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Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) Parasitic fungi on roses Marcel Pârvu1, Alina E. Pârvu2 1 Department of Biology, Faculty of Biology and Geology, "Babes-Bolyai" University, 42 Republicii Street, 400015 ClujNapoca, Romania. 2 Department of Pathophysiology, Faculty of Medicine, "Iuliu Hatieganu" University of Medicine and Pharmacy, 3 Victor Babes Street, 400012 Cluj-Napoca, Romania. Corresponding authors: [email protected], [email protected] Roses are susceptible to many diseases, and some of the major ones are caused by parasitic fungi like Podosphaera pannosa, Diplocarpon rosae, Phragmidium mucronatum and Botrytis cinerea. Powdery mildew is caused by P. pannosa, one of the most important fungal diseases of roses. P. pannosa mycelium and conidia are common on leaves and shoots of roses and infections are limited to the epidermal cells. Inside the host cell, P. pannosa haustoria provide a large area of contact with the host. A natural antagonist of P. pannosa is Ampelomyces quisqualis mycoparasite which forms typically pycnidia within different host structures. Black spot is caused by D. rosae and rose rust by P. mucronatum, a fungus which in the biological cycle presents five types of spores. Mycoparastism relations between roses and D. rosae and P. mucronatum were studied on the base of ultrastructural plant changes produced by the pathogens and on the mycelium development in plant tissues. Rose gray mold is caused by the B. cinerea species and the disease occurs on leaves or flower buds of plants. B. cinerea produces abundant gray mycelium and long and branched conidiophores that have ovoid and one-celled conidia. The B. cinerea conidia had numerous randomly positioned protuberances and a regular cell wall with a two-layer structure. The fungus frequently produces black and irregular sclerotia with distinct layers. The B. cinerea conidia lost viability due to severe ultrastructural changes induced by some plant extracts as Chelidonium majus and Berberis vulgaris. Key words: electron microscopy, fungal, parasitism, sporulation, ultrastructure 1. Introduction Roses continue to be one of the most popular garden flowers, as well as one of the most economically important ornamental flowers that are grown in the worldwide. In addition to their ornamental qualities, they possess some therapeutically important properties, for example the high levels of vitamin C and cancer-preventing compounds present in rose hips[1]. The susceptibility of roses to disease is the greatest risk for their quality. The major pathogens causing disease on rose include fungi, bacteria, nematodes, and viruses [2]. Several rose pathogens are capable of serious damage. Therefore, substantial research targeted the biology of rose pathogens, in order to increase rose’s resistance, to avoid excessive use of pesticides and to extend the use of biocontrol methods. The major parasitic fungi on roses are Podosphaera pannosa, Diplocarpon rosae, Phragmidium mucronatum, and Botrytis cinerea. Significant yield losses due to fungal attack limit both rose productivity and commercial value [3,4]. 2. Podosphaera pannosa Powdery mildew is caused by the fungus Podosphaera pannosa (syn. Sphaerotheca pannosa var. rosae) and it is one of the most important fungal diseases occurring on roses, both in the garden and in the greenhouse. This disease appears on roses year after year and causes reduced flower production and weakening of the plants by attacking their buds, young leaves, and growing tips [5]. P. pannosa are obligate, biotrophic fungi, meaning they can survive only on cells in specific living hosts. Despite their restrictive host specificity, powdery mildews are ubiquitous [2]. The mycelium and conidia of P. pannosa are common on leaves and shoots of cultivated and wild roses [6]. On young leaves the disease appears at first as slightly raised blister-like areas that soon become covered with a grayish white powdery fungus. As the leaves expand, they become curled and distorted, leading to shriveling and defoliation. On older leaves, as fungus grows, appear large white patches that cause little distortion but may eventually become necrotic. Young rapidly extending stem tissue can become infected