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Louisiana State University Louisiana State University
LSU Digital Commons LSU Digital Commons
LSU Historical Dissertations and Theses Graduate School
1994
Interactions Between Fusarium Oxysporum F. Sp. Lycopersici and Interactions Between Fusarium Oxysporum F. Sp. Lycopersici and
Nonpathogenic Strains of Fusarium Oxysporum. Nonpathogenic Strains of Fusarium Oxysporum.
Monica Michelle Lear Louisiana State University and Agricultural & Mechanical College
Follow this and additional works at: https://digitalcommons.lsu.edu/gradschool_disstheses
Recommended Citation Recommended Citation Lear, Monica Michelle, "Interactions Between Fusarium Oxysporum F. Sp. Lycopersici and Nonpathogenic Strains of Fusarium Oxysporum." (1994). LSU Historical Dissertations and Theses. 5736. https://digitalcommons.lsu.edu/gradschool_disstheses/5736
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O rder N um ber 9502122
Interactions between Fusarium oxysporum f. sp. Lycopersici and nonpathogenic strains of Fusarium oxysporum
Lear, Monica Michelle, Ph.D.
The Louisiana State University and Agricultural and Mechanical Col., 1994
U M I300 N. ZeebRd.Ann Arbor, MI 48106
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INTERACTIONS BETWEEN FUSARIUM OXYSPORUM F. SP. LYCOPERSICI AND
NONPATHOGENIC STRAINS OF FUSARIUM OXYSPORUM
A Dissertation
Submitted to the Graduate Faculty of the Louisiana State University and
Agricultural and Mechanical College in partial fulfillment of the
requirements for the degree of Doctor of Philosophy
in
The Department of Plant Pathology and Crop Physiology
byMonica Michelle Lear
B. S., Louisiana State University, 1982 . M. S., Louisiana State University, 1986
May 1994
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ACKNOWLEDGEMENTS
I would like to thank the following people:
My committee, including my major professor, Dr. R. W. Schneider, Dr. C.A. Clark, Dr. J. Hoy, Dr. M. C. Rush, Dr. E. Dunigan, and Dr. T. Bricker, for serving and helping me complete this dissertation.
The office staff of the Department of Plant Pathology and Crop Physiology, including Mildred Charles and Jill Atwood but especially Mrs. Patricia Hives, for staying after me.
My family for their encouragement and support.
All my friends, whom I will not name for fear of forgetting someone very important, who helped me keep working at it especially when I didn't want to.
My co-workers at the Louisiana Department of Agriculture and Forestry, Horticulture and Quarantine Division, for their patience, support, and help.
Commissioner Bob Odom for pressing me until I finally finished this.
ii
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TABLE OF CONTENTS
page
ACKNOWLEDGEMENTS ........................................................................................................... ii
LIST OF TABLES .................................................................................................................... jv
LIST OF FIG URES.................................................................................................................... vi
A B S T R A C T ..................................................................................................................................vii
CHAPTER
1 REVIEW OF LITERATURE.................................................................................. 1Literature Cited in Chapter 1 ..................................................................... 10
2 SELECTION OF AN ORANGE MUTANT OF FUSARIUMOXYSPORUM F. SP. LYCOPERSICI.......................................................... 14Introduction...................................................................................................... 15Materials and Methods ................................................................................ 16Results .............................................................................................................. 20Discussion.........................................................................................................28Literature Cited in Chapter 2 .....................................................................31
3 COMPETITIVE INFECTION STUDIES BETWEEN PATHOGENICAND NONPATHOGENIC ISOLATES OF FUSARIUM OXYSPORUM 33Introduction ......................................................................................................3 4Materials and Methods ................................................................................36Results ..............................................................................................................42Discussion.........................................................................................................50Literature Cited in Chapter 3 ................................................................ 54
4 ISOZYME ANALYSIS OF SELECTED VEGETATIVE COMPATIBILITYGROUPS OF NONPATHOGENIC FUSARIUM O X Y S P O R U M 58Introduction ......................................................................................................59Materials and Methods ................................................................................60R e s u lts ..............................................................................................................65Discussion........................................................................................................ 66Literature Cited in Chapter 4 .....................................................................71
APPENDICES
A MEDIA RECIPES...............................................................................................74B BUFFER SYSTEMS AND ENZYME STAINING SYSTEMS ..................81
VITA ............................................................................................................................................88
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I
LIST OF TABLES
2.1. Mycelial growth and production of microconidia of orange mutants of Fusarium oxysporum f . sp. lycopersici andwild-type c o n tro ls ............................................................................. 22
2.2. Pathogenicity of orange mutants of Fusarium oxysporum f. sp. lycopersici and wild-type controls .................................................. 25
2.3. Evaluation of orange mutants of Fusarium oxysporum for sectoring following serial transfers on potatodextrose a g a r ..................................................................................... 26
2.4. Evaluation of orange mutants of Fusarium oxysporum for sectoring following serial transfers on 10% potatodextrose a g a r ..................................................................................... 27
3.1. Strains of Fusarium oxysporum used in the present studyand their designation by vegetative compatibility group ............. 40
3.2. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of £. oxysporum formembers of VCG 2028 ................................................................... 44
3.3. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of £. oxysporum formembers of VCG 2035 .................................................................... 45
3.4. Relative competitive infection of nonpathogenic Fusarium oxysporum isolated from tomato ro o ts ........................................... 46
3.5. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of E. oxysporum formembers of VCG 2050 ................................................................... 47
3.6. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of E. oxysporum formembers of VCG 2061 ................................................................... 48
4.1. Strains of Fusarium oxysporum used in the present study andtheir designation by vegetative compatibility group .................... 62
4.2. Enzymes, abbreviations, Enzyme Commission (E.C.) numbersand buffer systems used in this study ........................................... 64
iv
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4.3. Putative allele distribution for 15 putative enzyme loci in 36 isolates of Eusarium oxysporum for symptomless tomato ro o ts .....................................................................
