Fusarium graminearumforms mycotoxin producing infection structures on wheat
© Boenisch and Schäfer; licensee BioMed Central Ltd. 2011
Received: 9 August 2010
Accepted: 28 July 2011
Published: 28 July 2011
The mycotoxin producing fungal pathogen Fusarium graminearum is the causal agent of Fusarium head blight (FHB) of small grain cereals in fields worldwide. Although F. graminearum is highly investigated by means of molecular genetics, detailed studies about hyphal development during initial infection stages are rare. In addition, the role of mycotoxins during initial infection stages of FHB is still unknown. Therefore, we investigated the infection strategy of the fungus on different floral organs of wheat (Triticum aestivum L.) under real time conditions by constitutive expression of the dsRed reporter gene in a TRI5prom::GFP mutant. Additionally, trichothecene induction during infection was visualised with a green fluorescent protein (GFP) coupled TRI5 promoter. A tissue specific infection pattern and TRI5 induction were tested by using different floral organs of wheat. Through combination of bioimaging and electron microscopy infection structures were identified and characterised. In addition, the role of trichothecene production for initial infection was elucidated by a ΔTRI5-GFP reporter strain.
The present investigation demonstrates the formation of foot structures and compound appressoria by F. graminearum. All infection structures developed from epiphytic runner hyphae. Compound appressoria including lobate appressoria and infection cushions were observed on inoculated caryopses, paleas, lemmas, and glumes of susceptible and resistant wheat cultivars. A specific trichothecene induction in infection structures was demonstrated by different imaging techniques. Interestingly, a ΔTRI5-GFP mutant formed the same infection structures and exhibited a similar symptom development compared to the wild type and the TRI5prom::GFP mutant.
The different specialised infection structures of F. graminearum on wheat florets, as described in this study, indicate that the penetration strategy of this fungus is far more complex than postulated to date. We show that trichothecene biosynthesis is specifically induced in infection structures, but is neither necessary for their development nor for formation of primary symptoms on wheat.
Fusarium graminearum Schwabe (teleomorph Gibberella zeae (Schwein) Petch) is the main causal agent of Fusarium head blight (FHB) disease of small grain cereals and cob rot of maize [1–3]. Mycotoxins produced by Fusarium species result in a loss of yield and reduced quality of grains [4–6]. Fusarium toxins including the trichothecenes nivalenol (NIV), deoxynivalenol (DON) and its derivatives 3- and 15-acetyldeoxynivalenol (3-ADON, 15-ADON) contaminate cereal products and have been shown to be harmful to humans, animals, and plants . Hence, the European Union and the United States set limits for DON in final products for human consumption of 0.75 μg/g [Commission Regulation [EC] no. 1881/2006] and of 1 μg/g [Council for Agricultural Science and Technology, 2003]. Trichothecenes are potent phytotoxins for many plants. They can produce symptoms including wilting, chlorosis and necrosis at concentrations of 10-5 to 10-6 M . The toxic effect of trichothecenes is mainly due to their ability to bind to the 60S ribosomal subunit of eukaryotes, resulting in inhibition of protein synthesis and induction of apoptosis . DON is a virulence factor in wheat [9–14]. DON production enables the fungus to spread from infected florets into the wheat rachis [9–13].
Although detailed information of the TRI gene cluster is currently available , the factors inducing mycotoxin production during infection on wheat are unknown. The first step of the trichothecene biosynthesis is catalysed by the enzyme trichodiene synthase encoded by the TRI5 gene [5, 16]. Thus, the TRI5 gene is used as a marker gene for the induction of trichothecene biosynthesis of the fungus [17–20]. Induction assays using axenic cultures revealed TRI5 inducing conditions and substances under laboratory conditions [17, 18, 20–22]. However, little is known about TRI5 inducing factors in planta. Wheat infection of a fungal mutant with a TRI5 promoter GFP (green fluorescent protein) fusion revealed a tissue specific TRI5 induction . A high TRI5 induction in the rachis node and in caryopses was observed. GFP and TRI5 expression were much lower in the adjacent rachis and no GFP fluorescence was observed on anthers, although they were heavily colonised. One objective of the current study was to test different parts of the infected wheat spikelet for tissue specific infection patterns and TRI5 induction. F. graminearum is one of the most intensively studied fungal plant pathogens [3, 6, 23], but our knowledge about fungal development on host surfaces and the penetration strategy of the pathogen during initial infection stages is limited. Thus, another objective of this study was to investigate fungal development and the penetration strategy of F. graminearum by different bioimaging techniques including bright field images, fluorescence microscopy, confocal laser scanning microscopy (CLSM), and scanning electron microscopy (SEM). We performed an in vitro bioassay that allows a continuous microscopic evaluation of detached glumes, lemmas, paleas, and caryopses under comparable conditions. The in vitro bioassay was designed according to Jansen et al. , who performed a similar assay to investigate caryopses of wheat and barley infected with F. graminearum reporter strains. In addition, an in vitro bioassay using previously frozen, detached glumes for microscopic studies of initial infection of different F. graminearum mutants was recently published . In the present study, monitoring of the infection process and TRI5 induction in real time was possible by use of reporter strains. We achieved a continuous observation of fungal development in planta by constitutive expression of the dsRed gene from Discosoma spec.. The expression of GFP gene driven by the endogenous TRI5 promoter in the reporter strain enabled monitoring of the trichothecene induction during infection in real time. Previous studies demonstrated that TRI5prom::GFP exhibits wild type-like growth and infectivity, TRI5 expression and DON production . Infection structures and TRI5 induction were studied on different floret organs of wheat. In the field, FHB disease is initiated by airborne spores landing on flowering spikelets [3, 25, 26]. Open florets during anthesis provide opportunities for the pathogen to contact primary penetration sites. Developing caryopses as well as the adaxial surfaces of lemma and palea are only accessible in open florets and are comparably susceptible to infection [3, 27, 28]. F. graminearum initially colonises the surface of wheat florets without immediate penetration [28, 29]. Most Fusarium species enter husks of wheat and barley by natural openings, such as stomata [3, 29–32], or penetrate epidermal cell walls with short infection hyphae [23, 28, 31, 33–36]. F. graminearum is described as a pathogen that does not form different types of appressoria [23, 34–36]. However, several recent publications provide light microscopy images of lobed, highly septate, and corralloid hyphal structures, which might be involved in penetration of glumes [24, 30, 32]. These authors distinguish between subcuticular coral-like hyphal mats and bulbous infection hyphae. The mitogen-activated protein kinase (MAPK) mutants Δgpmk1 [37, 38] and Δmgv1 , and also the GTPase Δras2 mutant , were tested for their ability to form coral-like subcuticular structures and bulbous infection hyphae. While Δmgv1 and Δras2 mutants were able to form coralloid, subcuticular hyphae and bulbous invasive hyphae similar to those of the wild type strain PH-1, the Δgpmk1 mutant formed coralloid subcuticular hyphae but no bulbous hyphae. Thus, gpmk1 gene of F. graminearum was discussed to be involved in the formation of bulbous infection hyphae. Additionally, first evidence was provided that papillae silica cells are preferred sites for invasion. We describe specific infection structures of F. graminearum wild type isolate 8/1 and reporter strains with 8/1 background. By combination of bioimaging and SEM on floret tissues infected with a TRI5prom::GFP strain and a trichothecene deficient ΔTRI5-GFP strain, the role of trichothecenes for different initial infection stages was evaluated. Comprehensive imaging techniques together with molecular analyses might improve our knowledge about early plant-pathogen interactions during FHB infection.
