Advertisement

Planta

, Volume 242, Issue 4, pp 1025–1035 | Cite as

The fungal endophyte Epichloë typhina improves photosynthesis efficiency of its host orchard grass (Dactylis glomerata)

  • Piotr Rozpądek
  • K. Wężowicz
  • M. Nosek
  • R. Ważny
  • K. Tokarz
  • M. Lembicz
  • Z. Miszalski
  • K. Turnau
Open Access
Original Article
First Online:

Abstract

Main conclusion

According to the results presented in this paper the fungal endophyte Epichloë typhina significantly improves the growth, PSII photochemistry and C assimilation efficiency of its host Dactylis glomerata.

In this paper, we present a comprehensive study of the impact of the endophytic fungi Epichloë typhina on its plant hosts’ photosynthesis apparatus. Chlorophyll a fluorescence, gas exchange, immuno-blotting and spectrophotometric measurements were employed to assess photosynthetic performance, changes in pigment content and mechanisms associated with light harvesting, carbon assimilation and energy distribution in Dactylis glomerata colonized with Epichloë typhina. According to the results presented in this study, colonization of D. glomerata results in improved photosynthesis efficiency. Additionally, we propose a new mechanism allowing plants to cope with the withdrawal of a significant fraction of its energy resources by the endophytic fungi. The abundance of LHCI, LHCII proteins as well as chlorophyll b was significantly higher in E+ plants. Malate export out of the chloroplast was shown to be increased in colonized plants. To our knowledge, we are the first to report this phenomenon. Epichloë colonization improved PSII photochemistry and C assimilation efficiency. Elevated energy demands of E+ D. glomerata plants are met by increasing the rate of carbon assimilation and PSII photochemistry.

Keywords

Endophyte Dactylis glomerata Epichloë typhina Photosynthesis NPQ 

Introduction

Nearly all plants associate in symbiotic relationships with endophytic fungi. Since the early 90s these interactions have been the subject of intensive research, allowing us to gain a general understanding of the role of fungal symbionts in plant physiology and ecology (Schardl 2001; Rodriguez et al. 2009). Many issues, however, evoke serious controversy. Questions concerning endophyte-imposed benefits on plant growth are still being raised. According to some authors endophytic fungi colonization is beneficial for its plant host (Stein et al. 2008; Oelmüller et al. 2009). On the contrary, others classify this interaction as “mild” biotrophic parasitism (Faeth and Sullivan 2003; Saikkonen et al. 2004). The association of plants with symbiotic fungi has been proven to significantly affect plant growth and development. Out of the numerous aspects of plant physiology affected by symbiotic fungi, growth (biomass production), resistance against pathogens and herbivores, nutrient uptake and plant reproduction figure to have the biggest impact on agriculture and shaping of plant communities (Kannadan and Rudgers 2008; Rudgers and Swafford 2009; Yuan et al. 2009; Hartley and Gange 2009; Johnson et al. 2013). Given the potential for biotechnology, there is great interest in understanding the mechanisms of this interaction (Aly et al. 2010; Johnson et al. 2013).

Dactylis glomerata, a C3 grass species, spread over the northern hemisphere has been shown to form a symbiotic association with the fungal endophyte Epichloë typhina, a member of the Clavicipitaceae family. Epichloë fungi are known for their ability to synthesize bioactive compounds, serving as plant protective agents against pathogens and herbivores (Yuan et al. 2009; Czarnoleski et al. 2012). This, however, has been shown to severely affect the health of livestock and the quality of dairy products. Milk from areas where the fungus has spread, due to its toxicity, has been banned from local markets (Bernard et al. 1993; Schmidt and Osborn 1993; Young et al. 2013). This phenomenon is widely known in the USA, New Zealand and Australia but recently it has been gaining significance in Europe. In Central Europe Epichloë endophytes have been reported in several grass species including Festuca, Lolium, Puccinellia, Agropyron, Poa, Elymus and others (Christensen et al. 2002; Górzynska et al. 2011; Lembicz et al. 2013).

E. typhina, similar to other members of Epichloë resides within host shoot tissues, being almost completely confined to the apoplast. During its sexual reproduction it forms characteristic, visible structures—the stromata—causing “choke disease” limiting seed formation, but supporting clonal growth (Schardl 2001). According to previous reports fungi from the Epichloë genus stimulate the growth of its host plant during certain periods of plant ontogenesis (Olejniczak and Lembicz 2007). The fungal partner benefits from the symbiosis withdrawing assimilated photosynthetic carbon and additional elements, particularly nitrogen and sulfur, in sufficient abundance for protein and other essential metabolite synthesis (Christensen et al. 2002).

One way to support elevated energy demands is to improve carbon assimilation efficiency. Photosynthesis requires the orchestrated action of light-driven energy production (ATP and NADPH) and CO2 assimilation in the Calvin–Benson–Bassham cycle. Alterations in the equilibrium between ATP and NADPH production and carbon assimilation due to increased energy demands or stress may substantially alter photosynthetic performance. Chloroplasts have evolved significant energy flexibility mechanisms allowing them to cope with environmental challenges. This plasticity derives from the ability of the photosynthetic apparatus to distribute absorbed energy quantum in a very flexible manner. Out of the many routes of energy management the cyclic electron flow, non-photochemical quenching mechanism (NPQ), malate valve and the water–water cycle seem to be the most important (Kramer and Evans 2011).

Non-photochemical quenching (heat dissipation of excess energy) is performed by at least three distinct mechanisms: energy-dependent quenching (qE), photoinhibitory quenching (qI) and state transition quenching (qT). In non-stressed leaves under moderate to saturating light conditions qE is the major component of NPQ (Baker 2008). It is activated upon light-driven, reversible acidification of the thylakoid lumen and activation of the xanthophyll cycle.

Thylakoid lumen acidification and its redox state is controlled by the malate valve and the malate dehydrogenase (MDH) in particular. It catalyzes the reduction of oxaloacetate to malate and exports the latter out of the chloroplast (the malate valve) enabling de-acidification of the thylakoid lumen (Fridlyand et al. 1998). It has been suggested to play a role in maintaining an appropriate ATP/NADPH ratio, allowing energy production, distribution and carbon assimilation during stress and acclimation. It also de-acidifies the thylakoid lumen by exporting H+ in the form of malate to the cytosol (Scheibe 2004).