v
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LIST OF FIGURES
2.1. Orange mutant (ORA-21) of Fusarium oxvsporum f. sp. lycppersici compared to wild-type Fusarium oxysporum
f. sp. lycopersici (LSU 3) (d) on (a) potato dextrose,(b) water, and (c) cornmeal agars .................................................. 23
2.2. Orange mutant (ORA-22) of Fusarium oxysporum f . sp. lycopersici compared to wild-type Fusarium oxysporum f. sp. lycopersici (LSU 3) (d) on (a) potato dextrose,
(b) water, and (c) cornmeal agars .................................................. 24
2.3. Orange mutants of Fusarium oxysporum f. sp. lycopersici and nonpathogenic £. oxysporum emerging from tomato roots on Komada's m edium ............................................................................. 30
3.1. Location of sites samples in Louisiana for nonpathogenic strainsof Fusarium oxysporum ................................................................... 38
3.2. Rate of infection by an orange mutant (ORA-22) of Fusarium oxysporum f. sp. lycopersici in the presence of nonpathogenic isolates of £. oxysporum in all VCGs ............................................. 49
4.1. Principle components analysis of isozyme polymorphisms innonpathogenic populations of Fusarium oxysporum .................... 68
vi
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ABSTRACT
Race 1 isolates collected from tomato roots were used to develop an
orange mutant of Fusarium oxysporum f. sp. lycopersici (FPL) for use in
competitive infection tests against nonpathogenic £. oxvsporum isolates. Eighty
one color mutants were induced by exposure to ultraviolet light. The mutant ORA-
22 retained pathogenicity and growth habit similar to the wild-type.
Preliminary competitive infection tests indicated differences within the
nonpathogenic population in the ability to suppress or enhance infection by FPL
orange mutant ORA-22. Four vegetative compatibility groups (VCGs) were tested
to determine if competitive infection ability was associated with VCG designation.
Results from these tests revealed a wide range of effectiveness, ranging from no
effect to suppression or enhancement of root infection by the pathogen, FPL. All
members of a VCG showed the same reaction. The results suggest that
competitive infection ability and VCG are closely related traits. Isozyme analysis
by starch gel electrophoresis was used to estimate genetic diversity within and
among the four VCGs. Principal components analysis of the results showed that
each population was unique and clearly separated from the pathogenic controls.
These results provide strong evidence that the genetic traits associated with
competitive infection ability are confined to genetically isolated populations of
nonpathogenic E. oxvsporum as delimited by VCG.
vii
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CHAPTER 1
REVIEW OF LITERATURE
1
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I
2
Fusarium oxysporum (Schlect.) Snyd. & Hans, is a soilborne fungus
which includes strains that cause vascular wilts of numerous cultivated
plant species including vegetables, flowers, herbaceous perennial
ornamentals, and plantation crops (1.1). Infection also has been reported
on noncultivated species (1.4, 1.7,1.10, 1.16, 1.20). The pathogen is
worldwide in distribution, and it is the most frequently isolated of all
Fusarium species in agricultural and nonagricultural soils (1.12). It may
exist as a saprophyte, parasite, or pathogen (1.10, 1.12, 1.32). The
fungus produces chlamydospores which allow it to persist in soils for many
years without a susceptible host (1.10). Agricultural soils may contain
between 103 and 105 propagules of £. oxysporum per gram (1.12).
Tomato (Lycopersicon esculentum L. Mill.) is one of the most widely
grown vegetable crops worldwide (1.19, 1.35). Fusarium w ilt, caused by
Fusarium oxysporum (Schlect.) f. sp. lycopersici (Sacc.) Snyder & Hansen
(EQL), is a recurring and devastating disease of tomato that has been
reported in at least 32 countries (1.19). It is particularly serious because of
the development of new races of the pathogen (1.14, 1.19, 1.21, 1.34).
There are three known races of FPL that are distinguished by their
pathogenicity to cultivars with specific dominant genes for resistance
(1.24). Race 1 was first described in 1886 (1.9), and race 2 was initially
reported in 1945 but did not cause serious crop damage until 1961 in
Florida (1.31). Race 3 was reported in Australia in 1978 (1.17) and was
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found in Florida in 1982 (1.34) and California in 1987 (1.14). Race 3 must
now be considered a major threat to the tomato industry because of limited
sources of resistance to this race (1.34) and the time required to
incorporate resistance into horticulturally acceptable cultivars.
Control of Fusarium wilts is limited to the use of resistant varieties,
cultural practices, and soil fumigation (1.1, 1.30). Soil fumigation has been
used with success, but it is expensive and the effect does not last long.
As costs of petrochemicals rise and the environmental effects of these
pesticides are elucidated, use of soil fumigation will probably have to be
abandoned. Cultural practices effective in reducing pathogen populations
include deep plowing, crop rotation, leaving the soil fallow, and the flooding
of fields (1.1). For greenhouse crops, soil sterilization and sanitation are
effective control measures. When available, the use of resistant varieties is
the most desirable and effective means of control.
Drawing momentum from the growing public concern regarding the
widespread use of hazardous chemicals in disease control, biological control
of plant pathogens has recently received considerable attention throughout
the world (1.2, 1.3, 1.6, 1.7, 1.11, 1.12, 1.23, 1.25, 1.26 1.27, 1.29,
1.36). Biological control is defined as the total or partial destruction of
pathogen populations by other organisms; or the use by man of an
organism for pathogen control (1.1, 1.12). Cook and Baker (1.12) listed
three general approaches to biological control of plant pathogens: (i)
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control of pathogen inoculum, (ii) protection against infection, and (iii)
cross-protection or induced resistance. Mechanisms of biological control by
antagonists are antibiosis, competition, and parasitism (1.11, 1.12). The
form of biological control which has been the most successful against
formae species of £. oxysporum is competition. Competition occurs when
two or more organisms require the same resource and the use of that
resource by one reduces the amount available to the other (1.11).