Screening of infection and TRI5induction in real time
Infection stages I-III on floret organs of wheat and their omnipresent characteristics
Typical fungal morphology
Runner hyphae Infection hyphae
Aerial hyphae Sporodochia
SEM of infection structures
Ultrastructural characterisation of GFP inductive infection structures was performed by combination of fluorescence microscopy and SEM. We identified GFP inductive infection cushions (15-50 μm in diameter) (Figure 2E), lobate appressoria (5-15 μm in diameter) (Figure 2F), and foot structures (4-5 μm in diameter) (Figure 2G). After removal of infection cushions from glumes, SEM revealed numerous penetration pores of about 1-2 μm in diameter in the epidermal cell walls (data not shown).
DON quantification in wheat floret tissues
Initial infection of a DON deficient mutant
Overview of experiments and microscopic methods
Microscopy of infection
Detached in vitroassay
Intact in vivoassay
Cultivar/strain combinations (Figure no.)
Sumai 3/TRI5prom::GFP (2*)
Time points of MZFLIII screening
all cultivar/strain combinations
6 hpi - 14 dpi
(1 A, 2 A-C, 4 A-C, 2 A-C*, 3 A-F*)
6 hpi - 7 dpi (3 A-F*)
Microscopy with Axio Imager Z1
all cultivar/strain combinations
Amaretto/TRI5prom::GFP (3 G*)
Nandu/TRI5prom::GFP (2 D, 1*)
Nandu/TRI5prom::GFP (2 E-F)
Nandu/ΔTRI5-GFP (4 D-F)
Infection stages and infection structures of F. graminearumon wheat
The colonisation of the inside of the wheat floret tissues by F. graminearum was evaluated in detail [12, 20, 28, 29, 54, 55], but information about fungal development on different wheat tissues and the penetration strategy of the fungus is limited. Three successive infection stages (stage I-III) were distinguishable on all floret tissues.
We did not observe disease symptoms during stage I. This is consistent with previous findings that hyphae of F. graminearum initially branch symptomlessly on the exterior surfaces of floret tissues from wheat and barley, and do not penetrate the epidermis immediately after germination [6, 29, 31]. The disease symptoms of spelts and caryopses as well as sporodochia production described for stage III confirm earlier descriptions of late infection stages of FHB on floret wheat tissues [6, 12, 32]. A very surprising result was the formation of compound appressoria during stage II of infection. Lobate appressoria and infection cushions are two types of so called compound appressoria . They are described as multicellular types of appressoria, formed by irregularly shaped hyphae . F. graminearum develops compound appressoria with striking morphological similarities to other fungal plant pathogens e.g. Rhizoctonia solani [40, 42, 48, 52, 53], Botrytis cinerea [46, 49], and Sclerotinia sclerotiorum [44, 47]. Previous publications provided the first microscopic evidences for more complex infection structures formed by F. graminearum [24, 30, 32]. Two different structures were described, namely coral-like hyphal mats [24, 30, 32] and bulbous infection hyphae . Coral-like hyphal structures were further specified by lobed, thickened, and branched hyphae [24, 30, 32]. We suggest that the coral-like hyphal mats are infection cushions, whereas the bulbous infection hyphae correlate to foot structures. However, coral-like infection structures were observed already at 24 hpi on glumes, while infection cushions appeared on glumes at 7 dpi in our assays. The difference might be explained by strain specific variations between the European wild type isolate Fg 8/1 we used, and the American strain PH1. Furthermore, the investigators studying PH1 used detached glumes, which were stored frozen before inoculation. In contrast to fresh detached glumes as used in our studies, the defence reactions of refrozen plant cells might be strongly reduced.
F. graminearum is commonly described to enter floret tissues of cereals by direct penetration via infection hyphae or by natural openings, such as stomata [14, 29, 30, 32]. Penetration through stomata by lobate appressoria and infection cushions was observed only occasionally during stage II, but seems to be undirected. The earliest infection structures observed are infection hyphae. Short infection hyphae are described in detail for different Fusarium species by ultrastructural studies using TEM and SEM [27, 28, 33, 56]. In our studies, infection hyphae were visible on all wheat organs during stage I and II. We were not able to appraise the number of actually penetrating infection hyphae during stage I. Thus, the impact of infection hyphae for further disease progression is not elucidated. Interestingly, the tissues remained macroscopically asymptomatic until necrotic lesions surrounding infection cushions appeared during stage II. Necrotic lesions on cotton hypocotyls infected with R. solani appeared when infection cushions were fully developed . This is consistent with our observations that lesions develop mainly around bigger infection cushions (Figure 1A and 4C).
