Isolation and Identification of Tobacco rattle tobravirus Affecting Onion (Allium cepa L.) Plants in Egypt
Om-Hashim M. El-Banna,
Tobacco Rattle Virus (TRV) was isolated from naturally infected onion (Allium cepa L.) plants growing in the fields of onion plants during the survey carried out in two successive seasons (2007-2008 and 2008-2009) in seven Egyptian Governorates. Plants showing yellowing, malformation, yellow stripping, white necrotic stripes and stunting symptoms were collected and subjected to identification studies that based on host range, symptomatology, modes of transmission, serological tests, inclusion bodies and morphology of virus particles. The virus was transmitted by mechanical inoculation and by seeds. On the other hand, cytological changes accompanied with the infection were investigated. Different methods of serological detection of the virus were also tested. The obtained results indicated that the host range of the expanded to 7 different plant families. The virus was transmitted mechanically and by seeds with percentages ranged between 8-13%. Different serological methods were used successfully for detection of TRV i.e., DAS-ELISA, TBIA and DIBA. Infection of tobacco leaves with TRV resulted in the formation of amorphous inclusion bodies in the cytoplasm. Light microscopy examination of semi thin sections in both healthy and artificially infected onion leaves showed anatomical changes which reflecting on the external symptoms on infected plants. Also, electron microscopy observed tubular particles with two main dimensions (length 48-114 nm and 180-197 nm and 22 nm width). Investigation of ultrathin sections by transmission electron microscopy revealed changes in both nucleus and chloroplast. According to the available data, TRV was isolated and identified for the first time in Egypt from onion plants during the present study.
June 20, 2011; Accepted: July 27, 2011;
Published: October 25, 2011
Onion (Allium cepa L.) has a worldwide importance ranking second among
all vegetables in economic importance after tomatoes (Griffiths
et al., 2002). In Egypt, onion is the third vegetable crop more consumed
(15 kg/capita/year), after potatoes and tomatoes and it is cultivated all over
the country in Delta area and Upper Egypt (84.3% of total area) and new land
areas (15.7%). The main onion cultivars white (Giza-6) and red (Beheri) onion
are the most produced varieties. The current production area is being around
147,490 feddan with total production 1.3 million ton.
Tobacco Rattle Tobravirus (TRV). TRV was named after the rattle-like
sound produced by the dried-out tobacco leaves, when the wind blows through
an infected field (Visser et al., 1999). TRV has
probably one of the widest host range plant viruses which infect more than 100
plant species. Also, it could be transmitted by sap-inoculation to about 400
species belonging to more than 50 families, including both mono- and dicotyledonous
plants under greenhouse conditions (Harrison and Robinson,
1978; MacFarlane, 1999). TRV causes economic losses
in bulbs production, such as tulip, narcissus, crocus and gladiolus. In Egypt,
TRV was isolated from several plants i.e., gladiolus (Sabek,
1973), henbane (Hyoscyamus muticus L.), (Shafie,
1978) and from Kaki (Diospyros Kaki) (Zein, 2004).
For this reason, the aim of the present was to isolate and identify an isolate
of TRV from the naturally infected onion plants.
MATERIALS AND METHODS
Virus isolation: Leaf samples of onion (Allium cepa L.) plants
showing malformation, yellowing, yellow stripping, white necrotic stripes and
stunting symptoms were collected from fields of onion plants during the survey
carried out during the two successive seasons (2007-2008 and 2008-2009) among
seven Egyptian Governorates.
The Collected leaf samples were homogenized with 0.1 M phosphate buffer-solution,
pH 7(1:2 w/v) in a sterilized mortar. The infectious sap was passed through
double layers of cheese cloth. Ten seedlings of each of C. amaranticolor
and N. tabacum cv. White Burley were dusted with carborandum (600 mesh)
and inoculated with the sap. Seedlings of each host were inoculated with distilled
water to serve as control. The plants were grown in the greenhouse (22-25°C)
and observed daily for symptoms appearance. Single local lesion technique (Noordam
et al., 1973) was used for biological purification of TRV. The virus
was submitted for two serial passage in C. amaranticolor as a local lesion
host and propagated in N. tabacum cv. White Burley.