The main source of carbon for green plants is photosynthesis, thus we hypothesized that D. glomerata infected with E. typhina must have developed photosynthesis-related mechanisms allowing it to meet elevated energy demands. According to previous reports, CO2 fixation efficiency is decreased in Lolium perenne by E. typhina’s asexual state-Neotyphodium lolii. It does not, however, affect photochemistry (Spiering et al. 2006). Additionally, Amalric et al. (1999) and Marks and Clay (1996) have shown that in high temperature E+ (endophyte) N. lolii positively affects photosynthesis in perennial ryegrass. Improved water use efficiency and other physiological traits observed in E+ plants suggest the possibility that fungal endophytes may indeed positively influence plant photosynthesis (Arachevaleta et al. 1989; Richardson et al. 1993). Previously performed pilot experiments on D. glomerata in its natural environment confirmed this assumption. Photosynthesis efficiency as well as the content of photosynthetically active pigments was increased upon E. typhina colonization. These results led us to examine the phenomenon of endophyte-induced photosynthesis efficiency in a more detailed fashion.

In this study, we attempted to assess the impact of the endophytic E. typhina on the photosynthesis apparatus of orchard grass.

Methods

Plant material

D. glomerata L. plants with and without developed stromata were obtained from the campus of University of Poznań (Poland) in May 2012. Plant rhizomes of uniform size (18 rhizomes from plants with stromata and 18 rhizomes from plants without visible stromata) were collected from the mother grass, planted in plexiglass rhizoboxes (40 × 20 × 4 cm) and grown from May until November 2012 in the substratum from the campus of the Jagiellonian University Kraków, Poland in the University garden (natural, field conditions). During harvest and measurements a c.a. 10 h photoperiod and 150 µmol m−2 s−1 PAR were present. Plants were irrigated on daily basis. No fertilizers or pest control was used during vegetation. At the end of the experiment, a uniform number of leaves from two plants (for one sample) were collected at the beginning of the photoperiod (0700 h) and frozen in liquid nitrogen. Nine samples for each treatment (E+ and control) were collected.

Fungi identification

The fungus was identified using the nucleotide sequences of the β-tubulin gene (tubB). DNA isolation, amplification and sequencing were performed according to the procedure described previously by Brem and Leuchtmann (2003) and Lembicz et al. (2010). A fragment that contained the first three introns of the β-tubulin gene (tubB) was amplified using primers by Craven et al. (2001). Sequences were compared to reference (Lembicz et al. 2011) and deposited in GenBank (National Center for Biotechnology Information, Bethesda, Maryland, USA) under accession number HM007554-HM007560.

Before measurements and harvest (plant material collection) intercellular mycelia were observed using a stereomicroscope, and the presence of the fungus as an endophyte in vegetative tissues of D. glomerata was confirmed. Isolates were obtained from surface-sterilized tissues of stroma that formed tillers grown in axenic cultures.

The presence of the endophyte in D. glomerata tissues was monitored by microscope observation three times during vegetation—at the beginning of the experiment (May), in the middle (August) and at the end of the experiment, before harvest (November). Only plants with confirmed presence/absence of the endophyte in D. glomerata tissues were examined.

Chlorophyll content determination

Chlorophyll content was determined according to the method described by Barnes et al. (1992). Chlorophyll a and b absorbencies were measured at 665 and 648 nm with the CECIL 9500 spectrophotometer and calculated for chlorophyll concentration in fresh weight in nine replicates.

SDS-PAGE and immuno-blotting

Plant leaves were frozen in liquid nitrogen, grounded with a mortar and pestle, and homogenized in ice-cold 100 mM Tricine–Tris buffer pH 8.0, containing 100 mM MgSO4, 1 mM DTT and 3 mM EDTA (Miszalski et al. 1998), flash frozen in liquid nitrogen and sonicated for 20 s. Repeated freezing and sonication was performed in three series (to a point where the supernatant was greener than the pellet) according to the liquid nitrogen + soni–freeze–thaw method described in Western blotting–tips and trouble-shooting (http://www.agrisera.com/cgi-bin/ibutik/AIR_ibutik.pl?funk=Webbsida&ID=152). After extraction, probes were centrifuged for 10 min at 10,000g at 4 °C. Soluble protein content was quantified according to Bradford (1976) using BSA as a standard. For protein denaturation, samples were treated with a 50 mM Tris containing 10 M urea, 2 % β-mercaptoethanol and 4 % SDS and heated at 70 °C for 10 min. Electrophoresis was carried out in a Mini-PROTEAN tetra System (BioRad, USA) in polyacrylamide (PAA) gels containing 4 % SDS according to Laemmli (1970). Protein separation for Rubisco LSU (large subunit) quantification was performed in 4 % stacking (pH 6.8) and 10 % resolving (pH 8.8), 5 µg of total protein was loaded per lane. For the remaining proteins 5.8 % stacking (pH 6.8) and 12 % resolving (pH 8.8) gels were used. 10 µg for D1, Lhca2, Lhca3 and PsaC of total protein was loaded per lane. Electrophoresis was carried out at constant 24 mA for the first 15 min (in the stacking gel), followed by 36 mA until full separation of the protein marker ladder (Thermoscientific, LT). Following electrophoresis, transfer to PVDF membranes (semi-dry) was performed using TransBlot Turbo Transfer System (BioRad, USA). For immunodetection Agrisera (S) primary polyclonal antibodies in the following dilutions were used: Rubisco LSU: 10,000, D1: 1:10,000, PsaC: 1:1,000, Lhca2: 1:2000, Lhcb3: 1:2000. After an overnight incubation period at 4 °C, membranes were treated with secondary antibodies conjugated with alkaline phosphatase (Sigma, USA) for 1.5 h (1:5000 dilution). Specific proteins were visualized by soaking membranes in 20 % BCIP/NBT solution for 1 min. After drying, membranes were scanned with an office scanner. Analysis was performed in triplicates. Densitometric analysis was performed with the Image J software (NIH, USA).

NADPH-malate dehydrogenase activity

The activity of NADPH-malate dehydrogenase (NADPH-MDH, EC 1.1.1.37) was determined in frozen leaf tissue (0.4 g) homogenized on ice in 1.0 ml of 0.1 M Hepes–NaOH pH 8.0, containing 5 mM DTT, 0.5 % (w/v) bovine serum albumin and polyvinylpyrrolidone 40 (0.5 % w/v). The homogenate was centrifuged at 10,000g for 5 min (4 °C). The activity measurement was performed according to Holtum and Winter (1982). Analysis was performed in nine replicates.