Disease suppressive soils are defined as those soils in which disease
development is suppressed even though the pathogen and a susceptible
host are present (1.30). Examples of soils suppressive to Fusarium wilts
have been found in California, Florida, and the Chateaurenard region in
France (1.3, 1.23, 1.29, 1.33). Toussoun (1.33) showed that some soils
are suppressive to pathogenic formae speciales, but not to nonpathogenic
populations of E. oxysporum. Alabouvette et al. (1.3) considered soil to be
a living entity which manifests a certain resistance to infestation and to the
expression of the pathogenic capabilities of an organism. Using E.
oxysporum f. sp. melonis (FOM). the causal agent of Fusarium w ilt of
muskmelon, they showed that soil suppressiveness to FOM could be
transferred to other soils and that chlamydospore germination was lowered
in these suppressive soils. They also concluded that nonpathogenic strains
of E. oxysporum and E. solani were the organisms responsible for soil
suppressiveness in soils in the Chateaurenard region in France. They
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5
proposed that the mechanism of suppressiveness to Fusarium w ilt of
muskmelon involved competition for the same ecological niche between the
pathogenic forma and saprophytic strains of £. oxysporum. Schneider,
working with celery, (1.29) was the first to demonstrate that some
nonpathogenic, parasitic strains of £. oxysporum predisposed plant roots to
infection by the pathogenic forma, £. a. f. sp. apii. while others
competitively suppressed infection. Furthermore, he provided evidence for
and concluded that naturally-occurring disease suppression was caused by
relatively high populations of effective, nonpathogenic root-infecting strains
of £. oxysporum. Because the pathogen is morphologically
indistinguishable from the competitors, Schneider used a pigmented mutant
of the pathogen in his investigations (1.29). Colonies growing from the
roots were easily differentiated on the basis of pigmentation. Larkin et al.
(1.22) reported the development of a soil suppressive to Fusarium w ilt of
watermelon, Fusarium oxysporum f. sp. niveum. which was induced by
monoculture to the moderately resistant Crimson Sweet cultivar. A
population of nonpathogenic £. oxysporum as well as bacteria,
actinomycetes, and fluorescent pseudomonads were present in this
suppressive soil which were not present in the conducive soils. Paulitz,
Park and Baker (1.27) isolated nonpathogenic strains of £. oxysporum from
symptomless surface-sterilized cucumber roots. They showed that some of
these isolates were effective while others were ineffective in reducing the
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rate of infection by the pathogen. They found one isolate which
significantly reduced the rate of infection by the pathogen, £. £. f. sp.
cucumerinum (FOCI, in raw soil. Park et al. (1.26) later showed that
nonpathogenic isolates of £. oxysporum and fluorescent pseudomonads,
which are ineffective alone, induced suppressiveness against FOC when
used in combination. Based on the work of Schneider (1.29) and Baker
(1.5), Alabouvette (1.2) reassessed his suppressive isolates and compared
them for saprophytic and parasitic competitive effectiveness. He found
that some isolates were saprophytically effective, while others were
effective parasitically, there being no correlation between the two.
Cross-protection is a form of biological control in which a biocontrol
agent induces resistance in a host rather than being directly antagonistic to
the pathogen. Resistance to a pathogen may be induced by the previous
inoculation of a plant with an incompatible race of the pathogen or
nonpathogenic form of the fungus. However, it should be noted that cross
protection is generally achieved following direct inoculation of the
susceptible plant organ with extremely high inoculum levels and is short
lived (1.8, 1.36). Ogawa and Komada (1.25) used £. oxysporum to pre
inoculate sweet-potato cuttings. They found that these inoculated plants
were protected from soilborne inoculum of £. £. f. sp. batatas as well as
that transmitted from infected roots. Biles and Martyn (1.8) pre-inoculated
watermelon seedlings with either FPL or avirulent races of £. q. niveum 24
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or 72 hr prior to challenge with a virulent race of £. £>. f. sp. niveum. All
treatments significantly reduced w ilt symptoms, but pre-inoculation with
avirulent races of £. q . niveum induced a higher level of resistance than the
other treatments.
Nonpathogenic strains of £. oxysporum. which survive in soil as
saprophytes and parasites, constitute the largest proportion of the soilborne
population (1.10, 1.33). These highly competitive saprophytes are able to
utilize a wide variety of organic substrates, including cellulose, pectin,
lignin, and other complex materials (1.11). Currently, nonpathogenic
saprophytes and parasites are included in a single taxonomic group because
they are morphologically indistinguishable from each other and from
pathogenic strains of £. oxysporum. Both pathogenic and nonpathogenic
strains of £. oxysporum are known to infect roots of weeds and other
nonsusceptible hosts, including cultivated and noncultivated species (1.4,
1.7, 1.10, 1.16, 1.18, 1.20).
Until recently, the role of nonpathogenic strains has been largely
ignored, probably because of the difficulties involved in identification. In
1983, Puhalla (1.28) developed a technique to assign isolates of £.
oxysporum to vegetative compatibility (heterokaryon) groups (VCG) using
nitrate metabolism (nil) mutants. When two different n il genotypes are
paired on minimal medium, complementation may occur. Complementation
is demonstrated by the formation of a dense aerial mycelium at the
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interface of the two colonies. Heterokaryon formation occurs when the
tw o o il mutants have identical alleles at all vegetative compatibility loci.