Compound appressoria were formed on different types of tissues, like caryopses and spelts, but, depending on the type of organ, at different time points after inoculation (data not shown). In summary, the results demonstrate that compound appressoria are formed independently of the biological function and morphological characteristics of different organs. They were formed on vegetative organs with silicified epidermal cells, but also on the pericarp of the caryopsis without silica cells. Silicified epidermal cells seem to be a preferred site of penetration, but are not a prerequisite of successful infection. Developing caryopses are highly susceptible for infection due to the absence for cell wall thickenings in the pericarp and underlying tissues. Additionally, the results exclude a dependence of compound appressoria formation on certain topographical features, because the epidermal architecture of bracts and caryopses is fundamentally different. Topographical features of the inoculated surface , the availability of nutrients [40, 57] and plant exudates [40, 43, 57–59] were discussed to be influencing factors for development and morphology of compound appressoria from R. solani. Several abiotic factors which influence fungal growth and development, like humidity, temperature, exposure to light, and nutrient availability will probably influence the development of compound appressoria. For example, exposure to light has been shown to influence infection cushion formation of R. solani . We propose that foot structures, lobate appressoria, and infection cushions mirror different developmental stages of infection cushion formation, similar to R. solani [40, 50]. A schematic model that illustrates the development of infection cushions by R. solani is provided by Armentrout and Downer . Furthermore, a development of lobate appressoria into infection cushions is described for R. solani , B. cinerea , and S. sclerotiorum . The increasing size and complexity of cellular structures observed during the time of infection supports the idea of a developmental process. It is currently unknown whether infection hyphae of F. graminearum, observed during stage I are involved in the development of compound appressoria.
In comparison to infection cushions, lobate appressoria are smaller and formed by fewer cells. They can be formed by a single lobate cell, but two-celled to multi-celled types are described as well . In general, hyphae of lobate appressoria are short, swollen, and highly septate . Each lobe of a lobate appressorium can form an infection peg . The development of compound appressoria from epiphytic mycelium is common for several other phytopathogenic fungi . Direct penetration of epidermal cells by infection hyphae, infection cushions, and lobate appressoria was evident by CLSM (Figure 2D and Additional file 1). The presence of penetration pores in the outer epidermal cell wall underneath infection cushions provides a hint for numerous penetration pegs. Many penetration pores resulting from penetration pegs of infection cushions were demonstrated by comparable ultrastructural studies on S. sclerotiorum  and R. solani [45, 53]. The primary hyphae from which compound appressoria originate are termed runner or running hyphae in other infection cushion producing fungi such as R. solani [45, 50], several Sclerotinia species [41, 47, 61] and Gaeumannomyces graminis, the causal agent of take-all patch disease [62, 63]. The observed runner hyphae are clearly distinguishable from other functionally specified hyphae, e.g. hyphae that form infection structures, aerial hyphae or reproductive hyphae (e.g. conidiophores and ascogenic hyphae).
The early infection process of susceptible and resistant wheat cultivars (Additional file 2 and 3) were indistinguishable. Infection structure formation as well as DON induction occurred comparably. This is consistent with the fact that type II resistance of Sumai 3 and Amaretto may prevent systemic infection of the wheat spikes, but does not prevent initial infection of the inoculated wheat spikelet [64–66]. An artificial effect on compound appressoria formation due to the dissection of floral organs was ruled out by microscopic evaluation of inoculated spikelets from intact potted wheat plants. The investigation demonstrated infection cushion formation on the surface of paleas, lemmas, and caryopses (Additional file 3). Glumes were not colonised by hyphae and showed no infection cushions at 4 dpi. The difference in colonisation between glumes and adaxial surfaces of paleas, lemmas, and on caryopses might depend on the applied inoculation method. Injecting conidia inside the wheat floret provides no initial contact of conidia to the glume surface. In bioassays using detached wheat tissues, infection cushions were formed later compared to tissues of intact plants. This might be explained by differences in humidity, light quality, and temperature differences. Adding additional nutritions, i.e. sugars, to the detached flower leaf assays resulted in much shorter infection times. Nevertheless, all different infection structures were formed at 2-3 dpi (data not shown).
Infection structures and DON induction
Previous infection studies with TRI5 knockout mutants on wheat revealed that the trichothecene deficient mutant is still able to infect the inoculated wheat spikelet like wild type [9, 11–13]. Therefore, trichothecenes seem to be of minor importance for initial infection stages on wheat. In contrast, a major role of trichothecenes for the initial establishment in the host tissue was suggested , because induction of TRI5 expression was detected during early infection stages on barley spikes infected with F. graminearum  as well as on seedlings of wheat infected with F. culmorum . A tissue specific induction of the TRI5 pathway during spike infections was indicated recently . In the present study we demonstrated that TRI5 expression is specifically induced in infection structures. The detection of high amounts of DON in glumes and caryopses infected with TRI5prom::GFP (Figure 3) confirmed that visible GFP fluorescence correlates to DON production of the mutant. Interestingly, infection structures and necrotic lesions are formed independently of trichothecene production. Several explanations seem possible. Firstly, the lesions surrounding the infection cushions are caused by the multiple penetration pores. These cellular destructions might induce host defence responses, similar to plant reactions by wounding (e.g. oxidative burst, apoptosis, modifications of the plant cell wall). Secondly, virulence factors, like an already described secreted lipase  and most likely other not yet discovered factors, act independently of DON, cause the observed destruction, and are responsible for the initial infection. The question remains why DON is induced, even though it does not contribute to the virulence of the fungus at this time of infection. DON is necessary to suppress plant defence enabling the pathogen to break through the rachis node. DON production is strongly induced, most likely by the host, at this point of infection [12, 20]. It seems possible that similar host factors induce DON at other stages of infection, for example during the penetration of the cuticle. This might explain why a DON deficient mutant colonises maize cobs similar to wild type, although the wild type produced high levels of DON during the infection .
Different host compounds can be discussed to be responsible for TRI5 induction during infection. Nitrogen and carbon sources as well as low pH play key roles in regulation of mycotoxins produced by Aspergillus species, such as sterigmatocystin and aflatoxin [69, 70]. Many nitrogen containing substances like various amines were identified that significantly induce TRI5 expression . The amine putrecine induced TRI5 expression and mycotoxin production in vitro to levels observed during infection . In addition, it was demonstrated that low extracellular pH is required for DON production in axenic culture . A combination of low pH and amines results in significantly enhanced expression of the TRI5 gene and increased DON production. The factors responsible for TRI5 induction of infection structures in planta has to be evaluated in further investigations.
We provided here the first evidence that F. graminearum is able to form lobate appressoria and infection cushions during FHB infection. It is generally believed that Fusarium species invade host tissues without generating an appressorium [23, 24, 34, 35]. In the present study we demonstrated that the penetration strategy of F. graminearum on wheat florets is more complex than postulated until now. Compound appressoria were formed on different types of tissues like caryopses and husks. Therefore, a tissue independent formation of compound appressoria is demonstrated. A major role of cushion formation on symptom development is suggested by necrotic lesions and penetration pores underneath cushions. A specific induction of trichothecenes in infection structures was demonstrated by CLSM. Consequently, a relation between DON production and direct penetration was investigated. Interestingly, infections with a trichothecene deficient mutant revealed no differences compared to infections with trichothecene producing strains. Trichothecene biosynthesis is specifically induced in infection structures, but not a prerequisite for their development and the initial penetration of wheat tissues. In summary, the combination of different bioimaging techniques with functional reporter strains and electron microscopy provided new insights into the penetration strategy of F. graminearum and the role of trichothecene induction during initial infection of wheat. A detailed knowledge about early development of FHB might help to explore new ways of disease control.