too, often where a thorn attaches. The infection generally will persist as the stem matures, resulting in irregular powdery patches of fungus on the stem [2]. Sometimes buds are attacked, become covered with white mildew before they open, and either fail to open or open improperly [5]. P. pannosa infections are restricted to the epidermal surface. The fungus produces white mycelia that grow on the surface of the plant tissues and forms short and erect hyphae or conidiophores. At the tip of each conidiophore, chains of 5 to 10 ellipsoid-ovoid conidia (asexual spores) are produced (Figure 1A). Sexual spores are occasionally produced in spherical structures, ascomata, which appear as reddish-brown dots in the hyphal mats [5,7]. After germination, an © 2012 FORMATEX 207 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) appressoria develops at the end of the germination tube, which attaches the mycelium to the plant surface by a fine slime layer. A penetration peg emerges through a pore in the appressorium and enters the cuticle and underlying epidermal cell wall. In the epidermal cell, the penetration peg enlarges to form the haustorial neck. From the center of the attachment of the appressoria, multilobed, globose mature haustoria are formed. Inside the host cell, P. pannosa haustoria provide a large area of contact with the host (Figure 1B). Haustoria continue to form as hyphae extend along the leaf surface [2]. The haustoria serve to absorb nutrients for the fungus from the rose host. The absorption of nutrients from rose cells may sometimes lead to their death and in the affected areas photosynthesis is greatly reduced [5]. A B Fig. 1 Podosphaera pannosa: A. Light microscopic views of conidiophore (a) and conidia (b); B. Transmission electron micrograph of cross section through leaf rose showing a haustorium (h) and haustorial lobe (hl) of fungus in epidermal cell. In cold weather the production of conidia ceases and cleistothecia may be formed. Cleistothecia form occasionally toward the end of the season. Each cleistothecium contains a single ascus with 8 ellipsoid-ovoid spores [7]. Ascospores and conidia are carried by wind to young green tissues, and if the temperature and the relative humidity are sufficiently high spores germinate and infect these tissues. Control of rose powdery mildew relies mostly on the application of a variety of fungicides. However, these fungicides can be phytotoxic, and could cause the selection of resistant populations of rosae. For these reasons, alternative control measures like mineral salts, oils, plant extracts or biological control agents, in combination or as a replacement for fungicides are needed [8,9]. The oldest known and the commonest natural antagonists of powdery mildews is Ampelomyces quisqualis Ces [4,7,10,11]. The interactions between host plants, powdery mildew fungi and Ampelomyces mycoparasites are one of the most evident cases of tritrophic relationships in nature. When applied alone, A. quisqualis provides good control of rose powdery mildew [10]. Conidia of A. quisqualis are produced in pycnidia developed intracellularly in the mycelia of powdery mildew fungi [6,12,13]. A. quisqualis forms pale golden brown pycnidia which have different shapes (pear-shaped, spindle-shaped, spherical) depending on the P. pannosa fungus organ (hyphae, conidiophores and cleistothecia) in which they develop and act as parasites (Figure 2). When parasitizing conidiophores, A. quisqualis pycnidia are pear-shaped. In the case of parasitism of hyphae they are spindle-shaped and in the case of parasitism of cleistothecia they are almost spherical. Pear-shaped and spindle-shaped pycnidia of A. quisqualis are formed first, and spherical pycnidia appear at the end of the mycoparasite development cycle. The A. quisqualis mycoparasite pycnidiospores are one-celled, hyaline and smooth, with round, straight or slightly curved ends, and are embedded in a mucilaginous matrix inside the pycnidia [14]. In the presence of water, these matrices swell to several times their normal diameter, and conidia are released from intracellular pycnidia by the rupture of the pycnidial wall. Under high humidity conditions conidia germinate and the resulting A. quisqualis hyphae can penetrate the hyphae of powdery mildews