Identification of TRV: The virus was identified according to host range, symptomatology, modes of transmission, serological reactions using ELISA techniques and by light and electron microscopy.
Host range and symptomatology of TRV: Twenty seedlings of each species and varieties belonging to seven families i.e., Alliaceae, Amarnthaceae, Chenopodiceae, Compositae, Cucurbitaceae, Ebenaceae, Fabaceae and Solanaceae were inoculated with infectious sap. The seedlings were grown in the greenhouse and examined daily up to 30 days for symptoms development. The developed symptoms were recorded. Symptomless plants were checked by back inoculation into C. amaranticolor and/or using ELISA kit for TRV detection.
Modes of transmission
Mechanical transmission: Mechanical inoculation was carried out as mentioned before.
Seed transmission: TRV was tested in onion seed batches collected from mechanically inoculated plants. Seedlings of cvs. Giza 6, Giza 20 and red (Beheri) were inoculated with TRV under greenhouse conditions. Virus free seedlings for each cultivar were sown in 20 cm diameter clay pots one seedling for pots and kept in an insect proof green-house, mechanically inoculated with virus isolate. Inoculated plants were kept until seed maturation. Five hundred seeds from each cultivar were sown after 5 month storage at lab conditions in paper bags (22-25°C). Emerged seedlings of onion plants were observed for virus symptoms development. Percentage of seed transmission was calculated. One hundred seeds of healthy plants of each cultivar were sown under the same conditions as control.
Serological diagnosis: Several serologic techniques i.e., indirect ELISA,
DAS-ELISA, TBIA and DBIA were applied to test leaf samples randomly selected
from onion plants. Samples consisted of leaf disks homogenized in buffer (DAS-ELISA
or indirect ELISA) at a ratio of 1:2 (w/v). Control of healthy and infected
sap were used. ELISA kit for detection of TRV was supplied by SANOFI, Sante,
Animals, Paris and France. The method of Clark and Adams
(1977) was applied as follows:
Direct ELISA: DAS-ELISA protocol was developed for detection of the virus, using plates which were coated with immunoglobulin G (IgG) 200 μL well-1 diluted in coating buffer at 1:500 and incubated for 2 h at 37°C, then the wells were washed 3 times with Phosphate Buffer Saline Tween (PBST). The tested sample (extracted in sampling buffer), were added to duplicate wells. The plate was incubated at 4°C overnight. Wells rewashed 3 times as before. Two hundred microliters of IgG conjugate diluted (1:500) in conjugate buffer and incubated at 37°C for 2 h then washed. A hundred microliter of freshly prepared substrate was used.
Indirect ELISA: Indirect ELISA was applied according to the method described
by Clark and Adams (1977) and Koenig
(1981). The absorbance was measured at 405 nm using ELISA reader (Dynatech
MR 7000). Samples with an absorbance of at least twice that of healthy control
were considered positive for the virus.
Tissue blot immuno bindingassay (TBIA) and dot blot immuno bindingassay
(DBIA): Dot blot and tissue blot immunobinding assays were carried out as
described by Lin et al. (1990).
Cytological changes in TRV infected plants light microscopy of inclusion
bodies: Cytological changes were observed in N. tabacum cv. White
Burley 20 days after inoculation with TRV, epidermal stripe were taken from
the lower surface of leaves and were treated with 5% Triton x-100 for 10 min
to disrupt the plastids and facilitated the observation of the inclusions (Edwardson
et al., 1984).
Morphology of virus particles: Virus preparations were negatively stained
with 2% Phosphotungstic (PTA) acid (Noordam, 1973) and
mounted on carbon coated cupper grids (400 mesh) and examined by transmission
electron microscope (TEM Joel-1400 in the electron microscope unit Faculty of
Agriculture Research Park (FARP).Images were captures by CCD camera (EMT) at
magnifications of 40000X.