Heterokaryons or vegetatively compatible isolates are known to be closely
related if not clonal derivatives (1.15, 1.28). Correll, Puhalla and Schneider
(1.13) showed that VCG could be used to separate populations of
nonpathogenic root-infecting strains of £. oxysporum from celery roots. In
a more detailed study, Elias, Schneider and Lear (1.15) conducted a large
survey and VCG analysis of nonpathogenic isolates of £. oxysporum from
tomato roots collected from eight sites in Louisiana and found a more
diverse population than that of celery. Isolates within a VCG were not
vegetatively compatible with isolates from other VCGs or pathogenic
isolates of FPL.
A primary conclusion to be drawn from the results discussed above
is that the population of nonpathogenic strains of £. oxysporum associated
with tomato is quite diverse. It was hypothesized that if certain segments
of the nonpathogenic population of £. oxysporum can effectively compete
with the pathogenic forma for the same ecological niche, then it could lead
to the reduction or suppression of infection and disease severity, a form of
biological control by antagonism. The objectives of this study were to (i)
determine the influence of nonpathogenic strains of £. oxysporum on
tomato root infection by the pathogen, £. q. f. sp. lycopersici: (ii) to use
vegetative compatibility groups (VCGs) as a qualitative measure of genetic
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diversity within the nonpathogenic population; and (iii) to obtain
quantitative measures of genetic diversity within and among VCGs (clonal
populations) of nonpathogenic strains of £. oxysporum.
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10
Literature Cited in Chapter 1
1.1. Agrios, G. N. 1988. Plant Pathology. 3rd ed. Academic Press, San Diego. 803 pp.
1.2. Alabouvette, C. 1990. Biological control of Fusarium w ilt pathogens in suppressive soils. Pages 27-43 in: Biological Control of Soil-borne Pathogens. D. Hornsby, ed. CAB International, United Kingdom.
1.3. Alabouvette, C., F. Rouxel, and J. Louvet. 1979. Characteristics of Fusarium w ilt suppressive soils and prospects for their utilization in biological control. Pages 165-182 in: Soil-borne Plant Pathogens.B. Schippers and W. Gams, eds. Academic Press, London. 686 pp.
1.4. Armstrong, G. M., and J. K. Armstrong. 1948. Nonsusceptible hosts as carriers of w ilt fusaria. Phytopathology 38:808-826.
1.5. Baker, R. 1980. Measures to control Fusarium and Phialophora w ilt pathogens of carnation. Plant Dis. 64:743-749.
1.6. Baker, R., P. Hanchey, and S. D. Dottarar. 1978. Protection of carnation against Fusarium stem rot by fungi. Phytopathology 68:1495-1501.
1.7. Beckman, C. H. 1987. The Nature of Wilt Diseases in Plants. American Phytopathology Press, St. Paul. 175 pp.
1.8. Biles, C. L., and R. D. Martyn. 1989. Local and systemic resistance induced in watermelons by formae speciales of Fusarium oxysporum. Phytopathology 79:856-860.
1.9. Booth, C. 1971. The Genus Fusarium. Commonwealth Mycological Institute, Kew, Surrey, England. 237 pp.
1.10. Burgess, L. W. 1981. General ecology of the Fusaria. Pages 225- 235 in Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. The Pennsylvania State University Press, University Park.
1.11. Campbell, R. 1989. Biological control of microbial plant pathogens. Cambridge University Press, Cambridge. 218 pp.
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1.12. Cook, R. J., and K. F. Baker. 1983. The Nature and Practice of Biological Control of Plant Pathogens. The American Phytopathological Society, St. Paul. 539 pp.
1.13. Correll, J. C., J. E. Puhalla and R. W. Schneider. 1986.Identification of Fusarium oxysporum f . sp. a p ii on the basis of colony size, virulence, and vegetative compatibility. Phytopathology 76:396-400.
1.14. Davis, R. M., K. A. Kimble and J. J. Farrar. 1988. A third race of Fusarium oxysporum f. sp. lycopersici identified in California. Plant Dis. 72:453.
1.15. Elias, K. S., R. W. Schneider, and M. M. Lear. 1991. Analysis of vegetative compatibility groups in nonpathogenic populations of Fusarium oxysporum isolated from symptomless tomato roots. Can. J. Bot. 69:2089-2094.
1.16. Gordon, T. R., D. Okamoto, and D. J. Jacobsen. 1989.Colonization of muskmelon and nonsusceptible crops by Fusarium oxysporum f. sp. melonis and other species of Fusarium. Phytopathology 79:1095-1100.
1.17 Grattidge, R., and R. G. O'Brien. 1982. Occurrence of a third race of Fusarium w ilt of tomatoes in Queensland. Plant Dis. 66:165- 166.
1.18. Hendrix, D. L. and L. W. Nielsen. 1958. Invasion and infection of crops other than the forma suscept by Fusarium oxysporum f. sp. batatas and other formae. Phytopathology 48:224-228.
1.19. Jones, J. P., and S. S. Woltz. 1981. Fusarium-incited diseases of tomato and potato and their control. Pages 157-168 in: Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. The Pennsylvania State University Press, University Park.
1.20. Katan, J. 1971. Symptomless carriers of the tomato Fusarium w ilt pathogen. Phytopathology 61:1213-1217.
1.21. Katan, J., and R. Ausher. 1974. Distribution of race 2 Fusarium oxysporum f. sp. lycopersici in tomato fields in Israel.Phytoparasitica 2:83-90.
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1.22. Larkin, R. P., D. L. Hopkins, and F. N. Martin. 1987. Cultivar- specific induction of soil suppressiveness to Fusarium w ilt of watermelon. Phytopathology 77:607-611.
1.23. Louvet, J., F. Rouxel, and C. Alabouvette. 1976. Recherches sur la resistance des sols aux maladies. I. Mise en evidence de la nature microbiologique de la resistance d'un sol au developpement de la fusariose vasculaire du melon. Ann. Phytopathol. 8:425-436.