The susceptible wheat cultivar Nandu (Lochow-Petkus, Bergen-Wohlde, Germany), the resistant Chinese wheat cultivar Sumai 3 and the semi-resistant cultivar Amaretto (B. Bauer, Niedertraubling, Germany, FHB resistance category 3) were grown in the greenhouse in plastic pots at 18-20°C, 60% relative humidity, and a photoperiod of 16 h.
Fungal material and preparation of inoculum
To investigate the initial stages of the infection on wheat florets we used a previously described TRI5prom::GFP reporter mutant . Localisation of the mycelium was possible due to constitutive expression of the dsRed gene under control of the glycerol-3-phosphate dehydrogenase (gpdA) promoter of Aspergillus nidulans. To evaluate the induction of DON during infection, the green fluorescence protein (GFP) gene was fused to the promoter of the TRI5 gene, coding for the trichodiene synthase of the fungus. Mutants were generated as described previously . The resulting TRI5prom::GFP mutant consists of a fully functional TRI5 gene and exhibits GFP fluorescence driven by an endogenous TRI5 promoter . The second reporter strain used (ΔTRI5-GFP) is DON deficient and expresses GFP constitutively under the control of gpdA promoter, which enables the detection of mycelium during infection under real time conditions . Both F. graminearum reporter strains were generated by transformation of the wild type isolate Fg 8/1 .
Vegetative conidia of F. graminearum strains were obtained as described previously . The concentration of conidia suspension was adjusted to 2 × 10 4 conidia/ml and stored at -70°C.
Detached in vitrobioassay
For the detached in vitro bioassay, spikelets of three-month-old wheat plants were taken at anthesis to isolate floret organs including caryopses, paleas, lemmas and glumes. Organs were detached from the floret with a razor blade and placed in Petri dishes (92 × 16 mm, SARSTEDT) on 1.6% (w/v) water agar (Difco granulated agar; Becton Dickinson). Four Petri dishes contained 8 biological replicates of one floret organ and represented one independent experiment. The ventral side of caryopses and the adaxial side of glumes, lemmas and paleas were inoculated with 5 μl sterile water containing 2 × 104 conidia/ml. After inoculation, the Petri dishes were sealed with Parafilm (Pechiney, Chicago, USA) and incubated in a growth chamber at 16 h light period with 18°C and 16°C at darkness. Floret organs of the susceptible cultivar Nandu and the resistant Chinese wheat cultivar Sumai 3 were inoculated equally with the TRI5prom::GFP strain to test for cultivar dependent differences during infection. Floret tissues of Sumai 3 plants were inoculated with 2.5 μl of a 4 × 104 conidia/ml water suspension. Conidia of a ΔTRI5-GFP mutant were used for inoculation to study infections of floret organs under trichothecene deficient conditions. Floret organs of the susceptible cultivar Nandu infected with conidia of the wild type isolate Fg 8/1 served as a control for the wild type-like character of observations derived from the TRI5prom::GFP strain.
Intact in vivobioassay
To test for artificial effects due to wounding and detachment from the plant in the in vitro bioassay, intact spikelets on potted wheat plants inoculated with macroconidia of TRI5prom::GFP were investigated microscopically. Spike inoculations were performed with three-month-old wheat plants at anthesis . 10 μl of conidia suspension containing 2 × 104 conidia/ml were injected into the cavity between lemma and palea. The incubation took place in a growth chamber under similar conditions as described for detached in vitro assay. The susceptible cultivar Nandu and the semi-resistant cultivar Amaretto were investigated equally.
Monitoring of TRI5induction during infection
The infection was studied in a two step process. Firstly, we screened infected organs using the MZFLIII microscope. Thereby fungal development, TRI5 induction and disease symptoms of the entire surface of the same sample were studied from conidia germination until sporulation. The typical stages of infection and TRI5 induction on different floret tissues were identified by the screening with MZFLIII. In the second step, we characterised TRI5 inductive fungal structures in detail by epifluorescence microscopy, CLSM, and SEM.
Screening of infection
Organs infected with the TRI5prom::GFP strain in in vitro bioassays were monitored with a MZFLIII microscope (see below) at 6, 12, and 24 hpi. From 24 hpi onward investigations proceeded in 1 day intervals until 14 dpi. Ten independent inoculation experiments (n = 8) were performed with organs of the cultivar Nandu infected with the TRI5prom::GFP strain provided similar results. The role of trichothecenes for the initial infection was evaluated in in vitro bioassays by using a ΔTRI5-GFP mutant for inoculation of floret organs of the cultivar Nandu. The colonisation of the host and plant necrosis was investigated with MZFLIII microscope at given above time points from 6 hpi to 14 dpi. Wheat organs of the resistant cultivar Sumai 3 were infected with the TRI5prom::GFP strain and investigated for cultivar dependent differences in colonisation, TRI5 induction, and plant necroses at time points given above. Floret organs infected with TRI5prom::GFP strain from attached in vivo assays were examined at a one day interval from 3 dpi to 7 dpi. We used white light and fluorescence microscopy of MZFLIII microscope to examine the colonisation, TRI5 induction and plant necroses. In vivo assays of the intact spikelet of potted wheat plants (n = 2) were repeated three times with similar results. Floret organs of the susceptible cultivar Nandu infected with conidia of the wild type isolate Fg 8/1 were investigated with MZFLIII microscope at given time points from 6 hpi to 14 dpi. Three independent experiments (n = 8) were performed with floral tissues of Sumai 3 infected with the TRI5prom::GFP strain and floral tissues of the cultivar Nandu infected with Fg 8/1 or the ΔTRI5-GFP mutant.