Generic processing protocol: Onion leaves tissue infected with either OYDV
or TRV, 45 days after transplanting were cut into small pieces about 1-2 mm.,
fixed in 2% glutraldhyde in 0.1 M Na-Cacodylate buffer, pH 7.2 and subjected
to a vacuum for 1-4 min every 15 min for 2 h on ice. Prior to vacuum treatment,
floating samples were poked under the buffer surface with pointed metal pokers.
Rinsing took place in 0.1 M Na-Cacodylate buffer, pH 7.2, for 45 min, with buffer
changes at 15 and 30 min. Further fixation in 1% Osmium Tetraoxide in Na-Cacodylate
buffer, under intermittent vacuum and poking, took place for 1.5 h (Osmont
and Freeling, 2001). Samples were then rinsed in the Na-Cacodylate buffer.
Samples were dehydrated through an Ethanol series in buffer: 35, 50, 70, 80,
95, 100 and 100% for 60 min. each, then infiltrate with res. Ultra-thin sections
were cut using ultramicrotome Leica model EM-UC6 at thickness 90 nm, mounted
on copper grids (400 mish). Sections were stained with double stain (Uranyl
acetate 2% 10 min followed by Lead citrate for 5 min and examined by transmission
electronmicroscope JEOL (JEM-1400) at the candidate magnification. Images were
captured by CCD camera model AMT, optronics camera with 1632x1632 pixel formate
as side mount configuration (Osmont and Freeling, 2001).
Isolation of TRV: The virus was isolated from naturally infected onion
(Allium cepa L.) plants collected from onion fields during the survey
carried out during the two successive seasons (2007-2008 and 2008-2009) in seven
Identification of the virus isolate: TRV was identified according to host range, symptomatology, modes of transmission, serological reactions using (ELISA) techniques, inclusion bodies and morphology of virus particles.
Host range and symptomatology of TRV: As shown in Table
1 and Fig. 1 all plant species and cultivars belonging
to Alliaceae, Amarnthaceae, Chenopodiceae, Cucurbitaceae, Fabaceae and Solanaceae
the virus were reacted positively with TRV inoculation. Only Zinnia elegance
and Vicia faba L. cv. Giza 3 reacted negatively with TRV. The tested
hosts could be classified according to their reactions as follows: firstly,
systemic symptoms varied between mild and severe were observed on the tested,
A. ascalonicum, A. kurrat, D. stramonium, N. rustica, N.
tabacum White Burley plants, 2-3 weeks after inoculation with
TRV. Secondly, TRV produced local lesions on the inoculated leaves of Cucucmis
sativus Baladi, Gomphrena globosa, chlorotic and white
necrotic stripes on onion, Allium cepa Giza 6 and 20
and Beheri; A. sativum, Phaseolus vulgaris Giza
1 and Cucurbita pepo. Thirdly, inoculatedleaves of C. album,
C. amaranticolar and C. quina, reacted with local infection followed
by systemic symptoms. TRV was not detected either by ELISA or back inoculation
into the indicator test plants which gave no symptoms.
Modes of transmission
Mechanical transmission: The virus was transmitted by mechanical inoculation
from infected source plants to the indicator test plants. Infection was confirmed
by back inoculation and/or by ELISA.