1.24. McGrath, D. J., D. Gillespie, and L. Vawdrey. 1987. Inheritance of resistance to Fusarium oxysporum f. sp. lycopersici races 2 & 3 in Ivcopersicon pennelli. Aust. J. Agric. Res. 38:729-733.
1.25. Ogawa, K. and H. Komada. 1985. Biological control of Fusarium w ilt w ith cross-protection by nonpathogenic Fusarium oxysporum. Pages 121-123 in: Ecology and Management of Soilborne Plant Pathogens. C. A. Parker, A. D. Rovira, K. J. Moore and P. T. W. Wong, eds. The American Phytopathological Society, St. Paul.
1.26. Park, C. S., T. C. Paulitz, and R. Baker. 1988. Biocontrol of Fusarium wilt of cucumber resulting from interactions between Pseudomonas putida and nonpathogenic isolates of Fusarium oxysporum. Phytopathology 78:190-194.
1.27. Paulitz, T. C., C. S. Park, and R. Baker. 1987. Biological control of Fusarium w ilt of cucumber with nonpathogenic isolates of Fusarium oxysporum. Can. J. Microbiol. 33:349-353.
1.28. Puhalla, J. E. 1985. Classification of strains of Fusarium oxysporum on the basis of vegetative compatibility. Can. J. Bot. 63:179-183.
1.29. Schneider, R. W. 1984. Effects of nonpathogenic strains of Fusarium oxysporum on celery root infection by Fusarium oxysporum f. sp. apii and a novel use of the Lineweaver-Burk double reciprocal plot technique. Phytopathology 74:646-653
1.30. Schneider, R. W., and D. M. Huber 1982. Suppressive Soils and Plant Disease. The American Phytopathological Society, St. Paul.88 pp.
1.31. Stall, R. 1961. Development of Fusarium w ilt on resistant varieties of tomato caused by a strain different from race 1 isolates of Eusarium oxysporum f. lycopersici. Plant Dis. Reptr. 45:12-15.
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1.32. Stoner, M. F. 1981. Ecology of Fusarium in noncultivated soils. Pages 276-286 in: Fusarium: Diseases, Biology and Taxonomy. P.E. Nelson, T. A. Toussoun, and R. J. Cook, eds. The Pennsylvania State University Press, University Park.
1.33. Toussoun, T. A. 1975. Fusarium-suppressive soils. Pages 145-151 in: Biology and Control of Soil-Borne Plant Pathogens. G. W.Bruehl, ed. American Phytopathological Society, St. Paul. 216 pp.
1.34. Volin, R. B., and J. P. Jones. 1982. A new race of Fusarium w ilt of tomato in Florida and sources of resistance. Proc. Fla. State Hort. Soc. 95:268-270.
1.35. Walker, J. C. 1971. Fusarium Wilt of Tomato. Monograph No. 6. The American Phytopathological Society, St. Paul. 56 pp.
1.36. Wymore, L. A., and R. Baker. 1982. Factors affecting cross protection in control of Fusarium w ilt of tomato. Plant Dis. 6:908- 910.
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CHAPTER 2
SELECTION OF AN ORANGE MUTANT OF FUSARIUM OXYSPORUMF. SP. LYCOPERSICI
14
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15
Introduction
Fusarium oxysporum is a soilborne fungus which includes strains that
cause vascular wilts of a wide variety of crop plants worldwide (2.12).
Most isolates from soil are nonpathogenic and exist as saprophytes or
parasites (2.2). Strains of E. oxysporum. including pathogens and
nonpathogens, are generally morphologically indistinguishable.
Nonpathogens have been largely ignored because of the difficulty in
identifying strains even though they are known to interact with pathogenic
strains (2.2). In order to conduct ecological studies, it is necessary to be
able to recognize and quantify populations of introduced strains relative to
other populations of E. oxysporum.
Ultraviolet irradiation of fungi may be used to induce color mutants
(2.6, 2.9, 2.10) as well as mutants which are resistant to fungicides such
as benomyl. Color mutants are advantageous as compared to benomyl
resistant mutants because, following selection and preliminary screenings,
they are well adapted to surviving in the soil and they can be observed
together with the pathogen on the sane plate of selective media. Therefore,
in studies involving introduced strains, these mutants can be used to
provide a fast and accurate means of identification and separation of the
nonpathogenic and pathogenic populations of E. oxysporum. They can then
be used to investigate interactions between the pathogenic and
nonpathogenic populations within the rhizosphere.
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16
The objective of this study was to induce pigmented mutants and
select and test selected mutants of race 1 £. oxysporum f. sp. lycopersici
for use in subsequent studies.
Materials and Methods
Mutagenesis and selection of orange mutants. In order to quantitatively
monitor root infection by the pathogen, £. a. f. sp. lycopersici. pigmented
mutants were sought which could be readily distinguished from
nonpathogens on Komada's agar medium (2.4), which is selective for £.
oxysporum. Pathogenic orange mutants of FPL were selected by irradiating
the following race 1 isolates using a modification of Puhalla's method (2.9):
PS-1, BFOL-54, BFOL-56, BFOL-67, LSU-3, LSU-4, LSU-5, and LSU-6.
Isolates were plated on minimal medium (MM) or potato dextrose agar
(PDA) (Appendix A) and incubated for 5-10 days at room temperature. Ten
ml of sterile, distilled water were pipetted onto the agar surface, and the
cultures were scraped with a flame-sterilized bent glass rod. The resulting
conidial suspension was filtered first through sterile cheesecloth into a
sterile beaker to remove pieces of mycelium and then through a 1.0 //m
mesh screen to separate macroconidia and chlamydospores from
microconidia. The microconidia were counted with a hemacytometer,
diluted to 104 per ml with sterile, distilled water, poured into petri dishes
containing a magnetic stir bar, and placed on a magnetic stir plate for
agitation. The plates were irradiated for 70 sec using a short-wave
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17
ultraviolet lamp (4 watts) placed 14 cm above the uncovered stir plate in a
darkened room. These parameters were determined previously by
constructing a kill curve and selecting distance and time to give 99% kill
(2.9). After irradiation, all work was performed in darkness. Irradiated
microconidia were plated onto MM at a rate of 30 to 300 colony forming
units per plate. The plates were wrapped in aluminum foil in groups of 10
and incubated for 7-10 days at room temperature. Orange colored mutants
were selected, single-spored, and stored on silica gel at 4 C (2.8).