Chlorophyll a fluorescence measurements

PSII photochemistry was analyzed with the Dual-PAM (Walz, D) fluorometer. Light curves were recorded in 0–851 µmol s−1 m−2 light range, with ten 1-min illumination steps on light-acclimated leaves. Light curves were collected from seven plants from each treatment at the end of the experiment.

The electron transport rate was calculated according to the following equations:
$${\text{ETR}} = {\text{Y(II)}}\cdot{\text{PAR}}\cdot0. 8 4\cdot0. 5$$
where PAR is the photosynthetic photon flux density (μmol photons m−2 s−1), 0.84 is the theoretical absorption factor of green leaves and 0.5 expresses the equal distribution of excitation energy between PSII and PSI (Maxwell and Johnsons 2000); the complementary quantum yields of energy conversion in PSII were calculated using the Dual-PAM software according to equations by Kramer et al. (2004):
$${\text{Y(II)}} = (F^{\prime}_{\text{m}} - F)/F^{\prime}_{\text{m}}$$
$${\text{Y(NPQ)}} = 1- {\text{Y(II)}} - 1/({\text{NPQ}} + 1+ {\text{qL(}}F_{\text{m}} /F_{0} - 1 ))$$
$${\text{Y(NO)}} = 1/({\text{NPQ}} + 1+ {\text{qL}}\; (F_{\text{m}} /F_{0} - 1 ))$$
$${\text{qL}} = (F^{\prime}_{\text{m}} - {\text{F}})/(F^{\prime}_{\text{m}} - F^{\prime}_{ 0} )\;F^{\prime}_{ 0} /F$$
where F 0′ is not measured, it is approximated according to Oxborough and Baker (1997):
$$F^{\prime}_{ 0} = F_{0} /(F_{\text{v}} /F_{\text{m}} + F_{0} /F^{\prime}_{\text{m}} )$$
NPQ measurements (induction curves) were performed on dark-acclimated leaves at actinic light intensities ranging from 37 to 126 µmol s−1 m−2. Actinic light intensities were selected according to light conditions directly before the measurement. The induction curve was performed according to the manufacturers’ instruction, with modifications. The actinic light phase of the measurement was prolonged to 10 min, with a 20-s relaxation period after application of each saturating pulse. NPQ measurements were performed on nine plants from each treatment at the end of the experiment according to the following equation:
$${\text{NPQ}} = (F_{\text{m}} - F^{\prime}_{\text{m}} )/F^{\prime}_{\text{m}}$$

Gas exchange, photosynthesis efficiency measurements

Gas exchange measurements including stomatal conductance were carried out on D. glomerata leaves with a portable, open gas exchange system (Li-6400, Li-Cor, Lincoln NE) equipped with a 6400-02B LED Light Source in a 6 cm2 cuvette. Measurements were performed in CO2 saturated conditions (650 µmol mol−1); 500 µmol s−1 of air flow, 40–45 % relative humidity, 25 °C leaf temperature and under the 400 µmol (quantum) m−2 s−1 red light intensity.

The A/Ci (assimilation at given intracellular CO2 concentration) response curves were registered in 400 µmol (quantum) m−2 s−1 of light and in the 0–1200 µmol CO2 m−2 s−1 range. The CO2 compensation points were calculated by extrapolation of the logarithmic function equations: y = 5.4916ln (x) − 23.773 (endophyte) and y = 5.3657ln (x) − 25.422 (control) based on the CO2 response curves data obtained from measurements. Gas exchange measurements were performed in five replicates.

Results

Plant biomass

D. glomerata plants grown from rhizomes yielded significantly higher biomass (an over twofold difference) compared to their uninfected counterparts (Fig. 1a), but did not produce seeds.
Fig. 1

Fresh weight of E+ and E− D. glomerata (a). Marks represent mean values from 18 measurements (n = 18 ± SD). Chlorophyll a and b concentration of E+ and E− D. glomerata (b). Marks represent mean values from nine independent measurements (n = 9 ± SD). Stars above symbols indicate statistically significant differences in relation to control at P ≤ 0.05

Fluorescence measurements

The electron transfer rate (ETR) a relative measure of the rate of electron flow through PSII (rate of charge separation at PS II reaction centers) (Fig. 2a) and qL (Fig. 2b) illustrating the fraction of open PSII reaction centers was increased in E+ plants in a similar fashion. A 43 % increase at 121 µmol s−1 m−2 was shown, reaching 69 % at 851 µmol s−1 m−2 for the former and from 18 to 50 % for the latter. From light curve analysis it seems clear that the presence of the endophyte improves the plants ability to convert incident light into chemical energy in a light-dependent manner. At given light conditions the efficiency of PTEC of E+ plants increases proportionally to light intensity. The effective quantum yield of PSII (Y(II)), illustrating the fraction of the absorbed quanta converted into chemically fixed energy was improved in Epichloë-colonized plants in PAR range from 121 to 851 µmol s−1 m−2 (Fig. 2c). In light intensities ranging from 0 to 79 µmol s−1 m−2 no differences were recorded, probably due to limited saturation of the photosynthetic apparatus, insufficient to utilize its full light harvesting potential. The effective quantum yield of E+ compared to E− plants increased by 23–43 % with growing light intensities (Fig. 1c). During light curve recording, the yield of non-photochemical quenching Y(NPQ) and the non-regulated energy dissipation Y(NO) (Fig. 2d, e) was not influenced by the presence of Epichloë endophytes in D. glomerata tissues at most tested light intensities. At low PAR (32–79 µmol s−1 m−2) statistically significant decreases were observed (data not shown). This ambiguity leads us to perform a more precise NPQ determination after dark acclimation (induction curve).
Fig. 2

Photosystem II efficiency measurements of D. glomerata colonized with E. typhina—black squares and control—grey circles. (a) Electron transport rate (ETR), (b) photochemical coefficient qL, (c) the effective quantum yield of PSII Y(II), (d) regulated energy dissipation Y(NPQ) and (e) non-regulated energy dissipation Y(NO). Light curves were registered from light-acclimated plants. Marks represent mean values from seven independent measurements (n = 7 ± SD). Stars above symbols indicate statistically significant differences in relation to control at P ≤ 0.05

At the onset of photosynthesis, i.e., after dark acclimation electrons from PSI cannot be transferred to the Calvin cycle because its enzymatic machinery is inactive and its activation occurs at lower rates than photochemistry (Cardol et al. 2010). This allows to study electron flux through PSII, in a more detailed fashion.