in their vicinity. After penetration, the hyphae of Ampelomyces invade the P. pannosa mycelia internally, and produce their pycnidia mostly in the conidiophores and young, immature ascocarps of powdery mildews. Occasionally, they also produce pycnidia in the invaded hyphal cells. The life cycle starts again when pycnidia are mature [10]. Cross sections of A. quisqualis pycnidia showed that they have different shape and their wall is composed of cells of different shapes and sizes. The cells of the internal wall of pycnidia contain many lipids and have a comparatively larger diameter than those situated on the pycnidia surface. In the centre of the pycnidia is the tissue which forms the conidia (Figure 3). © 2012 FORMATEX 208 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) A B Fig. 2 Ampelomyces quisqualis: light microscopic views of pycnidium shapes (a) and conidium (b); A. Pear-shaped; B. Spindleshaped. A. quisqualis conidia can be dispersed within the same plant by rain or water run off from plant surfaces. It can also spread over long distances as hyphal fragments in parasitized and detached powdery mildew conidia. Ampelomyces was found to produce pycnidia saprophytically in the senescent or dead plant tissues at the end of the season, suggesting that these structures served as overwintering structures for Ampelomyces in the field. The conidia, the pycnidial cells and the cells of the resting hyphae of Ampelomyces produced in the mycelia of powdery mildews during the previous season can all initiate the life cycle of these mycoparasites in the spring [10]. Ampelomyces is good for P. pannosa biocontrol because the appearance of mature cleistothecia is affected by the hyperparasite, limiting the attack of powdery mildew on roses [14]. On the other hand, A. quisqualis is tolerant to several fungicides used against powdery mildews, so that integrated control may be possible [15]. A B Fig. 3 Transmission electron micrograph of cross section through Ampelomyces quisqualis pycnidia: A. Pycnidium (p) and conidium (c); B. Details of pycnidium (p) wall and conidium (c) ultrastructure. 3. Diplocarpon rosae Black spot is caused by D. rosa, a fungus that is obligate to the genus Rosa, and does not infect any other plant taxa. It is hemibiotrophic, because it is parasitic on living host tissue and also has some ability for saprophytic growth [16]. The disease appears as black spots on the leaves that may coalesce to produce large, irregular, black lesions. The leaf tissue around the lesions may turn yellow, and often entire attacked leaves become yellow and fall off prematurely, leaving the canes almost completely defoliated [5]. Black spot is the most damaging rose disease worldwide [17,18]. © 2012 FORMATEX 209 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) D. rosae is mainly spread through asexual spores, conidia. The sexual stage, represented by ascospores, is extremely rare and plays no part in the disease cycle. The fungus overwinters as mycelium, ascospores, and conidia in canes and fallen infected leaves. In the spring conidia are dispersed via water splash. The mycelium grows in the mesophyll and forms acervuli and conidia at the upper surface. The primary infection of leaves is caused by direct penetration of conidia and ascospores. Available water is necessary for the fungus to germinate and directly penetrate the epidermis of rose leaves and stems [5,19]. On susceptible rose genotypes D. rosae fungus produces Marssonina – type of 2-celled hyaline conidia from acervuli, within infection sites on leaves and stems, between the outer wall and cuticle of the epidermis (Figure 4). Subcuticular hyphae radiate from the infection site followed by branching intercellular hyphae that give rise to intracellular haustoria [16]. Conidia push up and rupture the cuticle [5]. A B Fig. 4 Diplocarpon rosae: A. Scanning electron micrograph of acervulus (a) and conidia (c) of the fungus; B. Transmission electron micrograph showing hyphae (hy) between the outer wall and cuticle (c) of the epidermis. Conidial morphology and colony color are quite variable among isolates when grown in culture, due to their genetic diversity reflected in pathogenic race diversity [19-21]. D. rosae fungus penetratation in cells and intercellular spaces