|| Reaction of different hosts to infection with TRV
|Ch: Chlorotic, St: Stunting, Chs: Chlorosis, YR: Yellow rings,
CLL: Chlorotic local lesion, YS: Yellow stripping, NLL: Necrotic local lesion,
WN: White necrotic, PP: Pin point, WNS: White necrotic stripes, SM: Systemic
mosaic, -: No reaction
||Reaction of some hosts with TRV infection: (a) White necrotic
stripe on onion (Allium cepa L. cv. Beheri), (b) Pin point on Phaseolus
vulgaris, (c) Necrotic local lesion on C. amaranticolor, (d)
Necrotic local lesion on Nicotiana glutinosa, (e) Chlorotic local
lesion on C. album and (f) Chlorosis on Solanum tuberosum
|| Seed transmission of TRV
|Serological diagnosis: Direct and indirect ELISA were used
to confirm the identity of TRV, positive reaction was obtained with the
virus and its specific antiserum
|| Detection of TRV by DAS-ELISA, TBIA and DBIA
Seed transmission: Results in Table 2 showed that TRV could be transmitted through onion seeds of the three tested onion cultivars with different transmission percentages. The percentages of transmission ranged from 8,10 and 13% in Giza 20, Giza 6 and Beheri, respectively. This high percentage of seed transmission is very effective as a source of early infection in the field.
Tissue blot immunobinding assay (TBIA) and dot blot immunobinding assay (DBIA): The antiserum of TRV successfully detected infected samples as shown in Fig. 2. DBIA and TBIA were able to detect TRV in onion leaves. Infected samples changed to purple color while healthy ones remained green. The advantage of DBIA technique for detection of small amounts of antigen over standard ELISA and also provides simplicity, rapidity, sensitivity and it is convenience for large numbers of samples.
Cytological effects of TRV infection: Light microscopy: Amorphous cytoplasmic inclusion bodies were observed with light microscopy in epidermal stripe of TRV-infected onion leaf, taken from the lower surface of systemically infected N. tabacum cv. and White Burley, 20 days after inoculation (Fig. 3).
Semi thin sections: Semi thin sections of both TRV infected and healthy
onion plants were examined after staining with Tiludine blue by light microscope.
The investigations revealed large differences between infected and healthy tissues
(Fig. 4). Mesophyll layer was reduced in infected plants (Fig.
4b) compared with healthy ones (Fig. 4a). The spongy tissue
was more compacted, characterized with reduced intracellular space (Fig.
4d) in comparison with tissues of healthy plants (Fig. 4c).
The number of chloroplasts was reduced in the infected cells than in healthy
ones (Fig. 4f, E, respectively).
||Amorphous inclusion bodies in epidermal cells of N. tabacum
cv. White Burley (a) and Healthy (b). (X-200) NU: Nucleus, AIB: Amorphous
||Light microscopy of semi thin sections of both TRV- healthy
and infected Beheri onion plants (a, b), mesophyll cells (c, d) spongy tissues
(e, f) chloroplasts in parenchyma cells and phloem tissues of healthy (g)
and diseased leaves (h). Ch: Chloroplast, M: Mesophyll, N: Necrosis, S:
Spongy tissue, IS: Intercellular spaces, PC: Palisade cells, V: Vacuoles
This finding reflects the symptoms of chlorotic stripe on TRV-infected leaves.
On the other hand, the phloem tissues were also affected and necrosis was observed
in the infected (Fig. 4h) comparing with healthy tissues (Fig.
||Electron micrograph of purified TRV negatively stained with
2% phosphotungestic acid
||Electron micrographs representing the effect of TRV-infection
on onion cell organelles compared with those of healthy cells. (a): Mesophyll
cell of healthy onion leaf with normal shape and number of chloroplasts
(arrow), (b): Cell of TRV-infected leaf showing several degrees of chloroplast
deformation and degradation, (c): Normal chloroplast at high magnification
compared with affected, (d): One, (e): The nucleus of infected cell swollen
and the chromatin is segmented and (f). Ch: Chloroplast and Chr: Chromati
Electron microscopy: The morphology of TRV particles was studied by electron microscopy using virus preparation negatively stained with 2% phospotungestic acid. Tubular particles with two different lengths of 48-114 nm and 180-197 and 22 nm width were observed (Fig. 5).
Ultrathin sections: Investigation of ultrathin sections by Transmission
electron microscope revealed changes in the different tissues and cell organelles
as illustrated in (Fig. 6). The number and organization of
chloroplast was different in cells of infected onion tissues. The chloroplasts
exhibited several degrees of deformation and lysis (Fig. 6b,c
and e) in comparison with healthy tissues (Fig.
