USE OF A CELL EXTRACT FROM ONE OR MORE AMPHIDINIUM MICROALGAE FOR ITS ANTIFUNGI EFFECT ON FUNGI AND / OR OOMYCETES

Description

[0001] The invention relates to the field of antifungal and antibacterial agents for seeds.

[0002] After the Second World War, and in order to address global population growth, the "Green Revolution" was launched, employing modern plant breeding programs, irrigation, fertilizers, and synthetic pesticides to control soil fertility and pathogens. These various elements enabled a near tripling of global food production in about forty years. Today, the challenge for agriculture is to feed 9 billion people by 2050 and to continue increasing production per unit area while taking into account increasingly limited resources and growing constraints. For example, potential losses due to biotic stresses and the lack of crop protection methods could amount to more than half of cereal production.Conventional plant protection products are therefore an integral part of crop protection worldwide in order to limit losses. However, these chemicals have a significant negative impact on human health and the environment, prompting the use of alternative methods to combat infectious diseases, such as biocontrol (the set of methods for protecting plants using natural mechanisms). The purpose of this patent is to exploit unicellular algae, derived from phytoplankton, as a source of new natural molecules capable of acting as a "biological pesticide" by directly affecting the survival of phytopathogens infecting crops of major agronomic importance, such as wheat and grapevines.

[0003] The document Washida et al. “Karatungiols A and B, two novel antimicrobial polyol compounds, from the symbiotic marine dinoflagellate Amphidinium sp”, TETRAHEDRON LETTERS, vol. 47, no. 15, April 10, 2006 describes a purification process for the compounds Karatungiols A and B.

[0004] The document Echigoya et al., HARMFUL ALGAE, vol.4, no.3, February 1, 2005 describes a purification process for amphidinols 2, 4, 9, 10, 11, 12 and 13.

[0005] US 8 815 565B2 releases excerpts d'Amphidianum's cart containing amphidinols 1 to 15.

[0006] The document Genoveffa et al., JOURNAL OF NATURAL PRODUCTS, vol. 77, no. 6, June 27, 2014, describes a purification process for Amphidinol 18. Fusarium wilt

[0007] In Europe, several diseases affect wheat (Summer wheat) are responsible for yield losses or a decline in the sanitary quality of the grains. One of the most important is septoria ( Septoriaspp.). Fusarium wilt is associated with a species complex comprising two genera of phytopathogenic fungi, Fusarium and Microdochium (1). These two genera include approximately 19 species capable of inducing Fusarium wilt of wheat ear. The most common species in Europe are F. graminearum, F. culmorum, F. avenaceum, F. poae, M. nivale and Mr. greater. The genre Fusarium It belongs to the division Ascomycetes and the family Nectriaceae. The genus Microdochium belongs to the Tuberculariaceae family and includes two species, M. nivale and Mr. bigger, causing the same symptoms on ears and leaves as Fusarium. Several species of Fusarium, including Fusarium gramineaeThe most prevalent fungi can be found together at the regional, plot, or even single-ear level, forming the Fusarium complex. The severity, incidence, and prevalence of each species vary according to geographic location, climatic variations, and agricultural practices. The presence of several of these species on the same ear can alter their balance and toxin production dynamics.

[0008] Fusarium head blight of wheat can devastate a crop a few weeks before harvest. It can be associated with significant yield losses (abortion and low grain weight), reduced germination rates, and decreased grain quality due to the presence of toxins. Indeed, fungi of the genus Fusarium, but not of the kind Microdochorium,are capable of producing toxic secondary metabolites, mycotoxins, the presence of which increases the incidence of the disease on agricultural production and constitutes a major economic and public health problem. The main methods of controlling Fusarium head blight include cultural practices, varietal resistance, and chemical control. Currently, few wheat varieties are resistant to Fusarium head blight. However, there are tolerant varieties with partial levels of resistance that limit yield losses and the accumulation of toxins in crops. Once the crop is established, chemical control is possible but of limited effectiveness. The diversity of pathogens and their varying sensitivities to active ingredients complicate this control. For example, fungi of the genus Fusarium are sensitive to triazoles, whereas fungi of the genus Microdochium are sensitive to strobilurins. The septorioses

[0009] Septoria leaf blotch is a disease of wheat responsible for significant yield losses and causing the greatest economic losses worldwide, particularly in humid temperate regions. Two main forms of septoria leaf blotch can be distinguished: Septoria tritici blotch ( Phaeosphere nodules ) and foliar septoria ( Mycosphaerella graminicola In France, septoria leaf spot is mainly found in continental areas, while septoria leaf spot is primarily found in the northwest and along the coast, where the fungus finds favorable climatic conditions for its development. The symptoms caused by M. grass-like plantThe lesions appear successively as chlorosis, light green spots, before evolving into brownish spots called necrosis. These necrotic lesions eventually merge into one another (coalescence). Then, pycnidia, barely visible black fruiting bodies, appear on these necrotic lesions. The damage caused by septoria leaf blotch in terms of losses in photosynthesis, growth, and yield has been studied by several research teams. A qualitative assessment of the damage, expressing the impact of the disease on the protein content of harvested grains, can thus be established.

[0010] M. graminicola is a hemibiotrophic fungus that establishes an initial biotrophic phase where infection occurs on living tissue, followed by a necrotrophic phase during which the fungus expresses toxins that cause the death of colonized tissues. Depending on environmental conditions, the reproduction of M. graminicolaDisease transmission is either sexual (ascospore production) or asexual (pycnidiospore production). Ascospores, dispersed by wind over long distances, play a crucial role in the fungus's survival in the absence of a host plant and are considered the primary source of inoculum for initiating the disease. Pycnidiospores, on the other hand, are mostly produced during the epidemic phase of the disease over several successive infection cycles. These spores are dispersed over short distances by rain splash. The decline in potential yields is all the more significant when the uppermost leaves below the ear, which are involved in grain filling, are severely affected by the disease. Yield losses attributable to Septoria were estimated at 1-2 t.ha -1< on average, with cases reaching up to 3-3.5 t.ha -1<, representing a 40% decrease in yields.

[0011] Control methods M. graminicola are based on the use of fungicides and resistant cultivars. However, recent years have seen a significant loss of fungicide efficacy due to strong selection of pathogens, with, for example, resistance to the strobilurin family, as well as a recent loss of triazole efficacy in the field. Les maladies de la vigne

[0012] Today, grapevines are cultivated worldwide, playing a central role in the economies of many countries. They are consumed as table grapes and juice, but their primary use lies in the wine industry. The European Union is the world's largest wine producer and the largest exporter of wine products. The sector contributes approximately €15 billion annually to the EU economy (www.ceev.be). In 2010, French vineyards covered nearly 865,000 hectares, representing almost 3% of arable land, making France the world's leading wine producer with 51.1 million hectoliters. Grapevines face numerous attacks from pathogens, including fungal diseases. These are called "wood diseases" when they affect the lignified parts of the plant, this is the case in particular with esca, black dead arm or eutypa dieback.The fungi that infect the berries and herbaceous parts of the vine (leaves, stems, etc.) induce "fungal diseases of the foliage" which include grey rot, black rot, downy mildew and powdery mildew. The bait

[0013] While downy mildew, powdery mildew, and botrytis bunch rot are the three main fungal diseases affecting vineyards worldwide, trunk diseases caused by fungal agents are becoming limiting factors in grape production. Winegrowers currently face two major problems with these trunk diseases: a lack of control methods and a profound lack of understanding of the various biotic and abiotic factors involved.

[0014] The most widespread fungal species worldwide that cause esca disease are ascomycetes. Diplodia seriata, Diplodia mutila, Neofusicoccum parvum And Neofusicoccum luteum. In France, the most isolated species are Diplodia seriata And Botryosphaeria dothidea.Numerous other fungi, including some pathogens, are frequently isolated from the wood necrosis of plants infected with esca. This is the case for Eutypa lata,The causative agent of Eutypa dieback. This disease presents in two forms: the slow form and the apoplectic form. Foliar symptoms are characteristic of the slow form, although they can also be present in the apoplectic form. The slow form is characterized by specific leaf discolorations: yellowish interveinal spots on white grape varieties and red-bordered spots on red grape varieties, with the veins remaining green. These spots gradually turn brown and dry out. The foliar symptoms of the slow form may be visible on a vine one year and disappear the following year. The apoplectic form is characterized by the rapid drying out of the aerial parts—shoots, leaves, and clusters—of part or all of the vine. This symptom generally appears during hot summers, leading to the death of the vines in just a few days without any warning signs.The variety of inoculum sources and the very slow, invisible development of fungi in grapevine wood make implementing control methods extremely difficult. Furthermore, evolving European regulations on plant protection products have led to a ban on sodium arsenite-based chemicals due to their carcinogenic effects on humans and their high toxicity to the environment. Extensive research is being conducted worldwide to test new molecules for use in nurseries or vineyards. Gray rot

[0015] Grey mold is a fungal disease caused by an ascomycete fungus called Botrytis cinerea. It belongs to the class of Leotiomycetes, to the order of Helotiales and the family of Sclerotiniaceae. B. cinereais a necrotrophic fungus capable of colonizing healthy, already infected plant tissues, as well as dead tissues (saprophytism). On leaves, symptoms appear as brown spots with a grayish downy growth on the underside (fungus fruiting bodies) that tend to enlarge and cover the entire leaf blade. Grape clusters can be affected before flowering and dry out. They are particularly susceptible at the veraison stage, when white grape varieties develop a brown discoloration and a thick gray downy growth appears. The conidia are dispersed by the wind and penetrate herbaceous organs directly or through wounds. This is why berry splitting due to downy mildew promotes infection by B. cinerea. This disease not only causes yield losses of up to 40% (Viniflhor, 2006 data) but also impairs the organoleptic qualities of the wines. Nevertheless, Botrytis cinerea is also responsible for the "noble rot" necessary to obtain certain sweet wines. Mildew

[0016] The two diseases that currently affect vineyards most severely are downy mildew and powdery mildew. The agent responsible for downy mildew is an oomycete. Plasmospora viticola belonging to the order Peronosporales, it is an obligate parasite; to keep it alive and multiply it, it is obligatory to propagate it on surviving vine leaves. P. viticola It attacks all the herbaceous tissues of the vine as well as the grape clusters. It causes defoliation, browning, and drying of the berries and stems. Without treatment and under favorable climatic conditions, downy mildew can devastate up to 75% of the season's harvest.

[0017] The life cycle of P. viticolaDowny mildew comprises a sexual and an asexual phase. The asexual phase leads to the production of spores necessary for secondary infections and the short-distance dispersal of the pathogen, while the sexual phase produces dormant, cold-resistant oospores that allow overwintering and primary infections. The first macroscopic evidence of downy mildew in a vineyard is the appearance of pale, irregular yellow spots (oil spots) that enlarge on the upper, or adaxial, surface of the leaves. As internal colonization by the mycelium progresses, the development of white, cottony cushions on the underside, corresponding to the oil spots, becomes more prominent. In advanced infections, these symptoms are accompanied by brown dead tissue. Downy mildew control is primarily achieved through preventative measures such as fungicide sprays.While it may be possible to stop an attack, the damage, once caused to the inflorescences and clusters, is irreversible. Powdery mildew

[0018] Powdery mildew of the vine ( Erysiphe killer*Erysiphales* is an obligate biotrophic ascomycete belonging to the order Erysiphales. The fungus colonizes the surface of all green organs of the grapevine, particularly the upper surface of the leaves, and spreads to the berries. A sexual phase, characterized by the production of cleistothecia containing ascospores, may alternate with an asexual phase leading to the formation of conidiophores bearing conidia. During the winter dormancy of the grapevine, the fungus survives as hyphae in dormant buds or as cleistothecia on the plant surface. The spores contained in the cleistothecia are released in the spring to germinate on the surface of buds and young leaves. A primary hypha then develops on the leaf surface, followed by an increasingly complex and branching mycelial network that covers the leaf surface.Subsequently, conidiophores differentiate from the mycelium, constituting the beginning of the sporulation stage, and will colonize other green tissues of the plant, giving rise to secondary infections.

[0019] The presence of mycelium and conidiophores bearing conidia on the surface of infected host tissues gives a powdery, grayish-white appearance. A white, felt-like coating develops on the flower buds, which then dry out. Only young berries with a sugar content of less than 8% are susceptible to powdery mildew. All leaf surfaces can be susceptible to infection, regardless of age. Young infected leaves first turn dark green, then become deformed and stunted. The upper surface of the leaves may show lighter, chlorotic spots resembling the oil spots of downy mildew. Currently, the main means of controlling the diseases that most severely affect vineyards is the use of large quantities of pesticides and fungicides. Therefore, disease pressure is particularly high in viticulture.