NPQ determinations in dark-acclimated plants showed that endophyte colonization resulted in alterations in NPQ activation kinetics (Fig. 4a). Typically after dark acclimation a rapid induction of NPQ occurs, followed by a gradual decline before reaching steady state. The rapid activation of NPQ in control plants can be attributed to an instantaneous buildup of a proton gradient across the thylakoid membrane and NPQ activation (a typical response). However, in plants colonized by Epichloë endophytes NPQ activation kinetics significantly differed from that found in control. NPQ gradually rose, to reach its steady state after 12 light pulses (approximately 5 min from the onset of actinic light). The activation of electron sinks, the Calvin cycle in particular resulted in a gradual decline. Steady-state NPQ did not vary in the presence of the endophyte, however, NPQ activation differed from control significantly. After eight excitation pulses NPQ in Epichloë-colonized plants reached control values. No rapid NPQ activation and gradual decline was observed. Non-photochemical quenching rose to a certain level to reach steady-state values.

Light intensity plays a pivotal role in NPQ activation, thus to determine whether NPQ activation kinetics in D. glomerata will change at higher light intensities we performed additional experiments at higher actinic light, with stronger saturation pulses. The rationale here was to verify whether lower NPQ at the initial stage of activation is a result of a higher electron flow capacity, allowing electron flow at fairly low actinic light preventing thylakoid lumen acidification and NPQ activation. In 126 µmol s−1 m−2 (the highest tested) of actinic light we observed a similar, but less significant reaction of the photosynthetic apparatus suggesting the presence of other mechanisms sustaining electron flow through PSII (data not shown).

Gas exchange measurements

To verify fluorescence analysis in the context of carbon assimilation we performed gas exchange measurements according to which E. typhinë improves nett photosynthesis at saturated CO2 (650 µmol mol−1) concentrations (Fig. 3c) in D. glomerata. Nett photosynthesis averaged 10.3 µmol CO2 m−2 s−1 in E+ plants and 7.8 µmol CO2 m−2 s−1 in control.
Fig. 3

A/Ci curve (a) and stomatal conductance (b), and nett photosynthesis (c) at optimal CO2 levels of D. glomerata colonized with E. typhina—black squares and control—grey circles. Marks represent mean values from five independent measurements (n = 5 ± SD). Stars above symbols indicate statistically significant differences in relation to control at P ≤ 0.05

To assess the efficiency of carbon assimilation in the biochemical phase of photosynthesis (Calvin cycle) we performed the A/Ci curve and found that the rate of carboxylation in E+ plants was significantly higher in CO2 concentrations up to 500 µmol m−2 s−1. At higher CO2 differences in the rate of carbon assimilation were insignificant (Fig. 3a). The CO2 compensation point as shown in Fig. 3a was significantly lower (close to twofold) in our model, suggesting a more effective rate of CO2 carboxylation in E+ plants.

Stomatal conductance (Fig. 3b) was significantly increased (by 15 %) in E+ D. glomerata, but its transpiration rate, as well as water use efficiency was similar to that found in control (data not shown).

Chlorophyll concentration

The concentration of total chlorophyll was significantly improved in Epicholë-colonized D. glomerata, by approximately 33 %. In E+ 0.0194 mg g FW−1, whereas in control 0.0145 mg g FW−1 was recorded. No statistically significant differences were reported in the concentration of chl a, however, a twofold increase in the concentration of chl b was shown in (Fig. 1b). In E+ 0.0062 mg g FW−1, whereas in control 0.003 mg g FW−1 was recorded. The chl a/b ratio was also changed in infected plants from 4:1 to 2:1.

Immuno-blot analysis of chloroplast proteins

To determine potential changes in photosystem antennae size/abundance, the content of selected PSII and PSI proteins was assessed. A twofold increase in the abundance of the PSII protein D1 and over threefold increase in the abundance of Lhcb3 chl a/b-binding proteins was shown. The content of PSI proteins: PsaC and Lhca2 chl a/b-binding proteins has been shown to be significantly (by over twofold) increased in Epichloë-colonized D. glomerata (Fig. 4c; Table 1).
Fig. 4

NPQ of D. glomerata colonized with E. typhina—black squares and control—grey circles. Induction curves were registered after dark acclimation at 63 µmol s−1 m−2 actinic light intensity (a). NADPH-MDH activity (b) from D. glomerata colonized with E. typhina—black bars and control—grey bars. Marks mean values from nine independent measurements (n = 9 ± SD). Stars above symbols indicate statistically significant differences in relation to control at P ≤ 0.05. Typical immunoblots of SDS-PAGE-separated polypeptides (c) of Rubisco (5 µg of total protein per lane), D1 (10 µg of total protein per lane), PsaC (10 µg of total protein per lane) and Lhca2 (10 µg of total protein per lane) from D. glomerata colonized with E. typhina and control

Table 1

Relative abundance of PSI and PSII proteins in D. glomerata leaves inoculated with E. typhina and control

Protein

Relative abundance

Control

Endophyte

Rubisco LSU

39,237 ± 5585a

48,939 ± 3995b

D1

24,952 ± 23a

48,189 ± 2167b

Psa C

2582 ± 217a

7280 ± 750b

Lhca 2

10,812 ± 347a

23,573 ± 1993b

Lhca 3

7432 ± 805a

26,273 ± 8687b

PSI and PSII proteins from crude extracts were separated in SDS-PAGE and transferred to PVDF membranes. Densitometric analysis of immunoblots was performed with ImageJ (NIH, US). Different letters indicate statistically significant differences at P ≤ 0.05. All analysis were performed in triplicates

NADPH-MDH activity

The activity of the NADPH-MDH enzyme was significantly (sixfold) increased in infected D. glomerata. In E+ plants 6.183 nmol min−1 mg−1 protein of NADPH was decomposed by NADPH-MDH compared to 1.17 nmol min−1 mg−1 protein in control (Fig. 4b).