6a, d). The nucleus of infected cells also affected as
observed to be misshapen and the chromatin material was segmented (Fig.
Crops of cultivated Allium species are commonly infected with one or
more viruses, especially when propagated vegetatively (Bos,
1983; Walkey, 1990). Approximately 20 viruses infect
Allium, of which about nine are considered to be the most important because
they are widely distributed and often occur at a high incidence in Allium
crops (Barg et al., 1997; Chen
et al., 2004). TRV had earlier been reported in garlic, onion, A.
moly and A. ursinum in Europe (Bos, 1983;
Van Dijk, 1993; Uhde et al.,
In this study, TRV was isolated from naturally infected onion plants. All tested
plant species and cultivars belonging Alliaceae, Amarnthaceae, Chenopodiceae,
Cucurbitaceae, Fabaceae and Solanaceae reacted positively with TRV. Only Zinia
elegance reacted negatively with TRV inoculation. The results are in agreement
with those obtained by Shafie (1978). On the contrary,
Zein (2004) recorded several differences in host range
studies, such results could be attributed to virus strain, tested plant species
and physiological stage of host plants during inoculation process.
On the other hand, Van Dijk (1993) reported that natural
infection of onion and garlic with an isolate of TRV showed cholorotic and white
necrotic stripe on the leaves.
Systemic symptoms varied from mild to severe, were observed on the tested, A. ascalonicum L., A. kurrat L., Datura stramonium and N. tabacum cv. White Burley plants, 2-3 weeks after inoculation with TRV. Whilst, local lesions produced on the inoculated leaves of C. album, C. amaranticolar, C. quina, Cucurbit pepo, Cucucmis sativus cv. Baladi and Gomphrena globosa, but produced pin pointon Phaseolus vulgaris L. cv. Giza 1.
Inoculatedleaves of N. glutinosa and N. rustica reacted with
infection as local lesions host followed by systemic symptoms while chlorotic
and white necrotic stripes on onion Allium cepa cv. (Giza 6, 20 and Beheri).
Also, A. sativum L. reacted with TRV-infection as local lesion followed
by systemic symptoms. TRV was not detected either by ELISA or back inoculation
into the indicator test plant which gave no symptoms. These results have already
been recorded by Kirk et al. (2008) who transmitted
TRV mechanically from potato cv. FL1879 tubers onto tobacco cv. Samsun NN. Also,
Koike et al. (2010) isolated TRV from infected
spinach in the fields to Chenopodium quinoa, C. murale, C. capitatum, spinach
andsugar beet (Beta vulgaris).
It was noticeable that TRV was transmitted through seeds of Beheri cv with
high percentage being 13%. This high percentage of seed transmission considered
as a very effective source of early infection in the field. Seed transmission
of TRV through onion seeds was not previously recorded, but its transmission
through different hosts was reported by Lister and Murant
(1967) through some weeds i.e., Capsella bursa-pastoris, Myosotis arvensis,
tomatoes (Visser et al., 1999; Dikova,
2005) and sugar beet seeds.
Concerning serologic detection, DBIA and TBIA techniques proved to be able
to detect TRV in infected plants. These results have already been declared by
Kamenova and Adkins (2004), Lin
et al. (1990), Fegla et al. (2001)
and Ghanem et al. (2002).
Amorphous cytoplasmic inclusion bodies were observed with light microscopy
in infected epidermal stripe with N. tabacum cv. White Burley leaves.