[0020] Fungicide treatments, primarily used to combat downy mildew and powdery mildew, are applied according to a precise schedule to prevent damage caused by disease outbreaks. The European Union (EU) uses approximately 68,000 tonnes of fungicides annually to control grapevine diseases, representing 65% of fungicides used in agriculture, while only 3.3% of the EU's usable agricultural land is dedicated to vineyards (Eurostat, 2007). To limit the significant environmental and health impacts of these chemicals, it is necessary to isolate naturally occurring molecules that can protect crops against infectious diseases and ultimately replace the chemical pesticides currently used. The apple scab

[0021] Apple scab, along with brown rot and powdery mildew, is one of the main fungal diseases of apple trees (genus Malus). It is caused by an ascomycete fungus called Unequal vents, of which there are several thousand strains, causing black or brown lesions on the surface of leaves, buds or fruit and sometimes even on the wood. The fruit and the underside of the leaves are especially susceptible.

[0022] The fungus overwinters on the fallen leaves of infected trees, in the form of perithecia. In spring, as the buds burst, the perithecia fill with ascospores. The ascospores are released into the orchard air on humid days and reach the trees via air currents. This release of ascospores begins at bud break and continues for 6 to 10 weeks, most often until the end of June. When the ascospores reach the foliage and the leaves remain wet for a period of time, they germinate and penetrate the leaves: this is the primary infection. Depending on the humidity and temperature conditions, the fungal infection becomes visible within one to three weeks on different parts of the tree. Dark olive or brown spots, about 5 mm in diameter, appear on the leaves and can eventually cover the entire leaf. Infected flowers may drop.Fruit infection is first recognized by grey spots on the stem.

[0023] Following the initial infection, the fungus develops throughout the rest of the summer, producing conidia, which are another form of reproductive structure. When the conidia are released, a secondary infection occurs. Conidia can infect any part of the tree, and those produced in late summer can even develop on stored fruit. Heavy rain disperses the conidia.

[0024] The disease rarely kills its host but can significantly reduce (up to 100%) fruit quality and yield if left untreated with fungicides. After preventative measures such as collecting fallen leaves in the autumn, the control strategy requires effective action in the spring to prevent released spores from infecting or developing on the trees. The traditional method of protection involved beginning fungicide application as soon as bud break and repeating treatments approximately every seven days until the end of June to protect new growth. Apple orchards are the most heavily treated with fungicides and insecticides, with an average of 28.8 fungicide treatments per year, 19 of which are specifically for apple scab (INRA data). Microalgae

[0025] Naturally occurring molecules with novel mechanisms of action, capable of circumventing the resistance developed by pathogens, hold significant potential for the development of new, environmentally friendly plant protection products. The oceans represent a vast array of organisms (bacteria, microalgae, algae, vertebrates, and invertebrates) that are a source of new bioactive molecules, many of which remain largely untapped (2). For example, marine microorganisms accumulate bioactive secondary metabolites with unique structures not found in terrestrial organisms. These metabolites thus represent potential new molecules of interest. Certain substances from marine organisms have been described as possessing antifungal or natural defense activity, but research into these molecules is still in its infancy (3).

[0026] Microalgae are single-celled organisms that play a key role in aquatic ecosystems. By producing organic matter, they play an important ecological role as they form the base of the marine food web. However, their incredible ability to colonize all the world's oceans suggests that they have likely developed effective strategies for combating pathogens, notably through the production of natural pesticides. For example, the abundant proliferation of biotoxin-producing microalgae in coastal regions is responsible for the formation of harmful algal blooms (HABs), which have a significant impact on the food chain.

[0027] Among microalgae, dinoflagellates, belonging to the order Gymnodiniales and the family Gymnodiniaceae, are present in temperate and tropical marine waters, living either free-living or in symbiosis with invertebrates (e.g., corals). Dinoflagellates synthesize a significant number of polyketide secondary metabolites (compounds with potentially toxic biological or pharmacological activity to confer a survival advantage), several of which have been characterized, including those responsible for HAB (4). For example, the model species of dinoflagellates, Amphidinium cartae,Amphidinium produces a profusion of different bioactive compounds, several of which have the potential to be developed as therapeutic agents (5). The polyketides produced by Amphidinium species are extremely diverse in structure and fall into three categories: macrolides, linear polyketides, and long-chain polyketides. For example, amphidinols are polyhydroxypolyenes (long-chain polyketides) that exhibit strong antifungal and hemolytic activity. They increase membrane permeability by associating with membrane lipids (6). Among the different Amphidinium strains, compounds similar to amphidinols with a long polyhydroxy chain have been isolated, such as lingshuiols, karatungiols, carteraol E, luteophanols, colopsinols, and amphezonol A (5).

[0028] To limit the significant impact of chemicals on the environment and human health, it is necessary to isolate naturally occurring molecules that can protect crops against infectious diseases, ultimately replacing the chemical pesticides currently used. These "biological pesticides" could directly affect the survival of plant pathogens in major agricultural crops such as wheat and grapes.

[0029] Surprisingly, the inventors observed a fungicidal effect from a cell extract d'Amphidinium carterae, on many plant pathogenic fungi. SUMMARY OF THE INVENTION

[0030] The object of the invention relates to a method for controlling fungi and / or oomycetes in plants and cultivated seeds, characterized by the following steps: Harvesting fresh cells of one or more microalgae of the genus Amphidinium ;Freezing and / or freeze-drying of said cells; Suspension of said freeze-dried or of said frozen cells in water, in a weight ratio of 1:200 to 1:2 at a temperature above 60°C; Application to cultivated plants and / or seed coating of the extract thus obtained. LEGEND OF THE FIGURES

[0031] Figure 1 The extract of Amphidinium bags possesses antifungal activity on Fusarium graminearum. A. Spores of Fusarium gramineae were incubated in the presence of extracts from different microalgae cultures and then placed on culture medium in vitro. The photo was taken 72 hours later. B. Spores of Fusarium gramineae were incubated in the presence of a range of extract concentrations (from 0 g / L to 2.0 g / L) from a culture d'Amphidinium carterae then placed on culture medium in vitro. The photo was taken 72 hours later. C. Similar to B, but the number of germinated spores was counted 6 hours after incubation. D. Spores of Fusarium gramineaewere incubated in the presence of A. extracts. bags which have been previously frozen ( Figure 1 D (above) or freeze-dried ( Figure 1 D down). Figure 2 The excerpt d'Amphidinium carterae inhibits in vitro And on the plant the growth of pathogenic wheat fungi. A. Procedure for inoculating wheat flowers with Fusarium graminearum spores and then treating them 24 hours later with a solution in the presence or absence (mock) of the extract d'Amphidinium cart. B. The onset and development of symptoms are monitored and the levels of incidence and severity (score from 0 to 9) are noted at 400°J and 450°J. Figure 3 The excerpt d'Amphidinium carterae inhibits in vitro And on the plant the growth of pathogenic fungi of the vine A. The extract d'Amphidinium carterae (1 g / L) or sterile water (mock) were sprayed onto detached vine leaves maintained under in vitro then sporangia of Plasmopara viticola or conidia The killer of Erysiphe were placed on these sheets. The reading of symptoms is carried out at 7 days and at 12 days respectively. B. Similar to A but with mycelial implants of Botrytis cinereawere applied to the treated leaves. The symptoms were assessed after 7 days by measuring the size of the necrotic lesions. C. Mycelial implants of different fungi involved in esca disease of the vine were deposited on a culture medium and then treated 24 hours later with water (mock) or A. extract. bags at different concentrations. The symptoms are read by measuring the surface area of ​​the mycelium at 4 days. DETAILED DESCRIPTION OF THE INVENTION

[0032] The object of the invention relates to a method for controlling fungi and / or oomycetes in plants and cultivated seeds, characterized by the following steps: Harvesting fresh cells of one or more microalgae of the genus Amphidinium ;Freezing and / or freeze-drying of said cells; Suspension of said freeze-dried or of said frozen cells in water, in a weight ratio of 1:200 to 1:2 at a temperature above 60°C; Application to cultivated plants and / or seed coating of the extract thus obtained. Les Amphidinium

[0033] Of the Amphidinium appropriate ones are chosen from the group consisting of Amphidinium achromaticum, Amphidinium aculeatum, Amphidinium acutissimum, Amphidinium acutum, Amphidinium alinii, Amphidinium aloxalocium, Amphidinium amphidinioides, Amphidinium asymmetricum, Amphidinium aureum, Amphidinium belauense, Amphidinium bidentatum, Amphidinium bipes, Amphidinium boekhoutensis, Amphidinium boggayum, Amphidinium caerulescens, Amphidinium carbunculus, Amphidinium carterae, Amphidinium celestinum, Amphidinium chattonii, Amphidinium coeruleum, Amphidinium conradii, Amphidinium conus, Amphidinium coprosum, Amphidinium corallinum, Amphidinium corpulentum, Amphidinium crassum, Amphidinium cristatum, Amphidinium cucurbita, Amphidinium cucurbitella, Amphidinium cupulatisquama, Amphidinium curvatum, Amphidinium cyaneoturbo, Amphidinium dentatum, Amphidinium discoidale, Amphidinium dubium, Amphidinium eilatiensis, Amphidinium emarginatum, Amphidinium fastigium, Amphidinium filum Böhm, Amphidinium flagellans, Amphidinium flexum, Amphidinium galbanum, Amphidinium gibbosum,Amphidinium glaucovirescens, Amphidinium glaucum, Amphidinium globosum, Amphidinium hadai, Amphidinium herdmanii, Amphidinium incoloratum, Amphidinium inflatum, Amphidinium kesselitzii, Amphidinium kesslitzii, Amphidinium klebsii, Amphidinium lacunarum, Amphidinium lanceolatum, Amphidinium lefevrei, Amphidinium lilloense, Amphidinium lissae, Amphidinium longum, Amphidinium luteum, Amphidinium machapungarum, Amphidinium macrocephalum, Amphidinium mammillatum, Amphidinium manannini, Amphidinium mananninii, Amphidinium massartii, Amphidinium mootonorum, Amphidinium mucicola, Amphidinium nasutum, Amphidinium obliquum, Amphidinium obrae, Amphidinium oceanicum, Amphidinium oculatum, Amphidinium operculatum, Amphidinium operculatum var. steinii, Amphidinium ornithocephalum, Amphidinium ovoideum, Amphidinium ovum, Amphidinium pacificum, Amphidinium pelagicum, Amphidinium phthartum, Amphidinium psammophila, Amphidinium psittacus, Amphidinium purpureum, Amphidinium pusillum,Amphidinium rhynchocephalum, Amphidinium roseolum, Amphidinium ruttneri, Amphidinium salinum, Amphidinium schilleri, Amphidinium schroederi, Amphidinium scissum, Amphidinium sphagnicola, Amphidinium sphenoides, Amphidinium steinii, Amphidinium stellatum, Amphidinium stigmatum, Amphidinium sulcatum, Amphidinium tortum, Amphidinium trochodinioides, Amphidinium trochodinoides, Amphidinium trulla, Amphidinium truncatum, Amphidinium turbo, Amphidinium vernal, Amphidinium vigrense, Amphidinium vitreum, Amphidinium vittatum, Amphidinium wigrense, Amphidinium yoorugurrum, Amphidinium yuroogurrum.,

[0034] Preferably, the or one of the microalgae of the genus Amphidinium used according to the invention is Amphidinium carterae. There are several strains d'Amphidinium carterae in collection such as the strains CCMP 124, 1314, 3177 (CCMP = Culture Collection of Marine Phytoplankton), AC 208, 792 (AC = Algobank Cean), BEA 01198 (BEA = Banco Español de Algas).

[0035] Advantageously, the strain d'Amphidinium carterae used according to the invention is CCMP 1314, AC208 or AC792.

[0036] Preferably, said extract comprises amphidinol 18 or amphidinol 19, particularly preferably amphidinol 18, advantageously in an amount greater than 1% w / w relative to the total weight of the extract, preferably between 2 and 10% w / w relative to the total weight of the extract, particularly preferably between 3 and 5% w / w relative to the total weight of the extract. Mode of action

[0037] This fungicidal activity on fungi and / or oomycetes that are pathogenic to plants and cultivated seeds can in particular be exerted by inhibiting spore germination or by inhibiting the growth of the fungus and / or oomycetes.

[0038] The activity is exerted through a lytic activity of the cell walls and membranes which results in cell lysis. Cultivated plants

[0039] These cultivated plants are in particular chosen from the group consisting of cereals such as wheat, corn, barley, rice, soybeans, fruits and vegetables such as potatoes, carrots, apple trees, peach trees, apricot trees, tomatoes, radishes, beans, vines and ornamental plants.