Inoculum preparation. Orange mutant cultures were grown in PDB on a
rotary shaker for 72 hr at room temperature. One hundred grams of finely
ground corncob grit (Grit O'Cob, Nebraska) in 250-ml Erlenmeyer flasks
were moistened with 10 ml 0.025M L-asparagine, autoclaved for 1 hr on
each of tw o consecutive days, inoculated with a conidial suspension (106 /
ml) obtained from the PDB cultures, and incubated for 2 wk at room
temperature. The ground corncob cultures, hereafter referred to as
inoculum, were dried at room temperature in 100mm by 80mm deep petri
plates covered with cheesecloth, ground with a mortar and pestle, and
refrigerated until used.
Pathogenicity of orange mutants. Greenhouse pathogenicity tests and race
determinations were performed using the orange mutant isolates and
nonmutagenized controls. The tomato cultivars 'Fantastic' (susceptible to
races 1, 2, and 3); 'Supersonic' (resistant to race 1); and 'Walter' (resistant
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to races 1 and 2) were used as hosts. Fungal strains were grown in
Czapek's solution for 5 days on an orbital shaker at room temperature. The
cultures were filtered through cheesecloth and the resulting spore
suspension was adjusted to about 106 spores per ml. Seedlings were
grown in sterile, commercially prepared potting soil mix for 2 wk until the
first true leaves emerged. The root dip method of inoculation was used
(2.13). Seedlings were gently uprooted, and roots were pruned to about 3
cm in length. Six seedlings per cultivar were dipped into spore suspensions
of each strain for 30 sec and transplanted to plastic cell trays pre-filled with
soil-peat moss mix (50:50, v:v) at the rate of one seedling per cell. Two
controls were used: seedlings with pruned roots were dipped in either
sterile water or inoculum of a race 1 FPL isolate. Disease symptoms were
recorded 10-14 days after inoculation. Pathogenicity tests using the
orange mutant isolates were conducted three times.
Phenotypic tests. Tests were performed using orange mutant isolates to
compare production of microconidia, colony growth and morphology, and
reversion to wild-type. Production of microconidia was determined by
growing orange mutant isolates in potato dextrose broth (PDB) at room
temperature on an orbital shaker for 36 hr. At that time, numbers of
conidia per ml broth were determined with a hemacytometer. Serial transfer
tests were performed using 26 single-spored orange mutant isolates plated
on full strength and 10% PDA and mass transferred weekly to test for
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19
reversion of mutants. Appearance of wild-type sectors was taken as
presumptive evidence for reversion. Radial growth of orange mutants and
wild-type FPL was measured at 16 and 24 C on full strength potato
dextrose, cornmeal and water agars for 5 days.
Inoculum density tests. Preliminary experiments were performed to
determine the appropriate amount of inoculum to incorporate into soil for
competitive infection experiments. The objective was to determine the
amount of inoculum to add to soil to give 50% of the maximum attainable
root infection measured as infections per 100 cm root length. In this way,
both increases and decreases in root infection could be determined. One kg
of sterile soil was amended with 0.25, 0.50, 0.75, or 1.0 g of orange
mutant inoculum, blended thoroughly in a large plastic bag, and dispensed
into 10-cm clay pots. Tomato seedlings, cultivar 'Supersonic', were
transplanted into the pots and grown for 4 wk in the greenhouse. Also
included were a noninoculated control and a noninoculated, sterilized
corncob grit control. At harvest, the plants were removed from the pots,
immersed in water, and the soil was carefully washed from the roots. The
roots were surface sterilized for 4 min in 0.21 % household bleach (2.10),
rinsed in three changes of sterile water, plated on Komada’s medium (2.4),
and incubated at room temperature for 1 wk. The number of orange
colonies was determined for each plate. Root lengths on each plate were
estimated using the line intersect grid method (2.7, 2.11). The number of
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orange colonies and root lengths were used to calculate the number of
colonies per 100 cm of root (2.10). Briefly, plates with roots were placed
on a grid of known line length. The number of root-line intersections was
determined, and the root length was estimated by the following
equation:
7i N AR = ----------
2 H
where R = root length, N = number of intersections, A = area of the grid,
and H = grid line length.
Results
Mutagenesis and selection of orange mutants. Eighty one orange
mutant isolates were obtained. Forty orange mutants were recovered from
isolate LSU-4, 14 from BFOL-67, and 17 from LSU-3. These three wild-type
isolates were all race 1 of FPL. Isolates PS-1, BFOL-54, BFOL-56, LSU-5,
and LSU-6 did not produce any orange mutants. Several yellow, pink, and
purple mutants were generated from these isolates. Orange mutants
selected for final studies had a vigorous growth habit and were medium to
deep orange in color.
Phenotypic tests
Mycelial growth on PDA at 16 and 24 C. A total of 26 mutant isolates and
three controls were grown on PDA at 16 and 24 C. Generally, there was a
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wide range of colony morphology with most orange mutants having a less
vigorous mycelial growth as compared to the wild type controls, LSU-4,
LSU-3, and BFOL-67, from which they were derived (Table 2.1). Isolates
ORA-6, ORA-21, ORA-22, ORA-23, ORA-24, ORA-25, and ORA-26 had
mycelial growth most comparable to that of the controls (Figures 2.1 and
2.2). Measurements for the orange mutants are significantly different from
the parents.