MZFLIII light microscopy
Infected floret organs were investigated with MZFLIII microscope (Leica Microsystems, Heerbrugg, Switzerland) in air without preparation, lying in Petri dishes. Inclined reflected light of an external halogen lamp KL 1500 Electronic (Schott, Mainz, Germany) was used to visualise plant necroses as well as the mycelium under white light conditions with Leica MZFLIII microscope. The dsRed fluorescence of the TRI5prom::GFP strain was detected with the Leica dsRed filter set containing an excitation filter at 546/12 nm and a long pass filter at 560 nm. The GFP fluorescence of the TRI5prom::GFP and ΔTRI5-GFP strain was visible by Leica GFP filter set with an excitation filter at 470/40 nm and a band pass filter transmitting light at 525/50 nm. To investigate the infection of the F. graminearum wild type 8/1, plant tissues were incubated in 96% ethanol for fixation and removal of chlorophyll. The mycelium was stained with 0.1% (w/v) trypan blue solution (Fluka analytical) in 10% (v/v) acetic acid for 20 minutes at room temperature. Excessive stain was removed by rinsing samples with distilled water. Samples were cut in pieces and transferred on glass slides for white light images of infected tissues. The Leica MZFLIII fluorescence microscope was equipped with a Leica 1.0 × objective. Photos were done with Leica DFC 500 coloured camera. The LAS Leica software (version 2.7.1) was used for image acquisition and procession.
Microscopy of infection structures
Bright field and epifluorescence microscopy
To investigate infection structures of the F. graminearum wild type 8/1 we used bright field microscopy with transmitted light of a Zeiss Axio Imager.Z1 microscope. Infection structures of reporter strains were investigated by fluorescence microscopy using Zeiss Axio Imager.Z1 microscope equipped with a Zeiss Apotome. A UV (ultra violet) lamp HAL 100 served as UV light source. DsRed was excited in the range of 538 to 562 nm and detected in the 570 to 640 nm range. GFP was excited with 450 to 490 nm and detected at 500 to 550 nm wavelength. The plant apoplast was excited in the range of 335 to 383 nm. The blue autofluorescence was detected in the 420 to 470 nm range. Images were taken with Zeiss AxioCam MRm CCD camera. Image processing, including overlay of different fluorescence channels and generation of maximum intensity projections (MIP) of z-stacks were done with Zeiss AxioVision software (version 4.8.1).
Laser scanning microscopy
To investigate the penetration of the epidermal layer through compound appressoria of F. graminearum laser scanning microscopy was performed. Paleas and glumes infected with TRI5prom::GFP were analysed with Leica TCS SPE microscope (Leica Microsystems, Wetzlar, Germany). DsRed was excited at 532 nm and detected in the 560 to 683 nm range. GFP was excited at 488 nm and detected in the 520 to 631 nm range. Autofluorescence of the plant apoplast was excited at 405 nm and detected in the 408 nm to 464 nm range. The sample shown in Figure 2D and Additional file 1 represents an area of 275 × 275 μm in xy-dimension. 22.47 μm were scanned by 107 steps in z-dimension. Image processing, maximum projection, and data analyses were done with the Leica LAS AF software.
Scanning electron microscopy
Four glumes from detached in vitro bioassays infected with TRI5prom::GFP or ΔTRI5-GFP were sampled each at 8 dpi. The glumes were fixed with 4% (v/v) glutaraldehyde in 50 mM phosphate buffer (pH 6.8) for 8-10 h at 4°C, then rinsed with the same buffer for 3 h. Afterwards, samples were post-fixed with 1% (w/v) osmium tetroxide in the same buffer for 2 h at 4°C. After dehydration for 24 h by a graded acetone series at room temperature, the samples were critical-point dried, mounted on stubs, and sputter-coated with gold. The scanning electron microscope SEM LEO 1525 was used operating at 6 kV.
DON quantification in wheat floret tissues
To confirm that an optical detection of GFP fluorescence of TRI5prom::GFP reporter strain resulted in a production of trichothecenes, the concentration of DON in ppb (parts per billion) of fresh weight of infected glumes and caryopses was quantified after GFP fluorescence of infected samples was observed by fluorescence microscopy using MZFLIII microscope. DON measurements were carried out by using the RIDASCREEN DON enzymatic immunoassay kit (R-Biopharm, Darmstadt, Germany). 28 infected glumes and caryopses were pooled and weighed at 8 dpi. Water inoculated glumes at 8 dpi were used as negative control. Pooled samples were pestled in liquid nitrogen and homogenates were diluted 1:5 (w/v) with sterile water according to respective fresh weight. Samples had been shaken for 30 min at 1500 rpm and 25°C in the thermomixer comfort (Eppendorf, Hamburg, Germany) for DON extraction. By centrifugation for 10 minutes at 25°C and 3500 rpm in the centrifuge MiniSpin (Eppendorf, Hamburg, Germany), the supernatant was freed from cell debris. 50 μl of the respective extract was used in the DON assay. The following experimental procedure, measurement and calculation were done according to RIDASCREEN DON kit manual. The extinction was measured by photometry at 450 nm by a 96-well-ELISA-reader Anthos 2010 (Mikrosysteme GmbH, Krefeld, Germany). The measurements were repeated three times for statistical analyses. The DON- concentration of the extracts was estimated by a calibration curve with DON standards. Calculations, statistics and graphics were done by using Microcal Origin calculation software (version 5.0).
We thank Brigitte Doormann, Peter Ilgen, and Dr. Jörg Bormann (Molecular Phytopathology and Genetics, Biocenter Klein Flottbek, University of Hamburg) for critical reading of the manuscript. Furthermore, we are grateful to Dr. Frank Friedrich and Renate Walter (Biocenter Grindel, University of Hamburg), Karen Dehn, and Elke Woelken (Systematics and Cell Biology, Biocenter Klein Flottbek, University of Hamburg) for their technical support during CLSM and electron microscopy, and Peter Ilgen for advice during fluorescence microscopy.