[0040] These cultivated plants are specifically chosen from the group consisting of the genera Abelmoschus, Acacia, Achras, Agave, Agrostis, Aleurites, Allium, Anacardium, Ananas, Annona, Apium, Arachis, Areca, Armoracia, Arracacia, Artocarpus, Asparagus, Aspidosperma, Avena, Bertholletia, Beta, Boehmeria, Borassus, Brassica, Cajanus, Camellia, Cannabis, Capsicum, Carica, Carthamus, Carum, Carya, Castanea, Ceiba, Ceratonia, Chenopodium, Chrysanthemum, Cicer, Cichorium, Cinchona, Cinnamomum, Citrullus, Citrus, Cocos, Coffea, Cola, Colocasia, Corchorus, Corylus, Crotalaria, Cucumis, Cucurbita, Cydonia, Cymbopogon, Cynara, Dactylis, Daucus, Dioscorea, Diospyros, Echinochloa, Elaeis, Elettaria, Eleusine, Eragrostis, Eriobotrya, Eugenia, Fagopyrum, Ficus, Foeniculum, Fragaria, Furcraea, Glycine, Glycyrrhiza, Gossypium, Guizotia, Helianthus, Hevea, Hibiscus, Hordeum, Humulus, Ilex, Indigofera, Ipomoea, Jasminum, Juglans, Lactuca, Lagenaria, Lavandula, Lawsonia, Lens, Lepidium, Lespedeza, Linum, Litchi, Lolium, Lopmoea, Lotus, Lupinus, Lycopersicon, Lygeum, Macadamia, Malus, Mangifera,Manihot, Maranta, Medicago, Mentha, Mespilus, Metroxylon, Moringa, Musa, Myristica, Nicotiana, Olea, Onobrychis, Oryza, Panicum, Papaver, Parsnip, Pelargonium, Pennisetum, Persea, Phaseolus, Phleum, Phoenix, Phormium, Pimpinella, Piper, Pistacia, Pisum, Prunus, Psidium, Punica, Pyrus, Raphanus Rheum, Ribes, Ricinus, Rose, Rubus, Saccharum, Scorzonera, Secale Sechium, Sesamum, Setaria, Solanum, Sorghum, Spinacia, Theobroma, Tragopogon, Trifolium, Trigonella, Triticum, Urena, Vaccinium, Valerianella, Vanilla, Vicia, Vigna, Vitellaria, Vitis, Xanthosoma, Zea, Zingiber., Pathogens

[0041] The aforementioned pathogenic fungi of plants and cultivated seeds are ascomycetes or basidiomycetes, preferably ascomycetes.