of leaf mesophyll causes irreversible ultrastructural changes of the affected cells (Figure 5). The intercellular penetration damages plant cell membranes and increases nutrient leakage into intercelullar spaces. At the same time the physiological and biochemical processes of the plant cells are strongly modified by mycoparasitism, affecting the overall functioning of plant tissues and the growth process [22]. A B Fig. 5 Transmission electron micrograph of cross section through leaf rose showing hyphae (hy) of Diplocarpon rosae: A. In the tissue cells and intercellular spaces; B. In intercellular spaces and penetrating in the mesophyll cell (mc). © 2012 FORMATEX 210 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) 4. Phragmidium mucronatum Rose rust is caused by the P. mucronatum fungus and this disease appears in spring and persists until the leaves fall. Susceptibility to rust varies widely among rose cultivars. The rose rust appears on leaves as yellow to red circular spots on the upper surface, corresponding to pustules of red, orange or black spores on the lower surface. In late summer, on the lower surface of the leaf there are black pustules which contain teliospores. Rose rust often causes the death of rose shrubs due to premature defoliation of plant. P. mucronatum is an obligate parasite and an autoecious and macrocyclic fungus. During its biological cycle it presents five types of spores (teliospores, basidiospores, pycniospores, aeciospores and uredospores) appearing in a definite sequence. The urediniospores are one-celled and yellowish-orange (Figure 6), and the teliospores contain 6-8 cells with very dark and rough walls and a long stalk (pedicel) which becomes easily detached from the lesions of leaves [6] (Figure 7). A B Fig. 6 Scanning electron micrograph of the fungus Phragmidium mucronatum showing: A. Uredospores (u) and teliospores (t) on lower epidermis; B. Uredospore. Typically, P. mucronatum fungus produces intercellular, hyaline and septate hyphae and haustoria, all of which are involved in the absorption of nutrients from living cells of the host plants [23] (Figure 8). A B Fig. 7 Scanning electron micrograph of the fungus Phragmidium mucronatum showing: A. Teliospore with dark and rough wall and a long stalk; B. Teliopsore with dark and rough wall (detailed). © 2012 FORMATEX 211 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) A B Fig. 8 Transmission electron micrograph of cross section through leaf rose showing the Phragmidium mucronatum fungus: A. Hyphae (hy) of the fungus in the intercellular spaces and irreversible changes in the mesophyll cells; B. Haustorial lobe (hl) in the mesophyll cell. 5. Botrytis cinerea B. cinerea is a necrotrophic opportunistic plant pathogenic fungus, also known as “gray mould fungus”. It causes serious pre- and postharvest diseases in more than 200 plant species, including agriculturally important crops and harvested commodities, such as grapes, tomatoes, strawberries, cucumbers, bulb flowers, cut flowers and ornamental plants [24]. The broad host range of B. cinerea results in great economic losses, not only during growth but also during storage and transportation of products [25]. Necrotrophs kill their host cells by secreting toxic compounds or lytic enzymes and also produce an array of pathogenic substances that can subvert host defences [26]. B. cinerea strains are highly genetically and physiologically variable and several strains developed resistance to most of the fungicides used to control them [24,27,28]. Rose gray mold occurs on leaves or flower buds of plants. B. cinerea produces abundant gray mycelium and long and branched conidiophores, that have ovoid and one-celled conidia (Figure 9A). B. cinerea conidia appear dark because of melanin, which protects the spores against enzyme action and probably UV [29]. The mycelium grows and invades the tissues, which become covered with a whitish-gray mold. The surfaces of dry B. cinerea conidia and other Botrytis spp. have many short protuberances (Figure 9B). Hydration and redrying causes the disappearance of these protuberances [30,31]. A B Fig. 9 Botrytis cinerea: A. Light microscopic view of a conidiophore with conidia; B. Transmission electron micrograph of a cross section showing hyphal cells