Pathogenicity of orange mutant isolates. Determination of
pathogenicity in most isolates was straightforward, in that all or none of a
particular cultivar died within 10-14 days after inoculation. The isolates
were variable in pathogenicity. Four of the 27 orange mutant isolates (ORA-
21, ORA-22, ORA-24, ORA-25) were determined to be virulent race 1
pathogens (Table 2.2). All other mutants were nonpathogenic.
Serial transfer studies. Isolates ORA-1 through ORA-20 were subjected to
14 weekly transfers onto PDA and 10% PDA, and isolates ORA-21 through
ORA-26 were subjected to 10 weekly transfers onto PDA and 10% PDA
(Tables 2.3 and 2.4). The rate of sectoring of the isolates was low. In
addition, single-spores were transferred at random from these plates in an
effort to detect changes in color or growth habit. No sectoring or mutation
was observed.
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Table 2.1. Mycelial growth and production of microconidia of orange mutants of Fusarium oxysporum f. sp. lycopersici and wild-type controls.
Isolate Colony diameter (cm)A 16C 24C
microconidia/mlB
ora-1 3.4 4.1 NDCora-2 2.6 3.8 NDora-3 2.8 4.2 NDora-4 2.0 3.6 NDora-5 3.8 7.3 NDora-6 5.0 8.0 NDora-7 2.8 4.4 NDora-8 2.4 4.2 NDora-9 2.5 4.5 NDora-10 2.6 4.4 NDora-11 2.9 4.2 NDora-12 2.8 4.0 NDora-13 2.9 4.3 NDora-14 2.8 4.4 NDora-15 2.8 3.8 NDora-16 2.6 4.0 NDora-17 2.8 4.0 NDora-18 2.8 4.4 NDora-19 2.8 3.8 NDora-20 2.7 4.5 NDora-21 3.5 7.3 8.49/1 O'ora-22 4.5 7.6 8.83/10'ora-23 4.7 7.5 NDora-24 4.0 7.6 NDora-25 5.0 8.0 1.84/10ora-26 4.7 8.0 NDLSU-4 4.4 7.9 NDLSU-3 4.8 7.5 2.19/10BFOL-67 4.9 8.0 ND
Agrown on potato dextrose agar.BPDB cultures inoculated with 10 ml of inoculum and incubated for 48 hrs. cnot determined.
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Figure 2.1. Orange mutant (ORA-21) of Fusarium oxysporum f. sp. lycopersici compared to wild-type Fusarium oxysporum f. sp. lycopersici (LSU 3)(d) on (a) potato dextrose, (b) water, and (c) cornmeal agars.
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Figure 2.2. Orange mutant (ORA-22) of Fusarium oxysporum f. sp. lycopersici compared to wild-type Fusarium oxysporum f. sp. I.ycppersisi (LSU 3)(d) on (a) potato dextrose, (b) water, and (c) cornmeal agars.
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Table 2.2. Pathogenicity of orange mutants of Fusarium oxysporum f. sp. lycopersici and wild type controls.
Isolate PathogenicityA test results
Origin6
ora-1 0 LSU-4ora-2 0 LSU-4ora-3 0 LSU-4ora-4 0 LSU-4ora-5 0 LSU-4ora-6 0 LSU-4ora-7 0 LSU-4ora-8 0 LSU-4ora-9 0 LSU-4ora-10 0 LSU-4ora-11 0 LSU-4ora-12 0 LSU-4ora-13 0 LSU-4ora-14 0 LSU-4ora-15 0 LSU-4ora-16 0 LSU-4ora-17 0 LSU-4ora-18 0 LSU-4ora-19 0 LSU-4ora-20 0 LSU-4ora-21 6 LSU-3ora-22 6 LSU-3ora-23 0 BFOL-67ora-24 6 BFOL-67ora-25 6 LSU-3ora-26 0 BFOL-67LSU-4 6LSU-3 6BFOL-67 0
A Number of plants wilted or dead after 10 days.B LSU-3 and LSU-4 were isolated from Plaquemines Parish, LA, and BFOL-
67 was isolated from Deltaville, MS.
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Table 2.3. Evaluation of orange mutants of Fusarium oxysporum for sectoring following serial transfers on potato dextrose agar.
Isolate No. of transfers No. of transfers at which sectors appearedA
ora-1 14 NSora-2 14 NSora-3 14 NSora-4 14 5ora-5 14 NSora-6 14 NSora-7 14 NSora-8 14 2ora-9 14 NSora-10 14 NSora-11 14 NSora-12 14 NSora-13 14 NSora-14 14 NSora-15 14 NSora-16 14 NSora-17 14 3ora-18 14 NSora-19 14 NSora-20 14 NSora-21 10 NSora-22 10 NSora-23 10 NSora-24 10 NSora-25 10 NSora-26 10 NS
ANo sectors were observed during the course of this study.
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Table 2.4. Evaluation of orange mutants of Fusarium oxysporum for sectoring following serial transfers on 10% potato dextrose agar.
Isolate No. of transfers No. of transfers at which Asectors appeared
ora-1 14 2Bora-2 14 NSora-3 14 NSora-4 14 NSora-5 14 11ora-6 14 NSora-7 14 NSora-8 14 NSora-9 14 NSora-10 14 NSora-11 14 NSora-12 14 NSora-13 14 NSora-14 14 NSora-15 14 NSora-16 14 NSora-17 14. NSora-18 14 NSora-19 14 NSora-20 14 NSora-21 10 NSora-22 10 NSora-23 10 NSora-24 10 NSora-25 10 NSora-26 10 NS
AAII isolates are orange colored except those noted with asterisks which are purple.
BNo sectors were observed during the course of this study.