[0042] The aforementioned plant and seed pathogens are plant and seed pathogens of the following genera: Acrocalymma, Acrocalymma medicaginis, Fusarium, Fusarium affine, Fusarium arthrosporioides, Fusarium crookwellense, Fusarium culmorum, Fusarium graminearum, Fusarium moniliforme, Fusarium incarnatum, Fusarium solani, Fusarium langsethiae, Fusarium mangiferae, Fusarium oxysporum f.sp. albedinis, Fusarium oxysporum f.sp. asparagi, Fusarium oxysporum f.sp. batatas, Fusarium oxysporum f.sp. betae, Fusarium oxysporum f.sp. cannabis, Fusarium oxysporum f.sp. carthami, Fusarium oxysporum f.sp. cattleyae, Fusarium oxysporum f.sp. ciceris, Fusarium oxysporum f.sp. coffea, Fusarium oxysporum f.sp. cubense, Fusarium oxysporum f.sp. cyclaminis, Fusarium oxysporum f.sp. dianthi, Fusarium oxysporum f.sp. lentis, Fusarium oxysporum f.sp. lini, Fusarium oxysporum f.sp. lycopersici, Fusarium oxysporum f.sp. medicaginis, Fusarium oxysporum f.sp. peas, Fusarium oxysporum f.sp. tomato root, Fusarium oxysporum f.sp.spinach, Fusarium oxysporum, Fusarium pallidoroseum, Fusarium patch, Fusarium proliferatum, Fusarium redolens, Fusarium sacchari, Fusarium solani, Fusarium subglutinans, Fusarium sulphureum, Fusarium tricinctum, Fusarium wilt,. Botrytis Botrytis allii, Botrytis anthophila, Botrytis cinerea, Botrytis fabae, Botrytis narcissicola, Alternaria, Alternaria alternata, Alternaria brassicae, Alternaria brassicicola, Alternaria carthami, Alternaria cinerariae, Alternaria dauci, Alternaria dianthi, Alternaria dianthicola, Alternaria euphorbiicola, Alternaria helianthi, Alternaria helianthicola, Alternaria japonica, Alternaria leucanthemi, Alternaria limicola, Alternaria linicola, Alternaria padwickii, Alternaria panax, Alternaria radicina, Alternaria raphani, Alternaria saponariae, Alternaria senecionis, Alternaria solani, Alternaria tenuissima, Alternaria triticina, Alternaria zinniae, Erisyphus, Erisyphe necator, Erysiphe betae, Erysiphe brunneopunctata, Erysiphe cichoracearum, Erysiphe cruciferarum, Erysiphe graminis f. sp. Avenae, Erysiphe graminis f.sp. tritici, Erysiphe heraclei, Erysiphe pisi, Claviceps Claviceps fusiformis, Claviceps purpurea, Claviceps sorghum, Claviceps zizaniae, Gaeumannomyces, Gaeumannomyces graminis, Leptosphaeria, Leptosphaeria nodorum, Leptosphaeria acuta, Leptosphaeria cannabina, Leptosphaeria coniothyrium, Leptosphaeria libanotis, Leptosphaeria lindquistii, Leptosphaeria maculons, Leptosphaeria musarum, Leptosphaeria pratensis, Leptosphaeria sacchari, Leptosphaeria woroninii,Microdochium, Microdochium spp. Microdochium bolleyi, Microdochium dimerum, Microdochium panattonianum, Microdochium phragmitis, Mycosphaerella, Mycosphaerella arachidis, Mycosphaerella areola, Mycosphaerella berkeleyi, Mycosphaerella bolleana, Mycosphaerella brassicicola, Mycosphaerella caricae, Mycosphaerella caryigena, Mycosphaerella cerasella, Mycosphaerella coffeicola, Mycosphaerella confusa, Mycosphaerella cruenta, Mycosphaerella dendroides, Mycosphaerella eumusae, Mycosphaerella gossypina, Mycosphaerella graminicola, Mycosphaerella henningsii, Mycosphaerella horii, Mycosphaerella juglandis, Mycosphaerella lageniformis, Mycosphaerella linicola, Mycosphaerella louisianae, Mycosphaerella musae, Mycosphaerella musicola, Mycosphaerella palmicola, Mycosphaerella pinodes, Mycosphaerella pistaciarum, Mycosphaerella pistacina, Mycosphaerella platanifolia, Mycosphaerella polymorpha, Mycosphaerella apple, Mycosphaerella punctiformis, Mycosphaerella pyri, Eyespots, Eyespots acuformis, Eyespots yallundae, Flower garden, Blumeria graminis, Pyrenophora, Pyrenophora avenae, Pyrenophora chaetomioides, Pyrenophora graminea, Pyrenophora seminiperda, Pyrenophora teres, Pyrenophora teres f. maculata, Pyrenophora teres f. teres, Pyrenophora tritici-repentis, Ramularia, Ramularia swan-neck, Ramularia beticola, Ramularia coryli, Ramularia cyclaminicola, Ramularia macrospora, Ramularia menthicola, Ramularia necator, Ramularia primulae, Ramularia spinachiae, Ramularia subtilis, Ramularia tenella, Ramularia vallisumbrosae, Rhynchosporium, Rhynchosporium secalis, Snail, Cochliobolus, Cochliobolus carbonum, Cochliobolus cymbopogonis, Cochliobolus hawaiiensis, Cochliobolus heterostrophus, Cochliobolus lunatus, Cochliobolus miyabeanus, Cochliobolus ravenelii, Cochliobolus sativus, Cochliobolus setariae, Cochliobolus spicifer, Cochliobolus stenospilus, Cochliobolus tuberculatus, Cochliobolus victoriae, Microdochium, Microdochium oryzae, Pyricularia, Rice blast, Sarocladium, Sarocladium oryzae, Ustilaginoides, Ustilaginoides virens, Cercospora, Cercospora, Cercospora apii, Cercospora apii f.sp. clerodendrons, Cercospora apiicola, Cercospora peanuts, Cercospora asparagus, Cercospora atrophiliformis, Cercospora beticola, Cercospora brachypus, Cercospora brassicicola, Cercospora brunkii, Cercospora cannabis, Cercospora cantuariensis, Cercospora capsici, Cercospora carotae, Cercospora corylina, Cercospora fuchsiae, Cercospora fusca, Cercospora fusimaculans, Cercospora gerberae, Cercospora halstedii, Cercospora handelii, Cercospora hayi, Cercospora hydrangeae, Cercospora kikuchii, Cercospora lentis, Cercospora liquidambaris, Cercospora longipes, Cercospora longissima, Cercospora mamaonis, Cercospora mangaferae, Cercospora medicaginis, Cercospora melongenae, Cercospora minuta, Cercospora nicotianae, Cercospora odontoglossi, Cercospora papayae, Cercospora penniseti, Cercospora pisa-sativae, Cercospora platanicola, Cercospora puderii, Cercospora pulcherrima, Cercospora rhapidicola, Cercospora rosicola, Cercospora sojina,Cercospora solani, Cercospora solani-tuberosi, Cercospora sorghi, Cercospora theae, Cercospora tuberculans, Cercospora vexans, Cercospora vicosae, Cercospora zeae-maydis, Cercospora zebrina, Cercospora zonata, Corynespora, Corynespora cassicola, Phakospora, Phakospora pachyrhizi, Phakopsora gossypii, Colletotrichum, Colletotrichum acutatum, Colletotrichum arachidis, Colletotrichum capsici, Colletotrichum cereale, Colletotrichum coffeanum, Colletotrichum crassipes, Colletotrichum dematium, Colletotrichum dematium f. spinaciae, Colletotrichum derridis, Colletotrichum destructivum, Colletotrichum gloeosporioides, Colletotrichum glycines, Colletotrichum gossypii, Colletotrichum graminicola, Colletotrichum higginsianum, Colletotrichum kahawae, Colletotrichum lindemuthianum, Colletotrichum lini, Colletotrichum mangenotii, Colletotrichum musae, Colletotrichum nigrum, Colletotrichum orbiculare, Colletotrichum pisi, Colletotrichum sublineolum, Colletotrichum trichellum, Colletotrichum trifolii, Colletotrichum truncatum, Pythium spp., Diplodia, Diplodia allocellula, Diplodia laelio-cattleyae, Diplodia manihoti, Diplodia paraphysaria, Diplodia seriata, Diplodia theae-sinensis, Necklaces, Monilinia azalea, Monilinia fructicola, Monilinia fructigena, Monilinia laxa, Monilinia oxycocci, Little piece, Pezzicula alba, Pezzicula malicorticis, Zymoseptoria, Zymoseptoria of wheat Phytophthora, Phytophthora infestans Guignard, Guignardia bidwelli, Guignardia camelliae, Guignardia fulvida, Guignardia mangiferae, Guignardia musae, Guignardia philoprina, Plasmopara, Plasmopara viticola, Puccinia, Puccinia angustata, Puccinia arachidis, Puccinia aristidae, Puccinia asparagi, Puccinia cacabata, Puccinia campanulae, Puccinia carthami, Puccinia coronata, Puccinia dioicae, Puccinia erianthi, Puccinia extensicola, Puccinia helianthi, Puccinia hordei, Puccinia jaceae, Puccinia kuehnii, Puccinia malvacearum, Puccinia mariae-wilsoniae, Puccinia melanocephala, Puccinia menthae, Puccinia oxalidis, Puccinia pelargonii-zonalis, Puccinia pittieriana, Puccinia poarum, Puccinia purpurea, Puccinia recondita, Puccinia schedonnardii, Puccinia sessilis, Puccinia striiformis, Puccinia striiformis, Puccinia subnitens, Puccinia substriata, Puccinia verruca, Puccinia xanthii, Rhizoctonia, Rhizoctonia solani, Rhizoctonia oryzae, Rhizoctonia cerealis, Rhizoctonia leguminicola, Rhizoctonia rubi, Sclerotinia, Sclerotinia borealis, Sclerotinia bulborum, Sclerotinia minor, Sclerotinia rici, Sclerotinia sclerotiorum, Sclerotinia spermophila, Sclerotinia trifoliorum, Septoria, Septoria ampelina, Septoria azaleae, Septoria bataticola, Septoria campanulae, Septoria cannabis, Septoria cucurbitacearum, Septoria darrowii, Septoria dianthi, Septoria eumusae, Septoria glycines, Septoria helianthi, Septoria humuli, Septoria hydrangeae, Septoria lactucae, Septoria lycopersici, Septoria lycopersici, Septoria menthae, Septoria passerinii, Septoria pisi, Septoria rhododendri, Septoria secalis, Septoria selenophomoides, Venturia, Venturia inequalis. Venturia carpophila, Acrodontium, Acrodontia simplex, Acrophialophora, Acrophialophora fusispora, Acrosporium, Acrosporium tingitanum, Aecidium, Aecidium aechmantherae, Aecidium amaryllidis, Aecidium breyniae, Aecidium campanulastri, Aecidium cannabis, Aecidium cantensis, Aecidium caspicum, Aecidium phoeniculi, Aecidium narcissi, Ahmadiago, Albonectria, Albonectria rigidiuscula, Allodus, Podophyllum allodus, Amphobotrys, Amphobotrys ticks, Anguillosporella, Anguillosporella vermiformis, Anthostomella, Anthostomella shootulans, Antrodia, Antrodia albida, Antrodia serialiformis, Antrodia serialis, Apiospora, Apiospora montagnei, Appendix, Armillaria Armillaria heimii, Armillaria sinapina, Armillaria socialis, Armillaria tabescens,Arthrocladiella, Arthuriomyces, Arthuriomyces peckianus, Ascochyta, Ascochyta asparagina, Ascochyta bohemica, Ascochyta caricae, Ascochyta doronici, Ascochyta fabae f.sp. lentis, Ascochyta graminea, Ascochyta hordei, Ascochyta humuli, Ascochyta pisi, Ascochyta prasadii, Ascochyta sorghum, Ascochyta spinaciae, Ascochyta tarda, Ascochyta tritici, Ascospora, Ascospora rubrum, Aspergillus, Aspergillus aculeatus, Aspergillus fischerianus, Aspergillus niger, Asperisporium, Asperisporium caricae, Asteridiella, Asteroma, Asteroma caryae, Athelia, Athelia arachnoidea, Athelia rolfsii, Aurantiporus, Aurantiporus fissilis, Aureobasidium, Aureobasidium sprouting, Bambusiomyces, Banana freckle, Bayoud disease, Beniowskia, Beniowskia sphaeroidea, Bionectria, Bionectria ochroleuca, Bipolaris, Bipolaris cactivera, Bipolaris cookei, Bipolaris incurvata, Bipolaris sacchari, Biscogniauxia, Biscogniauxia capnodes, Biscogniauxia marginata, Bjerkandera, Burnt birch, Block sigatoka, Blakeslea, Blakeslea trispora, Botryodiplodia, Botryodiplodia oncidii, Botryodiplodia ulmicola, Botryosphaeria, Botryosphaeria cocogena, Botryosphaeria dothidea, Botryosphaeria marconii, Botryosphaeria obtusa, Botryosphaeria rhodina, Botryosphaeria ribis, Botryosphaeria stevensii, Botryosporium, Botryosporium pulchrum, Botryotinia, Botryotinia fuckeliana, Botryotinia polyblastis, Boxwood blight, Brachybasidiaceae, Brasiliomyces, Brasiliomyces malachrae, Briosia, Briosia ampelophaga, Brown ring patch, Buckeye rot of tomato, Bulbomicrosphaera, Cadophora, The apple tree, Turf, Calonectria, Calonectria ilicicola, Calonectria indusiata, Calonectria kyotensis, Calonectria pyrochroa, Calonectria quinqueseptata, Camarotella, Camarotella acrocomiae, Camarotella costaricensis, Cane rust, Capitorostrum, Coconut palm, Capnodium, Capnodium footii, Capnodium mangiferum, Capnodium ramosum, Capnodium theae, Cephalosporium, Cephalosporium gramineum, Ceratobasidium, Ceratobasidium cereale, Ceratobasidium cornigerum, Ceratobasidium noxium, Ceratobasidium ramicola, Ceratobasidium setariae, Ceratobasidium stevensii, Ceratocystis, Ceratocystis adiposa, Ceratocystis coerulescens, Ceratocystis fimbriata, Ceratocystis moniliformis, Ceratocystis oblonga, Ceratocystis obpyriformis, Ceratocystis paradoxa, Ceratocystis pilifera, Ceratocystis pluriannulata, Ceratocystis polyconidia, Ceratocystis tanganyicensis, Ceratocystis zombamontana, Ceratorhiza, Ceratorhiza hydrophila, Ceratospermopsis, Cercoseptorium, Cercoseptoria ocellata, Cercosporella, Cercosporella rubi, Cereporia, Ceriporia spissa, Ceriporia xylostromatoides, Cerrena, Cerrena unicolor, Ceuthospora, Ceuthospora lauri, Choanephora, Choanephora cucurbitarum, Choanephora infundibulifera, Chrysanthemum, Chrysanthemum white rust, Chrysomyxa, Chrysomyxa cassandrae, Chrysomyxa, Chrysomyxa himalensis, Chrysomyxa ledi, Chrysomyxa ledi var. rhododendri, Chrysomyxa ledicola, Chrysomyxa nagodhii, Chrysomyxa neoglandulosi, Chrysomyxa piperiana, Chrysomyxa pyrolata, Chrysomyxa pyrolae, Chrysomyxa reticulata, Chrysomyxa roanensis, Chrysomyxa succinea, Cladosporium, Cladosporium arthropodii, Cladosporium cladosporioides, Cladosporium cladosporioides f.sp. pisicola, Cladosporium cucumerinum, Cladosporium herbarum, Cladosporium musae, Cladosporium oncobae, Climacodon, Climacodon pulcherrimus, Climacodon septentrionalis, Clitocybe, Clitocybe parasitica, Clonostachys rosea f. rosea, Clypeoporthe, Clypeoporthe iliau, Coleosporium, Coleosporium helianthi, Coleosporium ipomoeae, Coleosporium madiae, Coleosporium pacificum, Coleosporium tussilaginis, Conidiosporomyces, Rabbit, Coniella castaneicola, Coniella diplodiella, Coniella fragariae, Coniothecium, Coniothecium chomatosporum, Coniothyrium, Coniothyrium celtidis-australis, Coniothyrium henriquesii, Coniothyrium rosarum, Coniothyrium wernsdorffiae, Coprinopsis, Coprinopsis psychromorbida, Cordana, Cordana johnstonii, Cordana musae, Coriolopsis floccosa, Corn grey leaf spot, Bark, Corticium invisum, Corticium penicillatum, Corticium theae, Coryneopsis, Coryneopsis rubi, Coryneum, Rhododendron coryneum, Covered smut, Crinipelli, Crinipellis sarmentosa, Cronartium, Cronartium ribicola, Cryphonectriaceae, Cryptobasidiaceae, Cryptocline, Cryptocline cyclamen, Cryptomelia, Cryptosporella, Cryptosporella umbrina, Cryptosporiopsis, Cryptosporiopsis tarraconensis Cryptosporidium, Cryptosporium minimal, Curved, Curvularia lunata, Curvularia caricae-papayae, Curvularia penniseti, Curvularia senegalensis, Curvularia trifolii, Cyclaneusma needle cast, Cylindrocarpon, Cylindrocarpon ianthothele var. ianthothele, Cylindrocarpon magnusianum, Cylindrocarpon musae, Cylindrocladiella, Cylindrocladiella camelliae, Cylindrocladiella parva, Cylindrocladium, Cylindrocladium clavatum, Cylindrocladium lanceolatum, Cylindrocladium peruvianum, Cylindrocladium pteridis,Cylindrosporium, Cylindrosporium cannabinum, Cylindrosporium juglandis, Cylindrosporium rubi, Cymadotea, Cymadothea trifolii, Cytospora, Cytospora palmarum, Cytospora personata, Cytospora sacchari, Cytospora sacculus, Cytospora terebinthi, Cytosporin, Cytosporina ludibunda, Dactuliophora, Dactuliophora elongata, Davidella, Davidiella dianthi, Davidiella tassiana, Deightoniella, Deightoniella papuana, Deightoniella torulosa, Dendrophora, Dendrophora marconii, Dendrophora erumpens, Denticular, Mangosteen, The skin of the pseudotsuga, Diaporthaceae, Diaporthe, Diaporthe arctii, Diaporthe dulcamarae, Diaporthe eres, Diaporthe helianthi, Diaporthe lagunensis, Diaporthe lokyae, Diaporthe melonis, Diaporthe orthoceras, Diaporthe perniciosa, Diaporthe phaseolorum, Diaporthe phaseolorum var. caulivora, Diaporthe phaseolorum var. phaseolorum, Diaporthe phaseolorum var. soybean, Diaporthe rudis , Diaporthe tanakae , Diaporthe toxica , Dicarpella, Dicarpella dryina, Didymella, Didymella applanata, Didymella bryoniae, Didymella fabae, Didymella lycopersici Didymosphaeria, Didymosphaeria arachidicola, Didymosphaeria taiwanensis, Dilophospora, Dilophospora alopecuri, Dimeriella, Dimeriella sacchari, Diplocarpon, Diplocarpon mespili, Diplocarpon rosae, Discord, Discosia artocreas, Discostroma, Cortical discostroma, Distocercospora, Distocercospora livistonae, Dothiorella, Dothiorella brevicollis, Dothiorella dominicana, Dothiorella dulcispinae, Dothiorella gregaria, Drechsler, Drechslera avenacea, Drechslera campanulata, Drechslera dematioidea, Drechslera gigantea, Drechslera glycines, Drechslera musae-sapientium, Drechslera teres f. maculata, Drechslera wirreganensis, Eballistra, Eballistra lineata, Eballistra oryzae, Eballistraceae, Echinodont, Echinodontium ryvardenii, Echinodontium tinctorium, The ectendomeliola, Elsinore, Elsinoë ampelina, Elsinoë batatas, Elsinoë brasiliensis, Elsinoë leucospila, Elsinoë randii, Elsinoë rosarum, Elsinoë sacchari, Elsinoë theae, Elsinoë veneta, Endomeliola, Endothia, Radical endothelium, Endothiella, Endothiella gyrosa, Entorrhizomycetes, Entyloma, Entyloma ageratinae, Entyloma dahliae, Entyloma ellisii, Epicoccum, Black Epicoccum, Hermitage, Eremothecium coryli, Eremothecium gossypii, Erysiphales, Exobasidiaceae, Exobasidium burtii, Exobasidium reticulatum, Exobasidium vaccinii var. japonicum, Exobasidium vaccinii-uliginosi, Exobasidium vexans,xxophiala alcalophila, Exophiala, Exophiala angulospora, Exophiala attenuata, Exophiala calicoides, Exophiala castellanii, Exophiala dermatitidis, Exophiala dopicola, Exophiala exophialae, Exophiala heteromorpha, Exophiala hongkongensis, Exophiala jeanselmei, Exophiala lecanii-corni, Exophiala mansonii, Exophiala mesophila, Exophiala necklaces, Exophiala negronii, Exophiala phaeomuriformis, Exophiala pisciphila, Exophiala psychrophila, Exophiala salmonis, Exophiala spinifera, Fomes, Fomes of Lamaens, Fomitopsis, Fomitopsis rosea, Sword Fusicladium pisicola,Fusicoccum, Aesculus fusicocum, almond fusicocum, oak fusicocum, Galactomyces, Galactomyces candidum, Ganoderma, Ganoderma brownii, Ganoderma lobatum, Ganoderma megaloma, Ganoderma meredithiae, Ganoderma orbiforme, Ganoderma philippii, Ganoderma sessile, Ganoderma tornatum, Ganoderma zonatum, Geastrumia, Geastrumia polystigmatis, Georgefischeriaceae, Georgefisheriales, Geosmithia, Geosmithia pallida, Geotrichum, Geotrichum candidum, Geotrichum klebahnii, Gibberella, Gibberella acuminate, Gibberella avenacea, Gibberella baccata, Gibberella cyanogena, Gibberella fujikuroi, Gibberella intricans, Gibberella pulicaris, Gibberella stilboides, Gibberella tricincta, Gibberella xylarioides, Gibberella zeae, Gibellina, Cereal gibellina, Gilbertella, Gilbertella persicaria, Gjaerumiaceae, Gliocladiopsis, Gliocladiopsis tenuis, Gliocladium, Gliocladium vermoeseni, Gloeocercospora, Gloeocercospora sorghi, Gloeocystidiellum, Gloeocystidiellum porosum, Gloeophyllum, Gloeophyllum mexicanum, Gloeophyllum trabeum, Gloeoporus, Gloeoporus dichrous, Gloeosporium, Gloeosporium cattleyae, Gloeosporium tea-sinensis, Glomerella, Glomerella cingulata, Glomerella graminicola, Glomerella tucumanensis, Gnomonia, Gnomonia caryae, Gnomonia combari, Gnomonia dispora, Gnomonia iliau, Gnomonia bush, Golovinomyces, Golovinomyces cichoracearum, Phoenician palm, Graphiolaceae, Graphium, Graphium rigidum, Graphium redum, Graphyllium, Graphyllium pentamerum, Grovesinia, Grovesinia pyramidalis, Gymnoconia, Gymnoconia nitens, Gymnopus, Gymnopus dryophilus, Gymnosporangium, Gymnosporangium kernianum, Gymnosporangium libocedri, Gymnosporangium nelsonii, Gymnosporangium yamadae, Haematonectria, Haematonectria haematococco, Hansenula, Hansenula subpelliculosa, Hapalosphaeria, Hapalosphaeria deformans, Haplobasidion, Haplobasidion of the Muses, Helicobasidium, Helicobasidium compactum, Helicobasidium longisporum, Helicobasidium purpureum, Helicoma, Helicoma muelleri, Helminthosporium, Helminthosporium cookei, Helminthosporium solani, Hendersonia, Hendersonia creberrima, Hendersonia theicola, Hericium, Hericium coralloides,Heterobasidion, Heterobasidion irregulare, Heterobasidion occidentale, Hexagons, Hexagonia hydnoides, Hymenula, Hymenula related, Hyphoderma, Corrugated hyphoderma, Hyphodontia, Hyphodontia aspera, Hyphodontia sambuci, Hypoxylon, Hypoxylon tinctor, Unknown, Inonotus arizonicus, Inonotus cuticularis, Inonotus dryophilus, Inonotus hispidus, Inonotus ludovicianus, Worm, Destructive weevil, milk weevil, Kabatiella, Kabatiella caulivora, Karnal is full, Koa wilt, Kretzschmaria, Kretzschmaria zonata, Kuehneola, Kuehneola uredinis, Kutilakesa, Kutilakesa pironii, Happy, Laetiporus ailaoshanensis, Laetiporus baudonii, Laetiporus caribensis, Laetiporus conifericola, Laetiporus cremeiporus, Laetiporus gilbertsonii, Laetiporus huroniensis, Laetiporus montanus, Laetiporus portentosus, Laetiporus zonatus, Loose text, Two-color loose-weave fabric, Leandria, Leandria momordicae, Lentinus, Tiger lentil, Lenzites, Lenzites betulina, Lenzites elegans, Leohumicola, Leohumicola black, Leohumicola encrusted, Leohumicola very light, Leptodontidium, Leptodontidium elatius, Leptograph, Leptographium microsporum, Leptosphaerulina, Leptosphaerulina crassiasca, Leptosphaerulina trifolii, Leptothyrium, Leptothyrium nervisedum, Leptotrochila, Leptotrochila medicaginis, Leucocytospora, Leucocytospora leucostoma, Leucostoma, Leucostoma auerswaldii, Leucostoma canker, Leucostoma kunzei, Leucostoma persoonii, Leveillula, Leveillula compositum, Leveillula leguminosarum, Leveillula tourica, Slug, A thin snail, Linochora, Linochora grass, Loose smut, Lopharia, Lopharia crassa, Lophodermium, Lophodermium aucupariae, Lophodermium schweinitzii, Macrophoma, Macrophoma mangiferae, Macrophoma theicola, Macrosporium, Macrosporium cocci, Magnaporthe, Magnaporthe grisea, Magnaporthe salvinii, Magnaporthiopsis, Mamianiella, Mamianiella coryli, Marasmiellus, Marasmiellus cocophilus, Marasmiellus stenophyllus, Marasmius, Horse-hairy Marasmius, Sugar-sweet Marasmius, Semi-striped Marasmius, Stenophyllous Marasmius, Thin-lipped Marasmius, Massarina, Massarina walkeri, Mauginiella, Mauginiella scaettae, Melampsora, Melampsora lini, Melampsora occidentalis, Melancholy, Carthusian Melancon, Melanconium, Walnut Melanconium, Meliola, Meliola mangiferae, Meliola zangii, Meruliopsis, Meruliopsis ambigua, Microascus, Microascus brevicaulis, Microbotryum, Microbotryum silenes-dioicae, Microbotryum violaceum, Microsphaera, Microsphaera coryli, Microsphaera diffusa, Microsphaera ellisii, Microsphaera euphorbiae, Microsphaera hommae, Microsphaera penicillata, Microsphaera vaccinii, Microsphaera verruculosa, Microstroma, Microstroma walnut, Moesziomyces, Moesziomyces bullatus, Moniliophthora, Moniliophthora rot, Monilochaetes, Monilochaetes infuscans, Monochaetia, Monochaetia corylus, Monochaetia mali, Monographella, Monographella albescens, Monographella cucumerina, Monographella nivalis, Monosporascus, Monosporascus cannonballus, Monosporascus eutypoides, Monostichella, Monostichella coryli, Mucor, Mucor circinelloides, Mucor winter, Mucor mucedo, Mucor paronychius, Mucor piriformis, Mucor racemosus, Mycenae, Mycena citricolor, Mycocentrospora, Mycocentrospora acerina, Mycoleptodiscus, Mycoleptodiscus terrestris, Didymella, The rabies of the rabid, Mycosphaerella, Mycosphaerella recutita, Mycosphaerella rosicola, Mycosphaerella rubi, Mycosphaerella stigma-platani, Mycosphaerella striatiformans, Mycovellosiella, Mycovellosiella concors, Passalore, Yellow passerine, Mycovellosiella, Mycovellosiella koepkei, Mycovellosiella vaginae, Myriogenospora, Myriogenospora aciculispora, Myrothecium, Myrothecium roridum, Myrothecium verrucaria, Naevala, Very small seagull, Naohidemyces, Naohidemyces vaccinii, Nectria, Nectria cinnabarina, Nectria ditissima, Nectria foliicola, Nectria mammoidea, Nectria mauritiicola, Nectria peziza, Nectria pseudotrichia, Nectria radicicola, Nectria ramulariae, Nectriella, Nectriella pironii, Nemania, Nemania diffusa, Nemania serpentina, Neocosmospora, Neocosmospora vasinfecta, Neodeightonia, Neodeightonia phoenicum, Neoerysiphe, Neoerysiphe galeopsis,Neofabraea, Neofabraea perennans, Neofusicoccus, Neofusicoccum mangiferae, Oedipus, Oidiopsis gossypii, Oedema, Groundnut powdery mildew, Carica-papaya powdery mildew, Indic powdery mildew, Mango powdery mildew, Manihotis powdery mildew, Olpidium, Brassica oleracea, Omphalia, The transparent navel, Ophiobolus, Ophiobolus eguillides, Ophiobolus cannabinus, Ophioirina, Ovulinia, Azalea ovules, Oxyporus, Oxyporus corticola, Ozone, Texas ozone, Peltaster, Peltaster fructicola, Penicillium, Penicillium expansum, Penicillium funiculosum, Peniophora, Periconia, Periconia circinata, Periconiella, Periconiella cocos, Periderm, Peridermium californicum, Pestalosphere, Pestalosphaeria concentrica, Pestalozzi, Pestalotia longiseta, Pestalotia rhododendri, Pestalotiopsis, Pestalotiopsis adusta, Pestalotiopsis arachidis, Pestalotiopsis disseminata, Pestalotiopsis guepini, Pestalotiopsis leprogena, Pestalotiopsis longiseta, Pestalotiopsis mangiferae, Pestalotiopsis palmarum, Pestalotiopsis sydowiana, Pestalotiopsis theae, Peyronella, Peyronellaea curtisii, Phacidiopycnis, Phacidiopycnis padwickii, Phaeochoropsis, Phaeochoropsis mucosa, Phaeocytostroma, Phaeocytostroma iliau, Phaeocytostroma sacchari, Phaeoisariopsis, Phaeoisariopsis bataticola, Phaeorumularia, Phaeoramularia heterospora, Phaeoramularia indica, Phaeoramularia manihotis, Phaeoseptoria, Phaeoseptoria musae, Phaeosphaerella, Phaeosphaerella mangiferae, Phaeosphaerella teae, Phaeosphere, Phaeosphaeria avenaria, Phaeosphaeria herpotrichoides, Phaeosphaeria microscopica, Phaeosphaeria nodorum, Phaeosphaeriopsis, Phaeosphaeriopsis obtusispora, Phaeotrichoconis, Phaeotrichoconis crotalariae, Phylophora, Phialophora asteris, Phialophora cinerescens, Phialophora gregata, Phialophora tracheiphila, Phoma, Phoma clematidina, Phoma costaricensis, Phoma cucurbitacearum, Phoma destructiva, Phoma draconis, Phoma exigua, Phoma exigua, Phoma exigua var. foveata, Phoma exigua, Phoma glomerata, Phoma glycinicola, Phoma herbarum, Phoma insidiosa, Phoma medicaginis, Phoma microspora, Phoma narcissi, Phoma nebulosa, Phoma oncidii-sphacelati, Phoma pinodella, Phoma sclerotioides, Phoma strasseri, Phomopsis, Phomopsis asparagi, Phomopsis asparagicola, Phomopsis cannabina, Phomopsis coffeae, Phomopsis ganjae, Phomopsis javanica, Phomopsis longicolla, Phomopsis mangiferae, Phomopsis prunorum, Phomopsis sclerotioides, Phomopsis theae, Phragmidium, Phragmidium mucronatum, Phragmidium rosae-pimpinellifoliae, Phragmidium rubiidaei, Phragmidium violaceum, Phyllachora, Phyllachora banksiae, Phyllachora cannabis, Phyllachora graminis, Phyllachora gratissima, Phyllachora musicola, Phyllachora pomigena, Phyllachora sacchari, Phyllactinia, Phyllosticta, Phyllosticta alliariaefoliae Phyllosticta arachidis-hypogaeae, Phyllosticta batatas, Phyllosticta capitalensis, Phyllosticta carpogena, Phyllosticta coffeicola, Phyllosticta concentrica, Phyllosticta coryli, Phyllosticta cucurbitacearum, Phyllosticta cyclaminella, Phyllosticta erratica, Phyllosticta hawaiiensis, Phyllosticta lentisci, Phyllosticta manihotis, Phyllosticta micropuncta, Phyllosticta mortonii, Phyllosticta nicotianae, Phyllosticta palmetto, Phyllosticta penicillariae, Phyllosticta perseae, Phyllosticta pseudocapsici, Phyllosticta sojaecola, Phyllosticta theae, Phyllosticta theicola,Phymatotrichopsis, Phymatotrichopsis omnivora, Physalospora, Physalospora disrupta, Physalospora persea, Physoderma, Physoderma alfalfa, Physoderma leproides, Physoderma trifolii, Physopella, Physopella ampelopsis, Pileolaria, Pileolaria terebinthi, Piricaudiopsis, Piricaudiopsis punicae, Piricaudiopsis rhaphidophorae, Piricaudiopsis rosae, Plenum, Plenodomus destructus, Plenodomus meliloti, Pleosphaerulina, Pleosphaerulina sojicola, Pleospora, Pleospora alfalfa, Pleospora beta, Pleospora herbarum, Pleospora lycopersici, Pleospora tarda, Pleospora theae, Pleuroceras, Podosphaera, Podosphaera fuliginea, Podosphaera fusca, Podosphaera leucotricha, Podosphaera macularis, Podosphaera pannosa, Polyscythalum, Polyscytalum pustulans, Poria, Poria hypobrownea, Post office, Postia tephroleuca, Powdery mildew, Pseudocercospora, Pseudocercospora arecacearum, Pseudocercospora cannabina, Pseudocercospora fuligena, Pseudocercosporella herpotrichoides, Pseudocercosporella gunnerae, Pseudocercospora pandoreae, Pseudocercospora puderi, Pseudocercospora rhapisicola, Pseudocercospora theae, Pseudocercospora vine, Pseudocercosporella capsellae, Pseudocochliobolus, Pseudocochliobolus eragrostidis Pseudoepicoccus, Pseudoepicoccus cocci, Pseudopeziza, Pseudopeziza jonesii, Pseudopeziza medicaginis, Pseudopeziza trifolii, Pseudoseptoria, Pseudoseptoria donacis, Pucciniaceae, Pucciniastrum, Pucciniastrum americanum, Pucciniastrum arcticum, Pucciniastrum epilobii, Pucciniastrum hydrangeae, Pycnostysanus, Pycnostysanus azaleae, Pyrenochaeta, Pyrenochaeta licopersici, Pyrenochaeta terrestris, Pyrenopeziza, Pyrenopeziza brassicae, Copper chloride, Ramichloridium musae, Ramulispora, Ramulispora sorghi, Ramulispora sorghicola, Rhinocladium, Rhinocladium corticola, Rhizophydium, Rhizophydium graminis, Rhizopus, Rhizopus arrhizus, Rhizopus circinans, Rhizopus microsporus, Rhizopus oryzae, Rhythm, Rhytisma punctatum, Rhytisma vitis, Rigid, Rigidoporus bound, Rosellinia, Rosellinia arcuata, Rosellinia bunodes, Rosellinia necatrix, Rosellinia pepo, Sugarcane, Saccharicola taiwanensis, Schiffnerula, Schiffnerula cannabis, Schizophyllum, Schizophyllum commune, Schizophora, Schizopora flavipora, Schizothyrium, Schizothyrium apple, Sclerophthora, Sclerophthora macrospora, Sclerotium, Sclerotium cinnamon, Sclerotium delphinii, Scytinostroma, Scytinostroma galactinum, Seimatosporium, Seimatosporium mariae, Seimatosporium rhododendri, Selenophoma, Selenophoma linicola, Septobasidium, Septobasidium bogoriense, Septobasidium euryae-groffii, Septobasidium gaoligongense, Septobasidium pilosum, Septobasidium polygoni, Septobasidium pseudopedicellatum, Septobasidium theae, Septocytes, Septocytes of red blood cells, Serpula, Serpula lacrymans, Setosphere, Setosphaeria rostrata, Setosphaeria turcica, Spencermartinsia, spencermartinsia pretoriaensis Sphaceloma, Sphaceloma arachidis, Sphaceloma menthae, Sphaceloma perseae, Sphaceloma poinsettiae, Sphaceloma sacchari, Sphaceloma theae, Sphacelotheca, Sphacelotheca reiliana, Sphaerotheca castagnei, Sphaerulina, Sphaerulina oryzina, Sphaerulina rehmiana, Sphaerulina rubi, Sphenospora, Sphenospora kevorkianii, Spilocaea, Spilocaea oleaginosa, Sporisorium, Sporisorium cruentum, Sporisorium ehrenbergii, Sporisorium scitamineum, Sporisorium sorghi, Sporonema, Sporonema phacidioides, Stagonospora, Stagonospora avenae, Stagonospora meliloti, Stagonospora recedens, Stagonospora sacchari, Stagonospora tainanensis, Stagonosporopsis, Stegocintractia, Stegocintractia reeds, Stemphylium, Stemphylium alfalfa, Stemphylium bolicii, Stemphylium cannabinum, Stemphylium globuliferum, Stemphylium licopersici, Stemphylium parciforme, Stemphylium solani, Stemphylium vesicarium, Stenella, Stenella anthuriicola, Stigmatomycosis, Stigmas, Stigmina carpophila, Stigmina palmivora, Stigmina plani-racemosae, Stromatinia, Stromatinia cepivora, Sydowella, Sydowiella depressula, Sydowiellaceae, Synchytrium, Synchytrium endobioticum, Tapestry, Tapesia acuformis, Tapesia yallundae, Taphrina, Taphrina coryli, Taphrina potentillae, Thanatephorus, Cucumber beetle, Thecaphora, Thecaphora solani, Thielaviopsis, Thielaviopsis basicola, Thielaviopsis ceramica, Thyrostoma, Thyrostoma compactum, Tiarosporella, Tiarosporella urbis-rosarum, Tilletia, Tilletia barclayana, Tilletia caries, Tilletia controversa, Tilletia laevis, Tilletia tritici, Tilletia walkeri, Tilletiariaceae, Togniniaceae, Tranzschelia, Tranzschelia pruni-spinosae,Trichoderma Trichoderma koningii, Trichoderma paucisporum, Trichoderma songyi, Trichoderma theobromicola, Trichoderma viride, Tubercularia, Laterite tubercles, Tunstallia, Tunstallia aculeata, Typhula, Typhula blight, Typhula idahoensis, Typhula incarnata, Typhula ishikariensis, Typhula variabilis, Ulocladium, Ulocladium consortiale, Hook, Uredo, Uredo behnickiana, Uredo kriegeriana, Uredo musae, Uredo nigropuncta, Uredo rangelii, Urocystis, Urocystis agropyri, Urocystis brassicae, Urocystis occulta, Uromyces, Uromyces apiosporus, Uromyces appendiculatus, Uromyces beticola, Uromyces cicerisarietini, Uromyces dianthi, Uromyces euphorbiae, Uromyces graminis, Uromyces inconspicuus, Uromyces lineolatus, Uromyces musae, Uromyces oblongus, Uromyces pisi-sativi, Uromyces proëminens, Uromyces medicaginis, Uromyces trifolii-repentis, Uromyces viciae-fabae, Urophlyctis, Urophlyctis leproides, Urophlyctis trifolii, Ustilaginales, Ustilago, Oat rust, Oat rust, Barley rust, Oat rust, Black rust, Oat rust, Scitamine rust, Wheat rust, Vankya, Vankya ornithogalum, Velvet blight, Veronaea, Verona, the muses, Verticillium, Verticillium albo-atrum, Verticillium alfalfae, Verticillium dahliae, Verticillium isaacii, Verticillium klebahnii, Verticillium longisporum, Verticillium nonalfalfae, Verticillium theobromae, Verticillium wilt, Verticillium zaregamsianum, Waitea, Waitea circina, West, Wheat leaf rust, Wheat mildew, Wuestneiopsis, Wuestneiopsis georgiana, Xeromphalina, Xeromphalina fraxinophila, Zopfia, Zopfia rhizophila, Zygosaccharomyces Zygosaccharomyces bailii, Zygosaccharomyces florentinus, Zythiostroma.