Discussion

In previous studies, selected strains of E. typhinë delivered benefits in productivity and persistence of Lolium perenne (Popay et al. 1999; Hume et al. 2007, 2009). The improved performance of these endophyte-infected grasses has been attributed to their effects on insect herbivores (Johnson et al. 2013). In this study, a significant yield improvement of D. glomerata colonized with commonly occurring in Central Europe strain of E. typhinë grown in semi-controlled conditions was shown. According to Easton (2007) the effect of Epichloe endophytes on grass species is small and inconsistent under controlled conditions.

Since no coherent data explaining the phenomenon of E. typhina-induced grass growth improvement have been presented yet, we propose that the presence of the beneficial fungi shifts plant metabolism from defense to growth allowing the plant to utilize available resources for photosynthesis and carbon assimilation. This allows the plant to “feed” its fungal partner and yield high biomass. Numerous studies with mycorrhizal plants have shown increased stress resistance and a significant improvement in photosynthesis efficiency upon fungal colonization (Aloui et al. 2011; Ruiz-Lozano et al. 2012).

Here, the efficiency of electron transport through PSII was shown to be improved in E+ D. glomerata plants, suggesting a higher rate of solar energy utilized for photochemistry. Increased electron density flux indicates higher ATP and NADPH production in the PETC (photosynthetic electron transport chain), employed for carbon assimilation in the Calvin cycle. Improved CO2 assimilation measured by gas exchange seems to support this point of view.

Besides photochemical reactions, incident light energy absorbed by the photosynthetic apparatus can be dissipated as heat or cause potential damage by generation of deleterious ROS (reactive oxygen species) when in excess (Moller and Sweetlove 2010). At high PAR intensities the amount of absorbed quanta dissipated as heat, Y(NPQ) and potentially harmful (Y(NO) non-regulated energy dissipation) increase with a parallel decrease in Y(II). In this study, no significant changes in Y(NPQ) and Y(NO) were shown during light curve recording. Y(NO) values were fairly low and steady, independent of irradiance, suggesting that the majority of the incident light energy is either converted into ATP and NADPH or dissipated as heat.

Photosynthesis is limited by biophysical and biochemical barriers such as stomatal conductance and carboxylation capacity. Carbon assimilation is strongly related to CO2 accessibility, which in turn depends on the intercellular carbon dioxide concentration and limitations in its diffusion. Stomatal conductance impacts gas diffusion rates resulting in a decline of chloroplastic CO2 concentration and subsequently limits photosynthesis (Sharkey et al. 2007; Centritto et al. 2009). Even though stomatal conductance in colonized D. glomerata plants was shown to be significantly higher no differences in transpiration rate were reported. These results are difficult to interpret in the context of gas exchange; however, the decreased CO2 compensation point of E+ plants suggests that the internal concentration of CO2 may had been higher, improving nett photosynthesis. Higher internal CO2 concentrations indicate an increased rate of carbon assimilation by Rubisco. Increased carboxylation may derive from increased Rubisco activity or abundance.

Improved electron flow rate and carbon assimilation should be accompanied by improved light harvesting. Total chlorophyll concentration was significantly increased in E+ plants. Measurements of chl a and chl b revealed that the amount of chl b (over 100 % increase) accounted for the observed difference. Chlorophyll b transfers excitation energy to chlorophylls from reaction centers and is necessary for proper assembly and stabilization in thylakoid membranes and for appropriate functioning of most LHC complexes (Hoober and Eggink 2001). Reduced chl a/b ratio characteristic for plants grown in low-light conditions usually results in increased grana stacking that is often associated with modifications in protein content. Tobacco plants overexpressing the CAO gene (chlorophyllide a oxygenase) responsible for chl b synthesis have been shown to have improved light harvesting capacities, increased electron transport and carbon dioxide fixation independently of light conditions (Biswal et al. 2012). The improved PS(II) efficiency and increased chl b content–characteristic for PSII—led us to speculate that in Epichloë-colonized plants the abundance of PSII should be elevated. To verify this hypothesis, we quantified the abundance of the PSII proteins PsbA and Lhcb3. PsbA along with several other proteins (D2, the α- and β-subunits of cytochrome b559, and the PsbI protein) form the PSII reaction center complex. The D1/D2 heterodimer binds the manganese cluster involved in water oxidation in PSII (Nanba and Satoh 1987, Sun et al. 2007). Lhcb3 is a preferential site of regulation of the antenna function in excess light conditions (Caffarri et al. 2004). A pronounced increase in the abundance of these proteins was shown in colonized plants, indicating a higher density of PSII in E+ plants.

According to our results, an increase of PSI-associated proteins was present in E+ plants. Lhca2 is one of four PSI Lhca proteins. It is associated with PsaA and to PsaJ via gap chlorophylls (Schmid 2008). PsaC is a conserved, Fe–S-binding protein present in all known PSI complexes. It is tightly bound to the PsaA/PsaB heterodimer and coordinates the Fe–S clusters FA and FB through two cysteine-rich domains. PsaC has been shown to be essential for in vivo assembly of PSI in Chlamydomonas reinhardtii (Takahashi et al. 1991, 1992). Taken together, we can conclude that improved photosynthetic performance in endophyte-colonized D. glomerata was due to improved harvesting capacities.

The photosynthesis apparatus of Populus alba and Medicago truncatula inoculated with AMF (arbuscular mycorrhiza fungi) species from the Glomus genus behaved similarly. According to proteomic and gene expression studies, the expression of Rubisco, several chlorophyll-binding proteins and PSII and I structural proteins was increased in AMF+ plants. The efficiency of carbon assimilation and PSII photochemistry was also improved in a manner similar to that found in E+ D. glomerata (Aloui et al. 2011; Cicatelli et al. 2010, 2012; Lingua et al. 2008). Even though AMF and fungal endophytes belong to distinct groups of fungi, both can be beneficial for their host. As shown in this study beneficial symbionts may similarly affect the photosynthesis apparatus of their host resulting in improved growth and/or stress resistance.

Significant changes in NPQ activation kinetics in E+ plants were recorded. Since carbon assimilation cannot serve as a sink for electrons at the onset of actinic light phase of the NPQ measurement, a mechanism changing NPQ activation kinetics, i.e., sustaining electron flow through PSII and/or an additional electron sink must had been activated in E+ plants.