from the inner layer of sclerotium, embedded in a polysaccharide matrix (CW. cell wall; N. nucleus; C. cytoplasm; L. lipids; PM. polysaccharide matrix). The B. cinerea conidium ultrastructure presents a regular cell wall, approximately 300–400 nm thick, with a twolayer structure, plasmalemma, and cytoplasm matrix with nucleus, mitochondria and vacuoles. The cell wall external layer is thin and electron dense and the inner one is thick, uniform and less electron dense. The plasmalemma tightly adhered to the cell wall. The cytoplasm matrix (cytosol) is uniformly distributed, and the nucleus is up to 2 µm in diameter and ovoid or spherical in shape. Among cell organelles, mitochondria are numerous, usually ovoid and medium electron dense. Vacuoles are similar in size to mitochondria [30,32]. © 2012 FORMATEX 212 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) The B. cinerea fungus frequently produces black and irregular sclerotia with distinct layers at the surface of infected tissues and the fungus overwinters in this form. Transverse sections of B. cinerea sclerotia showed a cortex more compact than the medulla, with less extracellular matrix between the cells. The rind cells had darkly pigmented septa. The medullary cells were embedded in a continuous polysaccharide extracellular matrix, uninterrupted by lacunae showed in Figure 9B. The morpho-functional integrity of fungal cell components is required in order to maintain their viability and germination capacity. It has been demonstrated that Chelidonium majus [33] and Berberis vulgaris [34] plant extracts induced important irreversible ultrastructural changes to B. cinerea conidia which were visualized by electron microscopy (TEM) [35]. Important antifungal activity of Berberis spp. has been demonstrated against some fungal strains with hydroalcoholic extracts, aqueous extract, methanolic or crude extracts, and alkaloidal fractions [36]. Alcoholic extracts provide more complete extraction and include fewer polar compounds [37]. The in vitro antifungal activity of berberine isolated from the same sources has also been investigated and it was found that berberine alkaloids are cationic antimicrobials. Twenty-two alkaloids of medicinal importance have been reported so far from the roots, stems, leaves and fruit of Berberis spp. The alkaloid content differs in Berberis from different areas, species and organs [38]. Examination by SEM revealed that B. vulgaris bark extract, at its MIC, induced large-scale damage to B. cinerea conidia, because the surface protuberances from the control disappeared. On TEM micrographs, B. vulgaris bark extract caused a disruption of the B. cinerea conidial cell wall, the external layer was more electron dense, the plasmalemma and the cytoplasm of the B. cinerea conidia had shrunk and detached itself altogether from the cell wall, the organelles and nucleus were also partly destroyed. Berberine treatment caused similar changes to the B. cinerea conidia as B. vulgaris bark extract [34]. C. majus is a common, poisonous herbaceous perennial from the poppy family, commonly known as celandine. Plant extracts and their purified compounds have antibacterial, antiviral and fungicidal effects both in vitro and in vivo. Their properties were attributed mainly to alkaloids, several flavonoids and phenolic acids. The main alkaloids from C. majus extracts are chelidonine, chelerythrine, sanguinarine, coptisine and berberine [33,39]. On the SEM micrographs of the B. cinerea conidia treated with MFC of C. majus extract, the shape and size did not change but the surface protuberances disappeared. The TEM micrographs showed important irreversible ultrastructural changes: the cell wall had a slightly irregular outline, loosely distributed components and was highly permeable; the cell wall external layer was more electron dense; the plasmalemma was mostly destroyed and did not adhere to the cell wall; precipitation of the entire cytoplasm and destruction of organelles and nucleus were seen. Due to these effects, the morpho-functional relationship between the cell wall and the cytoplasm was destroyed and a less electron dense band was formed between the altered cytoplasm and the cell wall [33]. The precipitation of the cytoplasm and the destruction of the organelles and nucleus caused the loss of viability and germination capacity of B. cinerea conidia treated with plant extracts [30]. The antifungal effects of the studied plant extracts recommend them as good candidates for the in vivo biological control of phytopathogenic fungi, limiting the overuse of chemical fungicides [40]. 