[0043] Preferably, the fungal, oomycete or bacterial vs. culture plant pairs targeted by the invention are the following: Blé (Wheat) Claviceps purpurea, Erysiphe graminis, Fusarium avenaceum, Fusarium culmorum, Fusarium graminearum, Fusarium langsethiae, Fusarium poae, Fusarium pseudograminearum, Gaeumannomyces graminis, Leptosphaeria nodorum, Microdochium spp., Mycosphaerella graminicola, Oculimacula acuformis, Oculimacula yallundae, Puccinia recondita, Puccinia striiformis, Pyrenophora tritici-repentis, Rhizoctonia cerealis, Microdochium And Zymoseptoria of wheat More ( Corn ) Fusarium graminearum, Fusarium proliferatum, Fusarium subglutinans, Fusarium verticillioides Barley (Barley) Blumeria graminis, Fusarium spp, Pyrenophora teres, Ramularia collo-cygni, Rhynchosporium secalis Rice (Oryza sativa) Cochliobolus miyabeanus, Fusarium fijikuroï, Magnaporthe oryzae, Microdochium oryzae, Pyricularia oryzae, Rhizoctonia oryzae, Rhizoctonia solani, Sarocladium oryzae, Ustilaginoides virens Potato ( Solanum tuberosum ) Alternaria alternata, Alternaria solani, Phytophtora infestans, Rhizoctonia solani Vine ( Viticultural wines ) Botrytis cinerea, Erysiphe necator, Plasmopara viticola, Guignardia bidwelli, Erysiphe necator, Diplodia seriata Soldier ( Glycine max ) Cercopora kikuchii, Colletotrichum dematium, Corynespora cassiicola, Fusarium graminearum, Pythium spp., Rhizoctonia solani, Sclerotinia sclerotiorum, Septoria glycines Apple tree ( Domestic apple ) Monilia fructigena, Monilia laxa, Pezzicula alba, Pezzicula malicorticis, Venturia inequalis Tomato ( Lycopersicon esculentum ) Phytophthora infestansBean ( Common bean ) Uromyces appendiculatus Radish (Radiash) Alternaria brassicae All Fruits and vegetables Botrytis cinerea Strawberry (Fragaria sp) Colletotrichum acutatum Carrots (Carrot) Alternaria alternata, Alternaria douci, Alternaria radicina Fishing (Prunus persica) and apricot (Prunus armeniaca) Monilia fructicola, Monilia fructigena, Monilia laxa