We have shown a threefold increase in the activity of the NADPH-MDH enzyme in Epichloë colonized plants. Some of this malate can be oxidized in the mitochondrion to synthesize ATP. It can also be oxidized back to oxaloacetate in the cytosol, generating NADH (Scheibe 2004). In the mitochondria malate generated by photosynthetic activity can be oxidize, providing ATP to support UDPG formation for sugar synthesis and allows the oxidation of glycine generated during photorespiration (Scheibe 2004). It cannot be ruled out that the malate synthesized by the NADPH-MDH serves as an additional energy resource for the plant due to its elevated energy demand. The endosymbiotic fungi present in the plant apoplast could in this case use malate or a product of its metabolism as a source of energy.

The results of our study shed a new light on mechanisms allowing plants to cope with the withdrawal of a significant fraction of its energy resources by endophytic fungi, allowing it at the same time to sustain improved growth. We also suggest that upon endophyte colonization, its host D. glomerata undergoes changes in its photosynthetic apparatus, leading to increased light harvesting and photosynthesis efficiency. This may be to support its fungal partners’ energy demands. According to the literature, D. glomerata benefits from the fungal antiherbivory substances (Yuan et al. 2009; Czarnoleski et al. 2012). Thus, it cannot be ruled out that this additional protection allows it to focus its own resources on carbon assimilation. The assimilated carbon may be transported, as proposed here via malate, from the chloroplast to the apoplast, where the fungi reside. This, however, needs further confirmation. Further investigations will allow us to gain a better understanding of communication and resource exchange between symbiotic plants and fungi.

Author contribution

Rozpądek P—MS preparation, chlorophyll a fluorescence, idea; Wężowicz K—western blotting; Ważny R—western blotting, plant cultivation; Nosek M—chlorophyll concentration, NADPH-ME activity; Tokarz K—gas exchange measurements; Lembicz M—plant and fungi preparation, idea; Miszalski Z—MS preparation; Turnau K—MS preparation, endophyte presence verification.

Notes

Acknowledgments

This work was supported by The National Science Center, Maestro Project, DEC -2011/02/A/NZ9/00137.

Supplementary material

425_2015_2337_MOESM1_ESM.pptx (211 kb)
Supplementary material 1 (PPTX 211 kb)