6.Conclusions During the past decades, studies focussing on rose pathogens have greatly increased. Rose diseases caused by the parasitic fungi P. pannosa, D. rosae, P. mucronatum and B. cinerea can be identified on the basis of the symptoms of disease and the ultrastructural characteristics of the pathogen. Less is known about the pathogenetic mechanisms. Because the parasitic fungi limit both productivity and commercial value of roses, disease control strategies demand the extension of nonchemical disease control and genomic approaches. The principal mechanisms involved include mycoparasitism, antibiosis, competition and induced resistance. Additional mechanisms include hypovirulence mediated through fungal viruses, reported for the first time in Botrytis cinerea and enzymatic interference with pathogenic enzymes [41,42]. Biological control methods seem to be safe and genetic resistance is effective and long lasting. Acknowledgements: These studies were financially supported by the Romanian Ministry of Education and Research from the CNCSIS grants 46/220/2006, 43/220/2007 and PNII–IDEI 2272/2008. References [1] [2] [3] Wen X, Xu Q, Cao Q, Deng X. Promising genetic resources for resistance to powdery mildew in chestnut rose (Rosa roxburghii) and its relatives in China. New Zealand J. Crop Hort. Sci. 2006; 34 (2):183–188. Whitaker VM, Hokanson SC. Breeding Roses for Disease Resistance. In: Janick J, ed. Plant breeding reviews. John Wiley &, Sons, Inc.; 2009; 31: 277-324. Volpin H, Elad Y. Influence of calcium nutrition on susceptibility of rose flowers to Botrytis blight. Phytopathology. 1991; 8:1390-1394. © 2012 FORMATEX 213 Current Microscopy Contributions to Advances in Science and Technology (A. Méndez-Vilas, Ed.) [4] Belanger RR, Labbe C, Jarvis WR. Commercial-scale control of rose powdery mildew with a fungal antagonist. Plant Dis. 1994;78: 420-424. [5] Agrios GN. Plant pathology. 5th ed. Elsevier Academic Press; 2005. [6] Webster J, Weber RWS. Introduction to fungi. Cambridge University Press; 2007. [7] Braun U. A monograph of the Erysiphales (powdery mildews). J. Cramer, Berlin-Stuttgart; 1987. [8] Paulitz TC, Belanger RR. Biological control in greenhouse systems. Annu. Rev. Phytopathol. 39:103-133. [9] Pasini C, D'Aquila F, Curir P, Gullino ML. Effectiveness of antifungal compounds against rose powdery mildew (Sphaerotheca pannosa var. rosae) in glasshouses. Crop Protection. 1997; 16(3): 251–256. [10] Kiss L, Russell JC, Szentiványi O, Xu X, Jeffries P. Biology and biocontrol potential of Ampelomyces mycoparasites, natural antagonists of powdery mildew fungi. Biocontrol Science and Technology. 2004; 14(7):635-651. [11] Ellis MB, Ellis JP. Microfungi on miscellaneous substrates. Croom Helm, London & Sidney; 1988. [12] Falk SP, Gadoury DM, Cortesi P, Pearson RC, Seem RC. Parasitism of Uncinula necator cleistothecia by the mycoparasite Ampelomyces quisqualis. Phytopathology. 1995;85:794-800. [13] Kiss L. Graminicolous powdery mildew fungi as new natural hosts of Ampelomyces parasites. Can J Bot.1997;75:680-683. [14] Pârvu M, Roşca-Casian O., Characteristics of Ampelomyces quisqualis mycoparasite identified on romanian roses infected with powdery mildew. Contrib. Bot. 2004;39:217-220. [15] Sundheim L. Control of cucumber powdery mildew by the hyperparasite Ampelomyces quisqualis and fungicides. Plant Pathol. 1982;31:209-214. [16] Blechert O, Debener T. Morphological characterization of the interaction between Diplocarpon rosae and various rose species. Plant Pathol. 2005;54:82–90. [17] Dobbs RB. Research battles blackspot in roses. Amer. Rose Annu.1984; 69:44-54. [18] Whitaker VM, Zuzek K, Hokanson SC. Resistance of 12 rose genotypes to 14 isolates of Diplocarpon rosae Wolf (rose blackspot) collected from eastern North America. Plant Breeding. 2007;126(1):83-88. [19] Allum JF, Bringloe DH, Roberts AV. Interactions of four pathotypes of Diplocarpon rosae with species and hybrids of Rosa. Plant Pathol. 