[0044] In a particularly preferred manner, the fungus or bacteria vs. culture plant pairs targeted by the invention are as follows: Wheat: Fusarium graminearum, Microdochium And Zymoseptoria of wheat Vineyard: Botrytis cinérea, Erysiphe necator, Plasmopara viticola, Guignardia bidwelli, Erysiphe necator, Diplodia seriata Potato : Alternaria alternata, Alternaria solani, Phytophtora infestans, Rhizoctonia solani Tomato: Phytophthora infestans Fighting process

[0045] The invention relates to a method for controlling fungi and / or oomycetes in plants and cultivated seeds, characterized by the following steps: Harvesting fresh cells of one or more microalgae of the genus Amphidinium ;Freezing and / or freeze-drying of said cells; suspension of said freeze-dried powder or frozen cells in water, in a weight ratio of 1:200 to 1:2 at a temperature above 60°C; application of the extract thus obtained to cultivated plants and / or seed coating. This control method can be curative or preventive, preferably curative.

[0046] Preferably, the suspension of said frozen cells or said lyophilized powder in an inorganic or organic solvent is carried out in a lyophilized powder or biomass / solvent weight ratio of between 1:100 and 1:50.

[0047] Preferably, the suspension of said frozen cells or lyophilized powder in water is carried out at a temperature above 80°C, particularly preferably at a temperature above 90°C. Preferably, the suspension of said frozen cells or lyophilized powder in water lasts less than 5 minutes, preferably less than 3 minutes, preferably less than 1 minute. Preferably, the temperature is then rapidly brought back to room temperature. Preferably, the temperature of the mixture is brought close to room temperature by placing the mixture in a cold environment, for example at a temperature close to 0°C, or by adding an inorganic solvent to the mixture at a temperature close to 0°C.

[0048] The suspension is made either by adding to the said frozen cells or lyophilized water previously brought to the desired temperature, or the water is added and the resuspended mixture is adjusted to the desired temperature.

[0049] Bringing the temperature "quickly" close to room temperature means in less than 5 minutes, preferably in less than 3 minutes, preferably in less than 1 minute.

[0050] The fresh cells harvested and extracted come from a cell culture under temperature, photoperiod and salinity conditions adapted to the strain concerned up to a cell concentration between 5.10 4< cells / ml and 5.10 6< cells / ml, preferably a cell concentration between 5.10 5< cells / ml and 1.10 6< cells / ml.

[0051] The cells are cultured for 5 to 20 days.

[0052] The light intensity is between 40 µE and 200 µE, preferably between 70 µE and 100 µE.

[0053] The growing temperature is generally between 17°C and 25°C.

[0054] The day / night photoperiod is preferably between 8am / 4pm and 4pm / 8am.

[0055] The minimum salinity is 15 ppt.

[0056] According to a particular embodiment, Amphidinium carterae is cultured as follows: the cells are incubated in natural or artificial seawater medium at a temperature between 17 and 25°C with a day / night cycle of between 8h / 16h and 16h / 8h, preferably 16h / 8h.

[0057] The application on cultivated plants can be carried out by any means known to a person skilled in the art that allows access to the parts of the plants affected by the fungus.

[0058] The extract is applied at a dose between 0.005 g / L and 20 g / L, preferably between 0.5 g / L and 10 g / L, particularly preferably between 1 g / L and 5 g / L.

[0059] Seed coating can be carried out by any technique known to a person skilled in the art which allows the active ingredient to remain in contact with the seed.

[0060] For example, coating can be achieved by powdering or spraying.

[0061] For example, the coating may include formulators and adjuvants.

[0062] The formulations aim to make it possible to apply and retain the active substance(s) on the grain, in equal and constant proportion throughout the entire application process of the product and this at very low doses.

[0063] The formulation agents include: organic solvents or water, dispersants, emulsifiers, surfactants or wetting agents, colorants...

[0064] Surfactants and emulsifiers have the property of bringing together and stably keeping two incompatible liquids together.

[0065] Various adjuvants can be applied to the seed. Coating agents involve applying a microporous film to the seed surface. They do not alter the seed's shape or size. They improve coverage and the uniformity of the treatment. When used by the farmer, they improve user comfort during sowing by suppressing dust and facilitating seed flow in the seed drill. They enhance the effectiveness of the active ingredient(s) under growing conditions. Coating agents modify the seed's shape, size, and weight. They improve sowing accuracy.