References

  1. Aloui A, Recorbet G, Gollotte A, Robert F, Valot B, Gianinazzi-Pearson V, Aschi-Smiti S, DumasGaudot E (2011) On the mechanisms of cadmium stress alleviation in Medicago truncatula by arbuscular mycorrhizal symbiosis: a root proteomic study. Proteomics 9:420–433CrossRefGoogle Scholar
  2. Aly AH, Debbab A, Kjer J, Proksch P (2010) Fungal endophytes from higher plants: a prolific source of phytochemicals and other bioactive natural products. Fungal Divers 41:1–16CrossRefGoogle Scholar
  3. Amalric C, Sallanon H, Monnet F, Hitmi A, Coudret A (1999) Gas exchange and chlorophyll fluorescence in symbiotic and non-symbiotic ryegrass under water stress. Photosynthetica 37:107–112CrossRefGoogle Scholar
  4. Arachevaleta M, Bacon CW, Hoveland CS, Radcliffe DE (1989) Effect of the tall fescue endophyte on plant response to environmental stress. Agron J 81:83–90CrossRefGoogle Scholar
  5. Baker N (2008) Chlorophyll fluorescence: a probe of photosynthesis in vivo. Annu Rev Plant Biol 59:89–113CrossRefPubMedGoogle Scholar
  6. Barnes JD, Balaguer L, Manrique E, Elvira S, Davison AW (1992) A reappraisal of the use of DMSO for the extraction and determination of chlorophylls a and b in lichens and higher plants. Environ Exp Bot 32:85–100CrossRefGoogle Scholar
  7. Bernard JK, Chestnut AB, Erickson BH, Kelly FM (1993) Effects of prepartum consumption of endophyte-infested Tall fescue on serum prolactin and subsequent milk production of holstein cows. J Dairy Sci 76:1928–1933CrossRefGoogle Scholar
  8. Biswal AK, Pattanayak GK, Pandey SS, Leelavathi S, Reddy VS, Govindjee Tripathy BC (2012) Light intensity-dependent modulation of chlorophyll b biosynthesis and photosynthesis by overexpression of chlorophyllide a oxygenase in tobacco. Plant Physiol 159:433–449PubMedCentralCrossRefPubMedGoogle Scholar
  9. Bradford M (1976) A rapid and sensitive method for quantification of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem 72:248–254CrossRefPubMedGoogle Scholar
  10. Brem D, Leuchtmann A (2003) Molecular evidence for host-adapted races of the fungal endophyte Epichloë bromicola after presumed host shifts. Evolution 57:37–51PubMedGoogle Scholar
  11. Caffarri S, Croce R, Cattivelli L, Bassi R (2004) A look within LHCII: differential analysis of the Lhcb1-3 complexes building the major trimeric antenna complex of higher plant photosynthesis. Biochem US 43:9467–9476CrossRefGoogle Scholar
  12. Cardol P, De Paepe R, Franck F, Forti G, Finazzi G (2010) The onset of NPQ and Deltamu(H) + upon illumination of tobacco plants studied through the influence of mitochondrial electron transport. Biochim Biophys Acta 1797:177–188CrossRefPubMedGoogle Scholar
  13. Centritto M, Lauteri M, Monteverdi MC, Serraj R (2009) Leaf gas exchange, carbon isotope discrimination, and grain yield in contrasting rice genotypes subjected to water deficits during the reproductive stage. J Exp Bot 60:2325–2339CrossRefPubMedGoogle Scholar
  14. Christensen MJ, Bennett RJ, Schmid J (2002) Growth of Epichloë/Neotyphodium and p-endophytes in leaves of Lolium and Festuca grasses. Mycol Res 106:93–106CrossRefGoogle Scholar
  15. Cicatelli A, Lingua G, Todeschini V, Biondi S, Torrigiani P, Castiglione S (2010) Arbuscular mycorrhizal fungi restore normal growth in a white poplar clone grown on heavy metal-contaminated soil, and this is associated with upregulation of foliar metallothionein and polyamine biosynthetic gene expression. Ann Bot 106:791–802PubMedCentralCrossRefPubMedGoogle Scholar
  16. Cicatelli A, Lingua G, Todeschini V, Biondi S, Torrigiani P, Castiglione S (2012) Arbuscular mycorrhizal fungi modulate the leaf transcriptome of a Populus alba L. clone grown on a zinc and copper-contaminated soil. Environ Exp Bot 75:25–35CrossRefGoogle Scholar
  17. Craven KD, Hsiau PTW, Leuchtman A, Hollin W, Schardl CI (2001) Multigne phylogeny of Epichloë species, fungal symbionts of grasses. Ann Mo Bot Gard 88:14–34CrossRefGoogle Scholar
  18. Czarnoleski M, Pawlik K, Olejniczak P, Kozłowski J, Lembicz M (2012) An endophytic fungus reduces herbivory in its recently colonised grass host: a food-choice experiment on common voles, weeping alkali grass and Epichloë typhina. Plant Ecol 213:1049–1053CrossRefGoogle Scholar
  19. Easton HS (2007) Grasses and Neotyphodium endophytes: coadaptation and adaptive breeding. Euphytica 154:295–306CrossRefGoogle Scholar
  20. Faeth SH, Sullivan TJ (2003) Mutualistic, asexual endophytes in a native grass are usually parasitic. Am Nat 161:310–325CrossRefPubMedGoogle Scholar
  21. Fridlyand LE, Backhausen JE, Scheibe R (1998) Flux control of the malate valve in leaf cells. Arch Biochem Biophys 349:290–298CrossRefPubMedGoogle Scholar
  22. Górzyńska K, Lembicz M, Olszanowski Z, Leuchtmann A (2011) Botanophila-Epichloë interaction in a wild grass, Puccinellia distans, lacks dependence on the fly vector. Ann Entomol Soc Am 104:841–846CrossRefGoogle Scholar
  23. Hartley SU, Gange AC (2009) Impacts of plant symbiotic fungi on insect herbivores: mutualism in a multitrophic context. Annu Rev Entomol 54:323–342CrossRefPubMedGoogle Scholar
  24. Holtum JAM, Winter K (1982) Activity of enzymes of carbon metabolism during the induction of crassulacean acid metabolism in Mesembryanthemum crystallinum L. Planta 155:8–16CrossRefPubMedGoogle Scholar
  25. Hoober JK, Eggink LL (2001) A potential role of chlorophylls b and c in assembly of light-harvesting complexes. FEBS Lett 489:1–3CrossRefPubMedGoogle Scholar
  26. Hume DE, Ryan DL, Cooper BM, Popay AJ (2007) Agronomic performance of AR37-infected ryegrass in northern New Zealand. Proc N Z Grassl Assoc 69:201–205Google Scholar
  27. Hume DE, Cooper BM, Panckhurst KA (2009) The role of endophyte in determining the persistence and productivity of ryegrass, tall fescue and meadow fescue in Northland. Proc N Z Grassl Assoc 71:145–150Google Scholar
  28. Johnson LJ, de Bonth ACM, Briggs LR, Caradus JR, Finch SC, Fleetwood DJ, Fletcher LR, Hume DE, Johnson RD, Popay AJ, Tapper BA, Simpson WR, Voisey CR, Card SD (2013) The exploitation of epichloë endophytes for agricultural benefits. Fungal Divers 60:171–188CrossRefGoogle Scholar
  29. Kannadan S, Rudgers JA (2008) Endophyte symbiosis benefits a rare grass under low water availability. Funct Ecol 4:706–713CrossRefGoogle Scholar
  30. Kramer DM, Evans JR (2011) The importance of energy balance in improving photosynthetic productivity. Plant Physiol 155:70–78PubMedCentralCrossRefPubMedGoogle Scholar
  31. Kramer DM, Johnson G, Kiirats O, Edwards GE (2004) New fluorescence parameters for the determination of QA redox state and excitation energy fluxes. Photosynth Res 79:209–218CrossRefPubMedGoogle Scholar
  32. Laemmli UK (1970) Cleavage of structural proteins during the assembly of the head bacteriophage T4. Nature 227:680–685CrossRefPubMedGoogle Scholar
  33. Lembicz M, Górzyńska K, Leuchtmann A (2010) Choke disease, caused by Epichloë bromicola, in the grass Agropyron repens in Poland. Plant Dis 94:1372CrossRefGoogle Scholar