Similar results were reported by Biljana and Polak (1968)
who observed inclusion bodies contain mature virions in epidermal cells of tobacco
infected by Tobacco rattle virus. Mesophyll layer was reduced in infected plants
compared with healthy plants. The spongy tissue was more compacted, characterized
with reduced intracellular space in comparison with healthy tissues. The number
of chloroplasts was reduced in infected cells than in healthy ones, it might
be due to the degradation of the chloroplasts. This finding reflects the symptoms
of chlorotic stripe on TRV-infected leaves. On the other hand, the phloem tissues
were also affected and necrosis was observed in infected compared with healthy
tissues. The anatomical changes were previously reported and explained by several
investigators who indicated that the chloroplasts and nuclei are the most organelles
affected by viral infections (Kim et al., 1989;
Ahmed, 1996; Sallam et al.,
1999). Also, Ibrahem et al. (1997) observed
necrosis in the phloem of vascular bundles of wheat leaves infected by Barley
yellow dwarf virus. Matthews (1991) found that these expected
changes in chloroplasts and nucleus are involved in virus replication and virus
particles might accumulate in these two organelles.
The morphology of TRV particles was studied by electron microscopy using virus
preparation negatively stained with 2% phospotungestic acid. Tubular particles
with two different lengths of 48-114 and 180-197 and 22 nm width were observed.
These results are similar with those recorded by Lister
and Bracker (1969).
Finally, according to the present study, TRV was isolated and identified for the first time in Egypt from onion plants during the present study. We recommend prevention of seed collection from cultivated areas infected with TRV to be used for onion cultivation in the next plantations.
Ahmed, H.H., 1996. Some viral disease of vegetables in Ismailia area. M.Sc. Thesis, Faculty of Science, Suez-Chanal University, El-Ismailia.
Barg, E., D.E. Lesemann, H.J. Vetten and S.K. Green, 1997. Viruses of alliums and their distribution in different Allium crops and geographical regions. Acta Horticulturae, 433: 607-616.
CrossRef | Direct Link |
Biljana, P.B. and Z. Polak, 1968. Intracellular inclusions epidermal cells of tobacco infected by Tobacco rattle virus. Biol. Plantarum, 11: 245-247.
Bos, L., 1983. Viruses and virus diseases of Allium species. Acta Hortic., 127: 11-29.
Chen, J., H.Y. Zheng, J.F. Antoniw, M.J. Adams, J.P. Chen and L. Lin, 2004. Detection and classification of allexiviruses from garlic in China. Arch. Virol., 149: 435-445.
Clark, M.F. and A.N. Adams, 1977. Characteristics of the microplate method of enzyme-linked immunosorbent assay for the detection of plant viruses. J. Gen. Virol., 34: 475-483.
CrossRef | PubMed | Direct Link |
Dikova, B., 2005. Tobacco rattle virus transmission by sugar beet seeds. Biotechnol. Biotechnol. Equipment, 19: 87-90.
Edwardson, J.R., R.G. Christie and N.J. Ko, 1984. Potyvirus cylindrical inclusion- subdivision-IV. Am. Phytopathological Soc., 74: 1111-1114.
Fegla, G.I., H.A. Younes and M.H.A. El-Aziz, 2001. Comparative studies for detection of Tomato mosaic Tobamovirus (ToMv), Cucumovirus (CMV) and Potato Y potyvirus (PVY). J. Adv. Agric. Res., 6: 239-254.
Ghanem, G.A.M., G.R. Stino and A.A. Semia, 2002. The use of modern methods for the detection and elimination of Apple Chlorotic Leaf Spot Trichovirus (ACLST) from apple trees in Egypt. Egypt. J. Phtopathol., 30: 1-23.
Griffiths, G., L. Trueman, T. Crowther, B. Thomas and B. Smith, 2002. Onions-a global benefit to health. Phytother. Res., 16: 603-615.
CrossRef | PubMed | Direct Link |
Harrison, B.D. and D.J. Robinson, 1978. The tobraviruses. Adv. Virus Res., 23: 25-77.
Ibrahem, A.M.I., N.A. Zaher, A.S.G. El-Din and H.M. Waziery, 1997. Histological and Agronomical studies on wheat plant infected with Barley Yellow Dwarf Virus (BYDV). Eygpt. J. Applied Sci., 12: 206-216.