[0066] The control method according to the invention is particularly suitable against Fusarium wilt, preferably a Fusarium wilt listed in Table 1. Tableau 1: summary of fusarios Name of the disease Pathogen EPPO code basal fusarium wilt of asparagus Fusarium wilt FUSS Fusarium basale of beans Fusarium solani f. sp. phaseoli FUSASH Fusarium basale of peas Fusarium solani f. sp. pisi I was shot fusarium wilt of beet Fusarium oxysporum f. sp. beet FUSED fusariose de la pomme de terre Fusarium blue FUSASC fusariose de la reine-marguerite Fusarium oxysporum f. sp. conglutinans FLUFF corn stem fusarium wilt Gibberella fujikuroi GIBBFU corn stem fusarium wilt Fusarium wilt FUSS corn stem fusarium wilt Gibberella zeae GIBBZE Fusarium wilt of vanilla Fusarium oxysporum f. sp. vanillae FUSAVN pineapple fusarium wilt Gibberella fujikuroi var. sticking together GIBBFS Fusarium head blight of corn Fusarium wilt FUSS Fusarium head blight of corn Fusarium tricinct FOUND fusarium wilt of carnation Fusarium oxysporum f. sp. dianthi FUSED fusarium wilt of bromeliads Fusarium oxysporum f. sp. aechmeae FUSAAE Fusarium wilt of bulbs Fusarium oxysporum f. sp. gladiolus FUSAGL Fusarium wilt of cereals Fusarium culmorum FUSACU Fusarium wilt of cereals Gibberella rosea FUSARO Fusarium wilt of cereals Gibberella avenacea GIBBAV Fusarium wilt of cereals Gibberella intricans GIBBIN Fusarium wilt of cereals Monographella nivalis MONKS Fusarium head blight Gibberella zeae GIBBZE fusariosis of asparagus roots Fusarium oxysporum f. sp. asparagus FUSAAS fusariosis of cacti roots Fusarium oxysporum f. sp. opuntia FUSAOP fusariosis of tomato roots and neck Fusarium oxysporum f. sp. radicis-lycopersici FUSARL root and collar fusarium wilt of cucumber Fusarium oxysporum f. sp. cucumerinum FUSACC wheat fusarium wilt Gibberella fujikuroi GIBBFU Fusarium wilt of cocoa trees Albonectria rigidiuscula CALORIES Fusarium wilt of coffee Gibberella stilboides GIBBST fusarium wilt Fusarium oxysporum f. sp. safflower FUSACA Quince fusarium wilt Gibberella baccata HUBBED fusariose du collet des cucurbitacées Fusarium solani f. sp. cucurbitae FUSASU fusarium wilt of cotton Fusarium oxysporum f. sp. vasinfectum FUSS fusarium wilt of gerbera Fusarium oxysporum f. sp. gerberae FUSION fusarium wilt of gladiolus Fusarium oxysporum f. sp. gladioli FUSEGL fusarium wilt of flax Fusarium oxysporum f. sp. lini FUSAL corn fusarium wilt Gibberella acuminata GIBBAC corn fusarium wilt Gibberella fujikuroi var. sticking together GIBBFS corn fusarium wilt Gibberella zeae GIBBZE fusarium wilt of oil palm Fusarium oxysporum f. sp. elaeidis FUSEAL soybean fusarium wilt Fusarium oxysporum f. sp. glycines FUSION soybean fusarium wilt Fusarium oxysporum f. sp. tracheiphilum FUSE fusariose du tubercule de la pomme de terre Gibberella cyanogena GIBBCN fusarium wilt Gibberella fujikuroi GIBBFU Fusarium wilt Monographella nivalis MONGNI fusarium wilt Pink gibberella FUSE vascular fusariosis Fusarium oxysporum FUSAOX fusarium vascular de la lentille Fusarium oxysporum f. sp. lentis FUSION fusariose vasculare de la pastèque Fusarium oxysporum f. sp. niveum FUSANV fusariose vasculare de la tomate Fusarium oxysporum f. sp. tomato FUSED fusariose vascular de la tulipe Fusarium oxysporum f. sp. tulipae FOUNDATION vascular fusarium des cruciferes Fusarium oxysporum f. sp. conglutinans FLUFF fusariose vascular du caféier Gibberella xylarioides GIBBXY Fusarium wilt of cabbage Fusarium oxysporum f. sp. conglutinans FLUFF fusarium vascular du chrysanthème Fusarium oxysporum f. sp. chrysanthemi FUSACH Fusarium vascular two cucumber Fusarium oxysporum f. sp. cucumerinum FUSACC fusarium vascular du cyclamen Fusarium oxysporum var. aurantiacum FUSAAU fusarium vascular du fraisier Fusarium oxysporum f. sp. fragariae FUSAFR fusarium vascular du haricot Fusarium oxysporum f. sp. phaseoli FUSAPH fusariosis vascular of melon Fusarium oxysporum f. sp. melonis FUSED Fusarium vascular blight of peas Fusarium oxysporum f. sp. pisi FUSAPI Fusarium vascular du pois chiche Gibberella baccata HUBBED fusarium vascular du pois-chiche Fusarium oxysporum f. sp. chickpea FUSSED Fusarium vascular blight of radish Fusarium oxysporum f. sp. raphani FUSION

[0067] The control method according to the invention is particularly suitable for the following fungal vs. crop plant pairs: Blé : Fusarium graminearum, Microdochium nivale And Zymoseptoria of wheat Vineyard: Botrytis cinerea, Plasmopara viticola, Guignardia bidwelli, Erisyphe necator, Diplodia seriata Apple tree: Unequal Venturia Banana tree: Fusarium oxysporum And Mycosphaerella fijiensis EXAMPLES MATERIAL & METHODS Example 1 : Microalgae culture

[0068] The microalga Amphidinium cartae, strain AC208, comes from Algobank (Caen) and microalgae Small Prymnesium, strain RCC 1436, and Phaeodactylum tricornutum,CCMP 632 strains originate from the Roscoff Culture Collection (RCC). These microalgae are cultured in L1 artificial seawater (https: / / ncma.bigelow.org / algal-recipes) at 19°C with a 12-hour day / night cycle. The light intensity used is 100 µE. Biomass is harvested at the end of the exponential growth phase by centrifugation (15 min at 3000 RPM). The resulting cell pellet is frozen and then freeze-dried using a laboratory freeze dryer (Alpha 1-2 LDplus, labconco) to ensure stable preservation of the active material over a long period. After freeze-drying, the dry matter is weighed. Example 2 : Preparation of the extract

[0069] To extract the active ingredient from the dry matter of Example 1, 20 mg of dry matter are resuspended in 1 mL of distilled water at 100°C. After incubation for 2 minutes at room temperature (20–25°C), the extract is kept on ice and then centrifuged for 5 minutes at 10,000 rpm at room temperature. The supernatant containing the active ingredient is frozen in liquid nitrogen to preserve its long-term antifungal properties. Example 3 : Germination test Fusarium gramineae

[0070] The spores of Fusarium graminearum are cultured in the depleted "Mung bean" medium. The spores are separated from the mycelium by filtration through miracloth (Calbiochem), centrifuged, and then resuspended at 1.6 x 10⁶ spores / mL. Approximately 16,000 spores are incubated in the presence of the control solution or the A. extract. bagsat different concentrations. After an incubation of 10 min at room temperature, the spores are placed on a coverslip for counting germination after 6H or on a petri dish for observing mycelium growth after 72H. ESSAY

[0071] Extracts from different species of marine microorganisms belonging to three familyMajor phytoplankton, dinoflagellates, haptophytes, and diatoms, were tested for their potential antifungal activity against cryptogamic fungi. These microalgae have the capacity to produce toxins that allow them to proliferate rapidly by competing with other species, and are therefore potential sources of molecules that may exhibit antifungal activity. Extracts of each microalga were obtained according to Example 2. To test the effect of these extracts on the survival of phytopathogenic fungi, the freeze-dried extracts were resuspended in water and then brought into contact with a given quantity of spores. Fusarium graminearum. Example 4: Inhibition of spore growth and germination Fusarium gramineae

[0072] The capacity of F. graminearum the formation of mycelium on agar medium in the presence of these extracts is tested 72 hours later. Of the three extracts tested ( Prymnesium parvum, Amphidinium carterae And Phaeodactylum tricornutus ), only the extract d'Amphidinium carteraeAccording to Example 2, it has an inhibitory effect on mycelium formation ( Figure 1A ).

[0073] To confirm this result, a dose-response test was performed by incubating the spores with the extract of A. carterae according to Example 2 diluted to different concentrations ( Figure 1B ). It turns out that this extract has a fungal activity that is dose-dependent, with a minimum concentration to obtain 100% inhibition (MIC) of 0.4 g / L ( Figure 1B ).

[0074] Finally, the excerpt from A. bags According to Example 2, it was tested to inhibit the germination of spores of F. graminearum. The results in vitro results obtained 6 hours after incubation with the extract demonstrate a total inhibition of spore germination at a concentration of 2 g / L ( Figure 1C suggesting that the extract inhibits spore germination as well as mycelium growth F. graminearum. Example 5 : Influence of the lyophilization of the extract d'A. bags sur l'activité anti-fongique de l'extrait

[0075] The inventors determined whether the freeze-drying of the A. extract. bags inhibited or not the antifungal activity. For this, a culture of A. bags was extracted according to Example 2, then half of the extract was frozen at -80°C while the other half was lyophilized and then resuspended in distilled water. These extracts were tested at different concentrations for their ability to inhibit the growth of F. graminearum according to Example 3. The results demonstrate that in both cases, frozen extract or freeze-dried extract, complete absorption of growth of F. graminearum is obtained at a concentration of 1 g / L and persists up to 5 g / L ( Figure 1D ). In conclusion, the lyophilization of the A. extract. bags does not affect its antifungal activity in any way. Example 6: Tests sur des plants de blé infectés en conditions contrôlées

[0076] Wheat ears were inoculated with spores of F. graminearumunder controlled conditions and then 24 hours after the A extract. bags from Example 2 was applied. The reading of symptoms was done at 20 days (400°d) and at 22 days (450°d) after infection ( Figure 2A The number of ears showing symptoms (disease incidence) and the symptom score (disease severity, scored from 0 to 9) were reported in both cases: in the absence (control) and in the presence of the extract from Example 2. Compared to the control treatment, the presence of the extract significantly reduced the number of ears affected by the disease by approximately 30%. Furthermore, these ears exhibited symptoms with a reduced severity of approximately 50%. Figure 2B ). These results demonstrate that the extract of A. bags Example 2 possesses significant antifungal activity on the growth of phytopathogenic fungi affecting wheat under certain conditions in vitro And in the plant. Example 7: Tests sur plusieurs familles de phytopathogenes de lavine: Botrytis cinerea, an ascomycete responsible for gray rot, Plasmopara viticola, an oomycete responsible for mildew, Erisyphe the slayer, an ascomycete responsible for oidium and Diplodia seriata, one of the causative agents of bait, wood disease.

[0077] At a concentration of 1 g / L, the extract of A. bags example 2 completely inhibits the growth of P. viticola on a detached sheet ( Figure 3A (left side), whereas under the same conditions the extract has no effect on growth of E. necator ( Figure 3A (right side). Tests in vitro were conducted on Botrytis cinerea indicating that the extract completely inhibits the growth of B. cinerea from a concentration of 5 g / L ( Figure 3B ). The antifungal activity of the extract on B. cinerea was confirmed on a detached vine leaf ( Figure 3B Furthermore, tests were carried out. in vitro on the different families of fungi responsible for esca in grapevines. The results demonstrate that the extract at a concentration of 2 g / L significantly inhibits the growth of these fungi ( Figure 3C ). Example 8: In vitro tests on Microdochium majus, Fusarium graminearum, Zymoseptoria tritici, Fusarium oxysporum, Rhizoctonia solani and Phytophthora infestans