2010; 59(3):516-522. [20] Whitaker VM, Zuzek K, Bradeen J, Hokanson SC. Culturing and long term storage of virulent races of the rose blackspot pathogen, Diplocarpon rosae Wolf. Acta Hort. 2007; 751:199–205. [21] Drewes-Alvarez R. Disease: Black spot. In: Roberts AV, Debener T, Gudin S, eds. Encyclopedia of rose science. Elsevier Academic Press, Oxford, UK. 2003:148–153. [22] Isaac S. Fungal-Plant Interactions. Chapman&Hall, London New York Tokyo Melbourne Madras;1992. [23] Cummins GB, Hiratsuka Y. Illustrated genera of rust fungi. American Phytopathological Society, St. Paul, Minnesota;2003. [24] Kars I, Krooshof G, Wagemakers CAM, Joosten R, Benen JAE, van Kan JAL. Necrotizing activity of five Botrytis cinerea endopolygalacturonases produced in Pichia pastoris. The Plant Journal. 2005;43:213-225. [25] Elad Y. Biocontrol of foliar pathogens: mechanisms and application. Commun. Agric. Appl. Biol. Sci. 2003;68:17-24. [26] Makovitzki A, Viterbo A, Brotman Y, Chet I, Shai Y. Inhibition of fungal and bacterial plant pathogens in vitro and in planta with ultrashort cationic lipopeptides. Appl. Environ. Microbiol. 2007;73:6629-6636. [27] Silva E, Valdés J, Holmes D, Shmaryahu A, Valenzuela PD. Generation and analysis of expressed sequence tags from Botrytis cinerea. Biol. Res. 2006;39:67-76. [28] van Baarlen P, Legendre L, van Kan JAL. Plant defence compounds against Botrytis infection. In: Elad Y, Williamson B, Tudzynski P, Delen N, eds. Botrytis: Biology, pathology and control. Netherlands: Kluwer Academic Publishers; 2004. [29] Epton HAS, Richmond DV. Formation, structure and germination of conidia. In: Coley-Smith JR, Verhoeff K, Jarvis WR, eds. The biology of Botrytis. London, UK: Academic Press; 1980:41–83. [30] Coley-Smith JR. Sclerotia and other structures in survival. In: Coley-Smith JR, Verhoeff K, Jarvis WR, eds. The biology of Botrytis. London, UK: Academic Press; 1980:314-317. [31] Doss RP, Christian JK, Potter SW, Soeldner AH, Chastagner GA. The conidial surface of Botrytis cinerea and several other Botrytis species. Can J Bot. 1997;75:612–617. [32] Segmüller N, Kokkelink L, Giesbert S, Odinius D, van Kan J, Tudzynski P. NADPH oxidases are involved in differentiation and pathogenicity in Botrytis cinerea. Mol. Plant. Microbe Interact. 2008;2:808-819. [33] Pârvu M, Pârvu AE, Crăciun C, Barbu-Tudoran L, Tămaş M. Antifungal activities of Chelidonium majus extract on Botrytis cinerea in vitro and ultrastructural changes in its conidia. J. Phytopathol. 2008;156:550-552. [34] Pârvu M, Pârvu AE, Crăciun C, Barbu-Tudoran L, Vlase L, Tămaş M, Roşca-Casian O, Tripon SC, Persecă O, Molnar AM. Changes in Botrytis cinerea conidia caused by Berberis vulgaris extract. Notulae Botanicae. 2010;38(3):15-20. [35] Hayat MA. Principles and techniques of electron microscopy: biological applications. Cambridge University Press, London; 2000. [36] Pârvu M, Roşca-Casian O, Crăciun C, Barbu-Tudoran L, Vlase L, Tămaş M, Danciu RM. Ultrastructural changes in Sclerotinia sclerotiorum sclerotia treated with Berberis vulgaris plant extract. IOBC/wprs Bull. 2007;30:149-152. [37] Webster D, Taschereau P, Belland RJ, Sand C, Rennie RP. Antifungal activity of medicinal plant extracts; preliminary screening studies. J. Ethnopharmacol. 2008; 115:140-146. [38] Stermitz FR, Lorenz P, Tawara JN, Zenewicz LA, Lewis K. Synergy in a medicinal plant: antimicrobial action of berberine potentiated by 5'-methoxyhydnocarpin, a multidrug pump inhibitor. Proc. Natl. Acad. Sci. U.S.A. 2000;97:1433-1437. [39] Saglam H, Arar G. Cytotoxic activity and quality control determinations on Chelidonium majus. Fitoterapia. 2003;74:127–129. [40] Pârvu M, Pârvu AE. Antifungal plant extracts. In: Méndez-Vilas A, ed. Science against microbial pathogens: communicating current research and technological advances. Formatex Research Center, Badajoz, Spain; 2011;2:1055-1062. [41] Jeger MJ, Jeffries P, Elad Y, Xu X-M. A generic theoretical model for biological control of foliar plant diseases. J. Theor. Biol. 2009; 256:201–214. [42] Whitaker VM, Bradeen JM, Debener T, Biber A, Hokanson SC. Rdr3, a novel locus conferring black spot disease resistance in tetraploid rose: genetic analysis, LRR profiling, and SCAR marker development. Theor Appl Genet. 2010; 120(3):573-585. © 2012 FORMATEX 214