms in the respective amino acids were derived from multiple reaction monitoring spectra of standard solutions and are listed in Supplemental Table S2. 15N-labeled amino acids were recorded with tuning parameters derived from unlabeled isotopes. To calculate 15N enrichment (%) in a particular amino acid, the peak area of the 15N-containing fragment was divided by the total peak area of 14N and 15N fragment. To account for the natural abundance of 13C and 15N, the obtained values were corrected against the background in unlabeled extracts. Incorporation of [35S]Met into Proteins To determine the incorporation of amino acids into proteins, 7-d-old maize seedlings were watered three times at 2-d intervals with 2 mm [35S]Met. These seedlings were infected as described above. Samples from tumors and control leaves were taken at 8 dpi. Proteins and free amino acids were extracted from finely ground material (100–300 mg) with 500 μL of extraction buffer (50 mm Tris-HCl, pH 7.4, 1 mm EDTA, 0.01% Triton X-100, and Complete Protease Inhibitor Cocktail [Roche]) before proteins were precipitated by the addition of an equal volume of 20% TCA. The pellet was washed twice with 1 mL of 10% TCA, the supernatants were combined, and radioactivity in the pellet and supernatant fractions was determined by liquid scintillation counting. Statistical Analysis of Nonmicroarray Data Statistical analysis of metabolite and physiological data was performed with the VANTED software (Junker et al., 2006) using the integrated Welch-Satterthwaite t test. Supplemental Data The following materials are available in the online version of this article. Supplemental Figure S1. Amino acid composition of sink leaves, source leaves, and tumors. Supplemental Figure S2. Amino acid contents in tumors/control leaves after treatment with 15NO3 ™. Supplemental Figure S3. MapMan representation of transcript levels of genes involved in maize protein biosynthesis at 8 dpi. Supplemental Figure S4. Metabolite analysis of upper systemic, symptomless sink leaves of plants infected with U. maydis. Supplemental Figure S5. Expression levels of senescence markers in leaf 3. Supplemental Table S1. Ion transitions used for the detection and quantification of metabolites by ion exchange chromatography-MS/MS. Supplemental Table S2. Ion transitions used for the detection and quantification of labeled and unlabeled amino acids by liquid chromatography-MS/MS. Supplemental Movie S1. Confocal projections of U. maydis-colonized maize leaf tissue at 8 dpi. Supplemental Materials and Methods S1. 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The author responsible for distribution of materials integral to the findings presented in this article in accordance with the policy described in the Instructions for Authors (www.plantphysiol.org) is: Lars M. Voll (lvoll@biologie.uni-erlangen.de). [W] The online version of this article contains Web-only data. [OA] Open Access articles can be viewed online without a subscription. www.plantphysiol.org/cgi/doi/10.1104/pp.109.147702 © 2010 American Society of Plant Biologists © The Author(s) 2010. Published by Oxford University Press on behalf of American Society of Plant Biologists. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (https://creativecommons.org/licenses/by/4.0/), which permits unrestricted reuse, distribution, and reproduction in any medium, provided the original work is properly cited.
TI - Ustilago maydis Infection Strongly Alters Organic Nitrogen Allocation in Maize and Stimulates Productivity of Systemic Source Leaves    
JF - Plant Physiology
DO - 10.1104/pp.109.147702
DA - 2009-12-29
UR - https://www.deepdyve.com/lp/oxford-university-press/ustilago-maydis-infection-strongly-alters-organic-nitrogen-allocation-KgBeo2yAAw
SP - 293
EP - 308
VL - 152
IS - 1
DP - DeepDyve
ER -