[0078] In order to determine if the extract from A. bags According to Example 2, it exhibits antifungal activity on a broad spectrum of phytopathogenic fungi; tests have been carried out on other fungi responsible for Fusarium wilt disease: Fusarium oxysporum (Fusarium wilt of banana) and Microdochium (Fusarium head blight of wheat) as well as on another important wheat disease: Septoria caused by Zymoseptoria of wheat. Tests were also carried out on two potato pathogens: the basidiomycete Rhizoctonia solani and the oomycete Phytophthora infestans. In all cases, the extract from A. bags According to Example 2, it severely limited the growth of fungi and oomycetes under the conditions in vitro (Tables 2 to 6). Table 2. in vitro grasses Efficacy of the microalgae extract against F. macroconidia grown on PDB medium at 25°C and in the dark for 24 and 72 h of incubation. Incubation time Efficacy fongicide (% du témoin non traité) a< 0.010 mg / ml 0.025 mg / ml 0.050 mg / ml 0.125 mg / ml 0.250 mg / ml 0.375 mg / ml 0.5 mg / ml 1.25 mg / ml 5.0 mg / ml 24 h 2.0 5.9 14.3 56.2 100.0 100.0 100.0 100.0 100.0 72 h 0.3 0.3 0.2 1.1 100.0 100.0 100.0 100.0 100.0 The fungicidal efficacy of the microalgae extract was determined after 24 and 72 h of incubation on PDB medium at 25°C and in the dark by measuring the optical density at 590 nm in each well of the 96-well microplate. Each value corresponds to the average of 3 replicates per tested condition. Table 3. in vitro Zymoseptoria tritici Rhizoctonia solani Microdochium majus Fusarium graminearum Efficacy of microalgae extract against strain Mg StA, strain Rsol AG3, strain Mmaj E11 and strain Fg 1. Pathogen Fungicidal efficacy (% of untreated control) a< 0.050 mg / ml 0.125 mg / ml 0.250 mg / ml 0.5 mg / ml 1.25 mg / ml 2.5 mg / ml 5.0 mg / ml Z. tritici 5.0 98.4 100.0 100.0 100.0 100.0 100.0 R. solani 5.7 71.1 100.0 100.0 100.0 100.0 100.0 Mr. Majus 16.2 42.4 100.0 100.0 100.0 100.0 100.0 F. graminearum 15.8 31.7 98.9 100.0 100.0 100.0 100.0 a< The fungicidal efficacy of the microalgae extract was determined after 72 h of incubation for Mr. Majus And F. graminearum or 5 days of incubation for Z. tritici And R. solani on PDB medium at 25°C and in the dark by measuring the optical density at 590 nm in each well of the 96-well microplate. Each value corresponds to the average of 3 replicates per tested condition. Table 4. Zymoseptoria tritici Rhizoctonia solani Microdochium majus Fusarium graminearum DE 50 and MIC (mg ma / ml) of microalgae extract against strain Mg StA, strain Rsol AG3, strain Mmaj E11 and strain Fg 1. Pathogen Fungicidal efficacy (mg ma / ml) a< OF 50 CMI Z. tritici 0,084 + / - 0,010 0,126 + / - 0,006 R. solani 0,106 + / - 0,015 0,189 + / - 0,041 Mr. Majus 0,123 + / - 0,009 0,266 + / - 0,019 F. graminearum 0,136 + / - 0,006 0,290 + / - 0,003 a< DE50: Effective dose of microalgae extract reducing the growth of tested pathogens by 50%, and MIC: Minimum Inhibitory Concentration, the lowest concentration that inhibits the growth of tested pathogens by 100%. Each value corresponds to the average of 3 replicates per tested condition + / - standard deviation. Table 5. in vitro Phytophthora infestans Fusarium oxysporum f. sp. cubense Efficacy of microalgae extract against PiF14 strain, CBS 102013 strain. Pathogen Fungicidal efficacy (% of untreated control) a< 0.050 mg / ml 0.125 mg / ml 0.250 mg / ml 0.5 mg / ml 1.25 mg / ml 2.5 mg / ml 5.0 mg / ml P. infestans 2,1 4,4 8,7 35,9 75,8 98,7 100.0 F. oxysporum f. sp. cubense 0,0 14,0 100.0 100.0 100.0 100.0 100.0 The fungicidal efficacy of the microalgae extract was determined after 72 h incubation for the 3 pathogens at 20°C and in the dark by measuring the optical density at 590 nm in each well of the 96-well microplate. Each value corresponds to the average of 3 replicates per tested condition. Table 6. Phytophthora infestans Fusarium oxysporum f. sp. cubense DE 50 and MIC (mg ma / ml) of the microalgae extract against strain PiF14, strain CBS 102013 Pathogen Fungicidal efficacy (mg ma / ml) a< OF 50 CMI P. infestans 0,70 + / - 0,040 5,0 + / - 0,0 F. oxysporum f. sp. cubense 0,175 + / - 0,02 0,25 + / - 0,03 a < DE 50: Effective dose of microalgae extract reducing the growth of tested pathogens by 50%, and MIC: Minimum Inhibitory Concentration, the lowest concentration that inhibits the growth of tested pathogens by 100%. Each value corresponds to the average of 3 replicates per tested condition + / - standard deviation. B < ai: No inhibition, even at the highest tested concentration of 5 mg / ml. Example 9 : Test in vitro And in planta (apple seedlings) with regard to apple scab (Venturia inaequalis)

[0079] The antifungal activity of extract D at 5 g / L was tested on petri dishes in the presence of spores of Venturia inaequalis The spores were inoculated 2 hours before or 3 hours after extract D. After 48 hours of incubation, the percentage of spore germination was evaluated. The presence of extract D, 2 hours before or 3 hours after inoculation, completely inhibited spore germination. V. inaequalis unlike the presence of water.

[0080] The tests in planta The following protocol was used on apple seedlings: 2 treatments tested: spraying of extract D at 5g / L 2h before inoculation (Extract Before) and spraying of extract D at 5g / L 3h after inoculation (Extract After) 3 control treatments: ∘2 untreated control treatments (water spraying on the same dates as the product) (Water Before and Water After) ∘ 1 treatment with a reference fungicide (captan)

[0081] Artificial inoculation of plants with a strain of Venturia inaequalis to 100,000 spores / ml. Notes of scab symptoms at 4 dates after inoculation (visual estimation of the % of scab-affected surface)

[0082] Biological material: Seedlings grown from apple seedlings in plug pots and approximately 3 weeks old - from seeds collected from the Gala variety (apples harvested in an orchard planted with Gala and Elstar) Spores of Venturia inaequalis on cellophane - EUB04 strain 3 boxes of 12 seedlings for each treatment Day 9, Day 14, Day 17, Day 21: Scoring as a percentage of leaf area reached (from 0 to 100% with a scale of 10% in 10% increments)

[0083] Since the conditions for normality and homogeneity of the residual variances were not met, a non-parametric Kruskal-Wallis test was performed. As this test was significant, the medians of the different categories were compared pairwise using the Nemenyi test based on the Tukey distance. These analyses were performed using R software (version 3.1.2).

[0084] The application of the extract from Example 2 did not result in phytotoxicity on the plants: no necrosis, chlorosis or blistering reaction was observed.

[0085] Observation at day 9: no symptoms of scab on any of the 5 modalities.

[0086] On the untreated witnesses(Water Before and Water After), scab developed well, reaching a median of 50 to 60% at day 21. No significant difference between the two water treatments regardless of the date.

[0087] Regarding the witness treated with captan, No scab development was observed.

[0088] Regarding the terms addressed (Extract before and Extract after), scab development is significantly lower than in untreated controls regardless of the observation date. Regardless of the observation date, there is no significant difference between the Extract before and captan treatment groups. 14 days post-inoculation, there is also no significant difference between the Extract after and captan treatment groups, but at 17 and 21 days post-inoculation, there is significantly more scab in the Extract after treatment group than in the captan treatment group. There are no significant differences between Extract before and Extract after.

[0089] The extract is very effective. A . carterae with regard to scab when applied 2 hours before inoculation or 3 hours after inoculation. Example 10 Test in planta on different species of Colletotrichum

[0090] In order to determine if the extract of A. carterae has a biocidal effect on the ascomycete Colletotrichum, two different species of Colletotrichum were tested: Colletotrichum fructicola And Colletotrichum orbiculare. For both species, the procedure is identical: a volume of extract at a given concentration (from 1 to 10 g / L), or a volume of water, was mixed with a volume containing 2 x 10⁶ spores of Colletotrichum fructicola or 2.10 6< spores of Colletotrichum orbiculare, Then, 10 µl spots were applied to detached strawberry or cucumber leaves, respectively. The leaves were kept in a petri dish under a humid atmosphere for 6 days at 24°C in a culture chamber (day / night; 14H / 12H). The results show that the extract of A . carteraecompletely inhibits the growth of these two species of Colletotrichum to starting from a concentration of 1g / L. Example 11: Testing the integrity of the cell wall and plasma membrane of conidiospores Fusarium graminearum

[0091] The conidiospores of F. graminearum are incubated for 1 hour in the presence of the extract according to example 2 (5 g / L) or of the same extract (5 g / L) inactivated by a temperature above 60°C. Propidium iodide is added to determine the membrane integrity of the spores.

[0092] The photographs show staining of conidiospores with propidium iodide in the presence of the extract according to example 2 (5 g / L) and not in the presence of the same extract (5 g / L) inactivated.

[0093] These results show that the extract according to example 2 acts by significantly increasing the porosity of the cell wall and plasma membrane of conidiospores of Fusarium graminearum.

[0094] All of these results demonstrate that the extract from A. carteraepossesses notable antifungal activity, whether under certain conditions in vitro Or in planta, on a broad spectrum of phytopathogenic fungi. BIBLIOGRAPHICAL REFERENCES

[0095] (1) Arseniuk, E., Foremska, E., Goral, T., Chelkowski, J. 1999. Fusarium head blight reactions and accumulation ofdeoxynivalenol (DON) and some of its derivatives in kernels of wheat, triticale and rye. Journal of Phytopathology 147, 577-590 (2) Devi P, Wahidulla S, Kamat T and D'Souza L (2011). Screening marine organisms for antimicrobial activity against clinical pathogens. Indian J.Geomar.Sci. (40) 338-346. (3) Mayer AM, Rodriguez AD, Taglialatela-Scafati O, Fusetani N (2013). Marine pharmacology in 2009-2011: marine compounds with antibacterial, antidiabetic, antifungal, anti-inflammatory, antiprotozoal, antituberculosis, and antiviral activities; affecting the immune and nervous systems, and other miscellaneous mechanisms of action. Mar Drugs. 11(7):2510-73 (4) Bowler, C., Vardi, A., & Allen, A. E. (2010). Oceanographic and biogeochemical insights from diatom genomes. Annual Review of Marine Science, 2, 333-65. doi:10.1146 / annurev-marine-120308-081051 (5) Murray S, Garby T, Hoppenrath M, Neilan BA (2012). Genetic diversity, morphological uniformity and polyketide production in dinoflagellates (Amphidinium, Dinoflagellata). PLoS One. 7(6) (6) Morsy N, Houdai T, Matsuoka S, Matsumori N, Adachi S, et al. (2006). Structures of new amphidinols with truncated polyhydroxyl chain and their membrane-permeabilizing activities. Bioorganic and Medicinal Chemistry 14: 6548-6554. (7) Nuzzo G, Cutignano A, Sardo A, Fontana A (2014). Antifungal Amphidinol 18 and its 7-sulfate derivative from marine dinoflagellate Amphidinium carterae, J. Nat. Prod., , 1524-1527.

Claims

1. A process for controlling crop plant and seed pathogenic fungi and / or oomycetes, characterized by the following steps: - Harvesting fresh cells from one or more microalga(e) of the genus Amphidinium; - Freezing and / or freeze-drying said cells; - Suspending said lyophilisate or said frozen cells in water in a weight ratio of 1:200 to 1:2 at a temperature greater than 60°C; - Applying the extract thus obtained to crop plants and / or coating seeds with said extract.

2. Process according to claim 1 wherein the or one of the microalgae of the genus Amphidinium is Amphidinium carterae.

3. Process according to claim 1 or 2, said extract comprising amphidinol 18 or amphidinol 19, preferably amphidinol 18.

4. Process according to any one of claims 1 to 3, wherein the fresh cells are harvested at a cell concentration comprised between 5.104 cells / ml and 5.106 cells / ml.

5. Process according to any one of claims 1 to 4, wherein said crop plant and seed pathogenic fungi are fungi pathogenic to crop plants and seeds of the genera Fusarium, Colletotrichum, Mycosphaerella, Phytophthora and Alternaria, preferably the pairs of fungi vs. crop plants Triticum sativum / Mycosphaerella graminicola - Triticum sativum / Fusarium graminearum - Solanum tuberosum / Phytophtora infestans - Vinis vitifera / Plasmospora viticola - Vinis vitifera / Erysiphe necator - Lycopersicon esculentum / Phytophtora infestans.

6. Process according to claim 5 wherein said fungi pathogenic to crop plants and seeds of the genera Fusarium, Colletotrichum, Mycosphaerella, Phytophthora and Alternaria are selected from the group consisting of Fusarium oxysporum, Fusarium solani, Fusarium avenaceum, Fusarium culmorum, Fusarium graminearum, Fusarium moniliforme, Fusarium poae, Fusarium proliferatum, Fusarium sporotrichioides, Fusarium subglutinans, Fusarium tricinctum, Colletotrichum acutatum, Colletotrichum graminicola, Colletotrichum coffeanum, Colletotrichum gloeosporioides, Mycosphaerella graminicola, Phytophthora infestans, Alternaria solani and Alternaria brassisicola.