  34. Lembicz M, Górzyńska K, Olejniczak P, Leuchtmann A (2011) Geographical distribution and effects of choke disease caused by Epichloë typhina in populations of the grass Puccinellia distans in Poland. Sydowia 63:37–48Google Scholar
  35. Lembicz M, Górzyńska K, Olszanowski Z, Michelsen V, Leuchtmann A (2013) The occurrence and preference of Botanophila flies (Diptera: Anthomyiidae) for particular species of Epichloë fungi infecting wild grasses. Eur J Entomol 110:129–134CrossRefGoogle Scholar
  36. Lingua G, Franchin C, Todeschini V, Castiglione S, Biondi S, Burlando B, Parravicini V, Torrigiani P, Berta G (2008) Arbuscular mycorrhizal fungi differentially affect the response to high zinc concentrations of two registered poplar clones. Environ Pollut 153:137–147CrossRefPubMedGoogle Scholar
  37. Marks S, Clay K (1996) Physiological responses of Festuca arundinacea to fungal endophyte infection. New Phytol 133:727–733CrossRefGoogle Scholar
  38. Maxwell K, Johnsons GN (2000) Chlorophyll fluorescence—a practical guide. J Exp Bot 51:659–668CrossRefPubMedGoogle Scholar
  39. Miszalski Z, Ślesak I, Niewiadomska E, Bączek-Kwinta R, Lüttge U, Ratajczak R (1998) Subcellular localization and stress responses of superoxide dismutase isoforms from leaves in the C3-CAM intermediate halophyte Mesembryanthemum crystallinum L. Plant, Cell Environ 21:169–179CrossRefGoogle Scholar
  40. Moller IM, Sweetlove LJ (2010) ROS signalling—specificity is required. Trend Plant Sci 15:370–374CrossRefGoogle Scholar
  41. Nanba O, Satoh K (1987) Isolation of a photosystem II reaction center consisting of D-1 and D-2 polypeptides and cytochrome b-559. Proc Natl Acad Sci USA 84:109–112PubMedCentralCrossRefPubMedGoogle Scholar
  42. Oelmüller R, Sherameti I, Tripathi S, Varma A (2009) Piriformospora indica, a cultivable root endophyte with multiple biotechnological applications. Symbiosis 49:1–17CrossRefGoogle Scholar
  43. Olejniczak P, Lembicz M (2007) Age-specific response of the grass Puccinellia distans to the presence of a fungal endophyte. Oecologia 152:485–494CrossRefPubMedGoogle Scholar
  44. Oxborough K, Baker NR (1997) Resolving chlorophyll a fluorescence images of photosynthetic efficiency into photochemical and non-photochemical components—calculation of qP and Fv’/Fm’ without measuring Fo’. Photosynth Res 54:135–142CrossRefGoogle Scholar
  45. Popay AJ, Hume DE, Baltus JG, Latch GCM, Tapper BA, Lyons TB, Cooper BM, Pennell CG, Eerens JPJ, Marshall SL (1999) Field performance of perennial ryegrass (Lolium perenne) infected with toxin-free fungal endophytes (Neotyphodium spp.). In: Woodfield DR, Matthew C (eds) Ryegrass endophyte: an essential New Zealand symbiosis, grassland research and practice, vol 7, pp 113–122Google Scholar
  46. Richardson MD, Hoveland CS, Bacon CW (1993) Photosynthesis and stomatal conductance of symbiotic and non symbiotic tall fescue. Crop Sci 33:145–149CrossRefGoogle Scholar
  47. Rodriguez RJ, White JF Jr, Arnold AE, Redman RS (2009) Fungal endophytes: diversity and functional roles. New Phytol 182:314–330CrossRefPubMedGoogle Scholar
  48. Rudgers S, Swafford AL (2009) Benefits of a fungal endophyte in Elymus virginicus decline under drought stress. Basic Appl Ecol 10:43–51CrossRefGoogle Scholar
  49. Ruiz-Lozano JM, Porcel R, Azcón C, Aroca R (2012) Regulation by arbuscular mycorrhizae of the integrated physiological response to salinity in plants: new challenges in physiological and molecular studies. J Exp Bot 63:4033–4044CrossRefPubMedGoogle Scholar
  50. Saikkonen K, Wäli P, Helander M, Faeth SH (2004) Evolution of endophyte-plant symbioses. Trends Plant Sci 9:275–280CrossRefPubMedGoogle Scholar
  51. Schardl CL (2001) Epichloe festucae and related mutualistic symbionts of grasses. Fungal Genet Biol 33:69–82CrossRefPubMedGoogle Scholar
  52. Scheibe R (2004) Malate valves to balance cellular energy supply. Physiol Plant 120:21–26CrossRefPubMedGoogle Scholar
  53. Schmid VH (2008) Light-harvesting complexes of vascular plants. Cell Mol Life Sci 65:3619–3639CrossRefPubMedGoogle Scholar
  54. Schmidt SP, Osborn TG (1993) Effects of endophyte-infected tall fescue on animal performance. Agr Ecosys Environ 44:233–262CrossRefGoogle Scholar
  55. Sharkey TD, Bernacchi CJ, Farquhar GD, Singsaas EL (2007) Fitting photosynthetic carbon dioxide response curves for C3 leaves. Plant, Cell Environ 30:1035–1040CrossRefGoogle Scholar
  56. Spiering M, Greer DH, Schmid J (2006) Effects of the fungal endophyte, Neotyphodium lolii, on net photosynthesis and growth rates of perennial ryegrass (Lolium perenne) are independent of in planta endophyte concentration. Ann Bot Lond 98:379–387CrossRefGoogle Scholar
  57. Stein E, Molitor A, Kogel KH, Waller F (2008) Systemic resistance in Arabidopsis conferred by the mycorrhizal fungus Piriformospora indica requires jasmonic acid signaling and the cytoplasmic function of NPR1. Plant Cell Physiol 49:1747–1751CrossRefPubMedGoogle Scholar
  58. Sun X, Peng L, Guo J, Chi W, Ma J, Congming LuC, Zhang L (2007) Formation of DEG5 and DEG8 complexes and their involvement in the degradation of photodamaged photosystem II reaction center D1 protein in Arabidopsis. Plant Cell 19:1347–1361PubMedCentralCrossRefPubMedGoogle Scholar
  59. Takahashi Y, Goldschmidt-Clermont M, Soen SY, Franzén LG, Rochaix JD (1991) Directed chloroplast transformation in Chlamydomonas reinhardtii: insertional inactivation of the psaC gene encoding the iron sulfur protein destabilizes photosystem I. EMBO J 10:2033–2040PubMedCentralPubMedGoogle Scholar
  60. Takahashi T, Kubota M, Watanabe M, Yoshihara K, Derguini F, Nakanishi K (1992) Diversion of the sign of phototaxis in a Chlamydomonas reinhardtii mutant incorporated with retinal and its analogs. FEBS Lett 275–279Google Scholar
  61. Young CA, Hume DE, McCulley RL (2013) Fungal endophytes of tall fescue and perennial ryegrass: pasture friend or foe? J Anim Sci 91:2379–2394CrossRefPubMedGoogle Scholar
  62. Yuan ZL, Zhang CL, Lin FC (2009) Role of diverse non-systemic fungal endophytes in plant performance and response to stress: progress and approaches. J Plant Growth Regul 29:116–126CrossRefGoogle Scholar

Copyright information

© The Author(s) 2015

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors and Affiliations

  • Piotr Rozpądek
    • 1
    • 2
  • K. Wężowicz
    • 1
  • M. Nosek
    • 3
  • R. Ważny
    • 4
  • K. Tokarz
    • 2
    • 5
  • M. Lembicz
    • 6
  • Z. Miszalski
    • 4
  • K. Turnau
    • 1
    • 4
  1. 1.Institute of Environmental SciencesJagiellonian UniversityKrakówPoland
  2. 2.Institute of Plant PhysiologyPolish Academy of SciencesKrakówPoland
  3. 3.Institute of BiologyPedagogical UniversityKrakówPoland
  4. 4.Malopolska Centre of BiotechnologyJagiellonian UniversityKrakówPoland
  5. 5.Institute of Plant Biology and BiotechnologyUniversity of AgricultureKrakowPoland
  6. 6.Department of Plant TaxonomyA. Mickiewicz UniversityPoznańPoland

Personalised recommendations