Kamenova, I. and S. Adkins, 2004. Comparison of detection methods for a novel tobamovirus isolated from Florida hibiscus. Plant Dis., 88: 34-40.
Kim, K.S., D. Gonsalves, D. Yeliz and K.W. Lee, 1989. Ultrastructure and mitochondrial vesiculation associated with closterovirus like particles in leaf roll-diseased grape virus. Phytopathology, 79: 357-360.
Kirk, W.W., S.L. Gieck, J. M. Crosslin and P.B. Hamm, 2008. First report of corky ringspot caused by Tobacco rattle virus on potatoes (Solanum tuberosum) in michigan. Plant Dis., 92: 485-485.
Koenig, R., 1981. Indirect ELISA methods for the broad specificity detection of plant viruses. J. Gen. Virol., 55: 53-62.
Koike, S.T., T. Tian and H.Y. Liu, 2010. First report of tobacco rattle virus in Spinach in California. Plant Dis., 94: 125-125.
Lin, N.S., Y.H. Hsu and H.T. Hsu, 1990. Immunological detection of plant viruses and a mycoplasmalike organism by direct tissue blotting on nitrocellulose membranes. Phytopathology, 80: 824-828.
CrossRef | Direct Link |
Lister, R.M. and A.F. Murant, 1967. Seed-transmission of nematode-borne viruses. Ann. Applied Biol., 59: 49-62.
Lister, R.M. and C.E. Bracker, 1969. Defectiveness and dependence in three related strains of Tobacco rattle virus. Virology, 37: 262-275.
MacFarlane S.A., 1999. Molecular biology of the Tobraviruses. J. General Virol., 80: 2799-2807.
Direct Link |
Matthews, R.E.F., 1991. Plant Virology. 3rd Edn., Academic Press, San Diego, Pages: 835.
Noordam, D.D., 1973. Identification of Plant Viruses: Methods and Experiments. Center for Agricultural Publishing and Documentation, Netherlands, ISBN-13: 9789022004647, Pages: 207.
Osmont, K. and M. Freeling, 2001. Characterization of extended auricle (eta) a developmental mutant that affects the blade/sheath boundary in maize. Proceedings of the 43rd Maize Genetics Conference, March 15-18, 2001, Lake Geneva, WI -.
Sabek, A.H.M., 1973. Studies on viruses affecting gladiolus in A.R.A. M.Sc. Thesis, Faculty of Agriculture, Ain Shams University.
Sallam, A.A.A., M.A. Baraka and E.K.F. Yossef, 1999. Effect of Broad bean stain virus on chemical and anatomical structure of broad bean plants. Proceedings of the 8th National Conference of Pests and Diseases of Vegetables and Fruits, November 9-10, 1999, Ismailia, Egypt, pp: 216-227.
Shafie, M.S.A., 1978. Further studies on viral diseases of some medicinal plants. Ph.D. Thesis, Faculty of Agriculture Ainmal Shams University.
Uhde, K., R. Koenig and D.E. Lesemann, 1998. An onion isolate of Tobacco rattle virus: Reactivity with an antiserum to Hypochoeris mosaic virus, a putative furovirus, and molecular analysis of its RNA 2. Arch. Virol., 143: 1041-1053.
Van Dijk, P., 1993. Carlavirus isolates from cultivated Allium species represent three viruses. Netherlands J. Plant Pathol., 99: 233-257.
CrossRef | Direct Link |
Visser, P.B., A. Mathis and H.J.M. Linthorst, 1999. Tobraviruses. In: Encyclopedia of Virology, Granoff, A. and R.G. Webster (Eds.). 2nd Edn., Academic Press, San Diego, pp: 1784-1789.
Walkey, D.G., A.A. Alhubaishi and M.J. Webb, 1990. Plant virus diseases in the Yemen Arab republic. Tropical-Pest-Manage., 36: 195-206.
Zein, S.N., 2004. Characterization of tobacco rattle tobravirus from Kaki (Diospyros kaki). Egypt. J. Virol., 1: 187-193.