- Bai S, Shaner G: Scab of wheat: prospects for control. Plant Dis. 1994, 78 (8): 760-766. 10.1094/PD-78-0760.View ArticleGoogle Scholar
- McMullen M, Jones R, Gallenberg D: Scab of wheat and barley: a re-emerging disease of devastating impact. Plant Dis. 1997, 81 (12): 1340-1348. 10.1094/PDIS.19220.127.116.110.View ArticleGoogle Scholar
- Trail F: For blighted waves of grain: Fusarium graminearum in the postgenomics era. Plant Physiol. 2009, 149 (1): 103-110. 10.1104/pp.108.129684.PubMedPubMed CentralView ArticleGoogle Scholar
- Desjardins AE, Hohn TM: Mycotoxins in plant pathogenesis. MPMI. 1997, 10 (2): 147-152. 10.1094/MPMI.1918.104.22.168.View ArticleGoogle Scholar
- Desjardins AE, Hohn TM, McCormick SP: Trichothecene biosynthesis in Fusarium species: chemistry, genetics, and significance. Microbiol Mol Biol Rev. 1993, 57 (3): 595-604.Google Scholar
- Goswami RS, Kistler HC: Heading for disaster: Fusarium graminearum on cereal crops. Mol Plant Path. 2004, 5 (6): 515-525. 10.1111/j.1364-3703.2004.00252.x.View ArticleGoogle Scholar
- Cutler HG: Trichothecenes and their role in the expression of plantdisease. In Biotechnology for crop protection. Volume 379. Edited by: HedinPA, Menn JJ, Hollingworth RM. Washington DC: The American ChemicalSociety; 1988:50-72.View ArticleGoogle Scholar
- Rocha O, Ansari K, Doohan FM: Effects of trichothecene mycotoxins on eukaryotic cells: A review. Food Addit Contam. 2005, 22 (4): 369-378. 10.1080/02652030500058403.PubMedView ArticleGoogle Scholar
- Proctor RH, Hohn TM, McCormick SP: Reduced virulence of Gibberella zeae caused by disruption of a trichothecene toxin biosynthetic gene. MPMI. 1995, 8 (4): 593-601. 10.1094/MPMI-8-0593.PubMedView ArticleGoogle Scholar
- Desjardins AE, Proctor RH, Bai GH, McCormick SP, Shaner G, Buechley G, Hohn TM: Reduced virulence of trichothecene-nonproducing mutants of Gibberella zeae in wheat field tests. MPMI. 1996, 9 (9): 775-781. 10.1094/MPMI-9-0775.View ArticleGoogle Scholar
- Bai GH, Desjardins AE, Plattner RD: Deoxynivalenol-nonproducing Fusarium graminearum causes initial infection, but does not cause disease spread in wheat spikes. Mycopathologia. 2002, 153 (2): 91-98. 10.1023/A:1014419323550.PubMedView ArticleGoogle Scholar
- Jansen C, von Wettstein D, Schäfer W, Kogel KH, Felk A, Maier FJ: Infection patterns in barley and wheat spikes inoculated with wild-type and trichodiene synthase gene disrupted Fusarium graminearum. PNAS. 2005, 102 (46): 16892-16897. 10.1073/pnas.0508467102.PubMedPubMed CentralView ArticleGoogle Scholar
- Maier FJ, Miedaner T, Hadeler B, Felk A, Salomon S, Lemmens M, Kassner H, Schäfer W: Involvement of trichothecenes in fusarioses of wheat, barley and maize evaluated by gene disruption of the trichodiene synthase (Tri5) gene in three field isolates of different chemotype and virulence. Mol Plant Path. 2006, 7 (6): 449-461. 10.1111/j.1364-3703.2006.00351.x.View ArticleGoogle Scholar
- Cuzick A, Urban M, Hammond Kosack K: Fusarium graminearum gene deletion mutants map1 and tri5 reveal similarities and differences in the pathogenicity requirements to cause disease on Arabidopsis and wheat floral tissue. New Phytologist. 2008, 177 (4): 990-1000. 10.1111/j.1469-8137.2007.02333.x.PubMedView ArticleGoogle Scholar
- Kimura M, Tokai T, Takahashi-Ando N, Ohsato S, Fujimura M: Molecular and genetic studies of Fusarium trichothecene biosynthesis: Pathways, genes, and evolution. Biosci Biotech Biochem. 2007, 71 (9): 2105-2123. 10.1271/bbb.70183.View ArticleGoogle Scholar
- Hohn TM, Desjardins AE: Isolation and gene disruption of the Tox5 gene encoding trichodiene synthase in Gibberella pulicaris. MPMI. 1992, 5 (3): 249-256. 10.1094/MPMI-5-249.PubMedView ArticleGoogle Scholar
- Gardiner DM, Kazan K, Manners JM: Nutrient profiling reveals potent inducers of trichothecene biosynthesis in Fusarium graminearum. Fungal Genet Biol. 2009, 46 (8): 604-613. 10.1016/j.fgb.2009.04.004.PubMedView ArticleGoogle Scholar
- Gardiner DM, Osborne S, Kazan K, Manners JM: Low pH regulates the production of deoxynivalenol by Fusarium graminearum. Microbiology-SGM. 2009, 155: 3149-3156. 10.1099/mic.0.029546-0.View ArticleGoogle Scholar
- Doohan FM, Weston G, Rezanoor HN, Parry DW, Nicholson P: Development and use of a reverse transcription-PCR assay to study expression of Tri5 by Fusarium species in vitro and in planta. Appl Environ Microbiol. 1999, 65 (9): 3850-3854.PubMedPubMed CentralGoogle Scholar
- Ilgen P, Hadeler B, Maier FJ, Schäfer W: Developing kernel and rachis node induce the trichothecene pathway of Fusarium graminearum during wheat head infection. MPMI. 2009, 22 (8): 899-908. 10.1094/MPMI-22-8-0899.PubMedView ArticleGoogle Scholar
- Covarelli L, Turner AS, Nicholson P: Repression of deoxynivalenol accumulation and expression of Tri genes in Fusarium culmorum by fungicides in vitro. Plant Pathol. 2004, 53 (1): 22-28. 10.1111/j.1365-3059.2004.00941.x.View ArticleGoogle Scholar
- Lemmens M, Haim K, Lew H, Ruckenbauer P: The effect of nitrogen fertilization on Fusarium head blight development and deoxynivalenol contamination in wheat. J Plant Pathol. 2004, 152 (1): 1-8. 10.1046/j.1439-0434.2003.00791.x.Google Scholar
- Kikot GE, Hours RA, Alconada TM: Contribution of cell wall degrading enzymes to pathogenesis of Fusarium graminearum: a review. J Basic Microbiol. 2009, 49 (3): 231-241. 10.1002/jobm.200800231.PubMedView ArticleGoogle Scholar
- Rittenour WR, Harris SD: An in vitro method for the analysis of infection-related morphogenesis in Fusarium graminearum. Mol Plant Path. 2010, 11 (3): 361-369. 10.1111/j.1364-3703.2010.00609.x.View ArticleGoogle Scholar
- Arthur JC: Wheat scab. Indiana Agricultural Experiment Station. 1891, 36: 129-132.Google Scholar
- Strange RN, Smith H: Fungal growth stimulant in anthers which predisposes wheat to attack by Fusarium graminearum. Physiol Plant Pathol. 1971, 1 (2): 141-150. 10.1016/0048-4059(71)90023-3.View ArticleGoogle Scholar
- Kang ZS, Buchenauer H: Cytology and ultrastructure of the infection of wheat spikes by Fusarium culmorum. Mycol Res. 2000, 104: 1083-1093. 10.1017/S0953756200002495.View ArticleGoogle Scholar
- Wanjiru WM, Kang ZS, Buchenauer H: Importance of cell wall degrading enzymes produced by Fusarium graminearum during infection of wheat heads. Eur J Plant Pathol. 2002, 108 (8): 803-810. 10.1023/A:1020847216155.View ArticleGoogle Scholar
- Bushnell WR, Hazen BE, Pritsch C: Histology and physiology of Fusariumhead blight. In Fusarium Head Blight of Wheat & Barley. Edited by: LeonardKJ, Bushnell WR. St. Paul, Minnesota, USA APS Press; 2003:44-83.Google Scholar
- Boddu J, Cho S, Kruger WM, Muehlbauer GJ: Transcriptome analysis of the barley-Fusarium graminearum interaction. MPMI. 2006, 19 (4): 407-417. 10.1094/MPMI-19-0407.PubMedView ArticleGoogle Scholar
- Kang Z, Buchenauer H: Ultrastructural and immunocytochemical investigation of pathogen development and host responses in resistant and susceptible wheat spikes infected by Fusarium culmorum. Physiol Mol Plant Pathol. 2000, 57 (6): 255-268. 10.1006/pmpp.2000.0305.View ArticleGoogle Scholar
- Pritsch C, Muehlbauer GJ, Bushnell WR, Somers DA, Vance CP: Fungal development and induction of defense response genes during early infection of wheat spikes by Fusarium graminearum. MPMI. 2000, 13 (2): 159-169. 10.1094/MPMI.2000.13.2.159.PubMedView ArticleGoogle Scholar
- Kang ZS, Zingen-Sell I, Buchenauer H: Infection of wheat spikes by Fusarium avenaceum and alterations of cell wall components in the infected tissue. Eur J Plant Pathol. 2005, 111 (1): 19-28. 10.1007/s10658-004-1983-9.View ArticleGoogle Scholar
- Cuomo CA, Gueldener U, Xu JR, Trail F, Turgeon BG, Di Pietro A, Walton JD, Ma LJ, Baker SE, Rep M, Adam G, Antoniw J, Baldwin T, Calvo S, Chang YL, DeCaprio D, Gale LR, Gnerre S, Goswami RS, Hammond-Kosack K, Harris LJ, Hilburn K, Kennell JC, Kroken S, Magnuson JK, Mannhaupt G, Mauceli E, Mewes HW, Mitterbauer R, Muehlbauer G, et al: The Fusarium graminearum genome reveals a link between localized polymorphism and pathogen specialization. Science. 2007, 317 (5843): 1400-1402. 10.1126/science.1143708.PubMedView ArticleGoogle Scholar
- Mendgen K, Hahn M, Deising H: Morphogenesis and mechanisms of penetration by plant pathogenic fungi. Annu Rev Phytopathol. 1996, 34 (1): 367-386. 10.1146/annurev.phyto.34.1.367.PubMedView ArticleGoogle Scholar
- Bluhm BH, Zhao X, Flaherty JE, Xu JR, Dunkle LD: RAS2 regulates growth and pathogenesis in Fusarium graminearum. MPMI. 2007, 20 (6): 627-636. 10.1094/MPMI-20-6-0627.PubMedView ArticleGoogle Scholar
- Jenczmionka NJ, Maier FJ, Lösch AP, Schäfer W: Mating, conidiation and pathogenicity of Fusarium graminearum, the main causal agent of the head-blight disease of wheat, are regulated by the MAP kinase gpmk1. Curr Genet. 2003, 43 (2): 87-95.PubMedGoogle Scholar
- Urban M, Mott E, Farley T, Hammond-Kosack K: The Fusarium graminearum MAP1 gene is essential for pathogenicity and development of perithecia. Mol Plant Path. 2003, 4 (5): 347-359. 10.1046/j.1364-3703.2003.00183.x.View ArticleGoogle Scholar
- Hou Z, Xue C, Peng Y, Katan T, Kistler HC, Xu JR: A mitogen-activated protein kinase gene (MGV1) in Fusarium graminearum is required for female fertility, heterokaryon formation, and plant infection. MPMI. 2002, 15 (11): 1119-1127. 10.1094/MPMI.2002.15.11.1119.PubMedView ArticleGoogle Scholar
- Armentrout VN, Downer AJ: Infection cushion development by Rhizoctonia solani on cotton. Phytopathology. 1987, 77 (4): 619-623. 10.1094/Phyto-77-619.View ArticleGoogle Scholar
- Boyle C: Studies in the physiology of parasitism VI. infection by Sclerotinia Libertiana. Ann Bot-London. 1921, 337-3Google Scholar
- Demirci E, Döken MT: Host penetration and infection by the anastomosis groups of Rhizoctonia solani Kühn isolated from potatoes. Turk J Agric For. 1998, 22: 609-613.Google Scholar
- EI-Samra IA, El-Faham YM, Kamara AM: Selective induction of infection cushions by Rhizoctonia solani in relation to host responses. Phytopathol Z. 1981, 102: 122-126.View ArticleGoogle Scholar
- Emmett RW, Parbery DG: Appressoria. Annu Rev Phytopathol. 1975, 13 (1): 147-165. 10.1146/annurev.py.13.090175.001051.View ArticleGoogle Scholar
- Hofman TW, Jongebloed PHJ: Infection process of Rhizoctonia solani on Solanum tuberosum and effects of granular nematicides. Eur J Plant Pathol. 1988, 94 (5): 243-252.Google Scholar
- Huang HC, Kokko EG, Erickson RS: Infection of alfalfa pollen by Botrytis cinerea. Bot Bull Acad Sin. 1999, 40 (1): 101-106.Google Scholar
- Huang L, Buchenauer H, Han Q, Zhang X, Kang Z: Ultrastructural and cytochemical studies on the infection process of Sclerotinia sclerotiorum in oilseed rape. J Plant Dis Protect. 2008, 115 (1): 9-16.Google Scholar
- Pannecoucque J, Hofte M: Interactions between cauliflower and Rhizoctonia anastomosis groups with different levels of aggressiveness. BMC Plant Biology. 2009, 9 (95).Google Scholar
- Tenberge KB: Infection sites and infection structures. In Botrytis: Biology, Pathology and Control. Edited by: Elad Y, Williamson B, Tudzynski P, Delen N. Dordrecht, The Netherlands: Kluwer Academic Publishers; 2004:74-84.Google Scholar
- Weihold AR, Sinclair JB: Rizoctonia solani: Penetration, Colonization and Host Response. Rhizoctonia species: Taxonomy, molecular biology, ecology, pathology and disease control. Edited by: Sneh B, Jabaji-Hare S, Neate S, Dijst G. Dordrecht, The Netherlands: Kluwer Academic Publishers; 1996:163-175.View ArticleGoogle Scholar
- Flentje NT, Dodman RL, Kerr A: The mechanism of host penetration by Thanatephorus cucumeris. Aust J Biol Sci. 1963, 16: 784-799.Google Scholar
- Marshall DS, Rush MC: Infection cushion formation on rice sheaths by Rhizoctonia solani. Phytopathology. 1980, 70 (10): 947-950.View ArticleGoogle Scholar
- Matsuura K: Scanning electron microscopy of the infection process of Rhizoctonia solani in leaf sheaths of rice plants. Phytopathology. 1986, 76 (8): 811-814. 10.1094/Phyto-76-811.View ArticleGoogle Scholar
- Ribichich KF, Lopez SE, Vegetti AC: Histopathological spikelet changes produced by Fusarium graminearum in susceptible and resistant wheat cultivars. Plant Dis. 2000, 84 (7): 794-802. 10.1094/PDIS.2000.84.7.794.View ArticleGoogle Scholar
- Brown NA, Urban M, van de Meene AML, Hammond-Kosack KE: The infection biology of Fusarium graminearum: Defining the pathways of spikelet to spikelet colonisation in wheat ears. Fungal Biology. 2010, 114 (7): 555-571.PubMedView ArticleGoogle Scholar
- Kang Z, Huang L, Buchenauer H: Ultrastructural and cytochemical studies on infection of wheat spikes by Microdochium nivale. J Plant Dis Protect. 2004, 111 (4): 351-361.Google Scholar
- Stockwell V, Hanchey P: The role of the cuticle in resistance of beans to Rhizoctonia solani. Phytopathology. 1983, 73 (12): 1640-1642. 10.1094/Phyto-73-1640.View ArticleGoogle Scholar
- Aziz NH, El-Fouly MZ, El-Essawy AA, Khalaf MA: Influence of bean seedling root exudates on the rhizosphere colonization by Trichoderma lignorum for the control of Rhizoctonia solani. Bot Bull Acad Sin. 1997, 38: 33-39.Google Scholar
- Reddy MN: Studies on groundnut hypocotyl exudates and the behaviour of Rhizoctonia solani in influencing the disease. Plant Soil. 1980, 55 (3): 445-454. 10.1007/BF02182704.View ArticleGoogle Scholar
- Keijer JWA, Sinclair JB: Plant-Pathogen Interactions of Rhizoctonia spp. Rhizoctonia species: Taxonomy, molecular biology, ecology, pathology and disease control.Edited by: Sneh B, Jabaji-Hare S, Neate SM, Dijst G.Dordrecht, The Netherlands: Kluwer Academic Publishers; 1996:147-174.Google Scholar
- Jamaux I, Gelie B, Lamarque C: Early stages of infection of rapeseed petals and leaves by Sclerotinia sclerotiorum revealed by scanning electron microscopy. Plant Pathol. 1995, 44 (1): 22-30. 10.1111/j.1365-3059.1995.tb02712.x.View ArticleGoogle Scholar
- Freeman J, Ward E: Gaeumannomyces graminis, the take-all fungus and its relatives. Mol Plant Path. 2004, 5 (4): 235-252. 10.1111/j.1364-3703.2004.00226.x.View ArticleGoogle Scholar
- Wildermuth GB, Rovira AD: Hyphal density as a measure of suppression of Gaeumannomyces graminis var. tritici on wheat roots. Soil Biol Biochem. 1977, 9 (3): 203-205. 10.1016/0038-0717(77)90076-1.View ArticleGoogle Scholar
- Mesterhazy A: Types and components of resistance to Fusarium head blight of wheat. Plant Breeding. 1995, 114 (5): 377-386. 10.1111/j.1439-0523.1995.tb00816.x.View ArticleGoogle Scholar
- Rudd JC, Horsley RD, McKendry AL, Elias EM: Host plant resistance genes for Fusarium head blight: Sources, mechanisms, and utility in conventional breeding systems. Crop Science. 2001, 41 (3): 620-627. 10.2135/cropsci2001.413620x.View ArticleGoogle Scholar
- Zhou WC, Kolb FL, Bai GH, Domier LL, Yao JB: Effect of individual Sumai 3 chromosomes on resistance to scab spread within spikes and deoxynivalenol accumulation within kernels in wheat. Hereditas. 2002, 137 (2): 81-89. 10.1034/j.1601-5223.2002.01674.x.PubMedView ArticleGoogle Scholar
- Evans CK, Xie W, Dill-Macky R, Mirocha CJ: Biosynthesis of deoxynivalenol in spikelets of barley inoculated with macroconidia of Fusarium graminearum. Plant Dis. 2000, 84 (6): 654-660. 10.1094/PDIS.2000.84.6.654.View ArticleGoogle Scholar
- Voigt C, Schäfer W, Salomon S: A secreted lipase of Fusarium graminearum is a virulence factor required for infection of cereals. Plant J. 2005, 42 (3): 364-375. 10.1111/j.1365-313X.2005.02377.x.PubMedView ArticleGoogle Scholar
- Kachholz T, Demain AL: Nitrate repression of averufin and aflatoxin biosynthesis. J Nat Prod. 1983, 46 (4): 499-506. 10.1021/np50028a013.View ArticleGoogle Scholar
- Keller NP, Nesbitt C, Sarr B, Phillips TD, Burow GB: pH regulation of sterigmatocystin and aflatoxin biosynthesis in Aspergillus spp. Phytopathology. 1997, 87 (6): 643-648. 10.1094/PHYTO.1922.214.171.1243.PubMedView ArticleGoogle Scholar
- Miedaner T, Reinbrecht C, Schilling AG: Association among aggressiveness, fungal colonization, and mycotoxin production of 26 isolates of Fusarium graminearum in winter rye head blight. J Plant Dis Protect. 2000, 107 (2): 124-134.Google Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.