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28
Discussion
The process of secondary metabolism in fungi results in the
production of metabolites with no obvious chemical function in the
organism (2.3). Examples of secondary metabolites produced by fungi
include penicillin, aflatoxins, carotenoids such as P-carotene and
xanthophylls. Carotenoids are lipid compounds and may be colorless or
pigmented yellow, orange, red or purple. In vivo, they are located in
lipophilic, hydrophobic regions in the cell and in association with protein in
membranes(2.1). In fungi, carotenoids function in photoreception and
photoprotection. In addition, p-carotene is a precursor to trisporic acid,
which controls gametogenesis in the fungus Blakeslea trispora (2.5).
Orange mutants have been previously used in ecological studies with
£. oxysporum (2.6, 2.10). Orange mutants, as compared to a drug
(benomyl) resistant mutants, allow for the use of a colored pathogen in
coinoculation studies because the mutant can be separated from
nonpathogenic £. oxysporum and other soil fungi by the use of Komada's
medium (2.4), which is selective for Fusarium spp. Pathogens can be
separated from nonpathogens on the same petri dish by the orange
pigmentation.
Nagao and Hirano (2.6) looked at pathogenicity, morphological
features, and survival in soil of UV-irradiated orange mutants of £. a . f. sp.
cucumerinum (FO_C). They concluded that their mutants retained the
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29
features and behaviors of wild-type FOC. The studies described herein and
those conducted previously (2.6, 2.10) show conclusively that
pigmentation is a valid marker for use in ecological studies. A total of
eighty one orange mutant isolates were obtained from UV irradiation of £.
oxysporum f. sp. lycopersici race 1 isolates. In addition, yellow, pink and
purple isolates were obtained. Isolate ORA-22 was selected from the
collection because of its similarity to the wild-type in growth habit and
pathogenicity as well as its deep orange coloration. An example is shown
in Figure 2.3.
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Figure 2.3. Orange mutants of Fusarium oxysporum f. sp. lycopersici and nonpathogenic £. oxysporum emerging from tomato roots on Komada's medium.
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31
2 .1.
2.2.
2.3.
2.4.
2.5.
2.6.
2.7.
2.8.
2.9.
2 .10.
2 .11.
Literature Cited in Chapter 2
Britton, G. 1971. The Biochemistry of Natural Pigments.Cambridge University Press, Cambridge. 366 pp.
Burgess, L. W. 1981. General ecology of the Fusaria. Pages 225- 235 in Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. The Pennsylvania State University Press, University Park.
Garroway, M. 0 ., and R. C. Evans. 1984. Fungal Nutrition and Physiology. John Wiley & Sons, New York. 401 pp.
Komada, H. 1975. Development of a selective medium for quantitative isolation of Fusarium oxysporum from natural soil. Rev. Plant Protection Res. 8:114-124.
Krinsky, N. I. 1971. Chapter X. Functions. Pages 669-716 in: Carotenoids. 0. Isler, ed. Birkhauser Verlag, Basel.
Nagao, H. and K. Hirano. 1990. Survival and pathogenicity of the orange mutant of Fusarium oxysporum f. sp. cucumerinum. Ann. Phytopath. Soc. Japan 56:185-193.
Newman, E. I. 1966. A method of estimating the total length of root in a sample. J. Appl. Ecol. 3:139-145.
Perkins, D. D. 1962. Preservation of Neurospora stock cultures with anhydrous silica gel. Can J. Microbiol. 8:591-594.
Puhalla, J. E. 1984. A visual indicator of heterokaryosis in Fusarium oxysporum from celery. Can. J. Bot. 62:540-545.
Schneider, R. W. 1984. Effects of nonpathogenic strains of Fusarium oxysporum on celery root infection by Fusarium oxysporum f. sp. apii and a novel use of the Lineweaver-Burk double reciprocal plot technique. Phytopathology 74:646-653.
Torssell, W. R., J. E. Begg, C. W. Rose, and G. F. Byrne. 1968. Stand morphology of Townsville lucerne (Stylosanthes humilis). Seasonal growth and root development. Aust. J. Exp. Agric. Anim. Hub. 8:532-543.
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32
2.12. Toussoun, T. A. 1975. Fusarium-suppressive soils. Pages 145-151 in: Biology and Control of Soil-Borne Plant Pathogens. G. W.Bruehl, ed. American Phytopathological Society, St. Paul.
2.13. Williams, P. H. 1981. Fusarium yellows. Pages 124-129 in: Screening Crucifers for Multiple Disease Resistance. P. H. Williams, ed. University of Wisconsin Press, Madison.
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CHAPTER 3
COMPETITIVE INFECTION STUDIES BETWEEN PATHOGENIC AND NONPATHOGENIC ISOLATES OF FUSARIUM OXYSPORUM
33
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Introduction
Fusarium oxysporum is comprised of more than 120 formae speciales
and races as well as nonpathogenic strains (3.3). The nonpathogenic
strains of £. oxysporum comprise the largest proportion of the soilborne
population (3.7, 3.29). The pathogenic and nonpathogenic strains form a
homogeneous taxonomic group because they are morphologically
indistinguishable from one another. Both are known to infect the roots of
host and nonhost plants (3.2, 3.5, 3.7, 3.13, 3.14, 3.15), and
nonpathogenic strains may colonize the root cortex without causing
disease. Thus, pathogenic and nonpathogenic strains are well adapted to
surviving in the soil, and some nonpathogenic strains are known to occupy
and compete with the pathogen for a specific niche, the cortex of the plant
root (3.12, 3.14, 3.29).
In 1975, Toussoun (3.30) suggested that some soils are suppressive
to pathogenic formae but not to nonpathogenic populations of £.
oxysporum. Schneider (3.27) demonstrated that certain nonpathogenic
strains of £. oxysporum. collected from symptomless celery roots,
effectively predisposed the host to or suppressed infection by the
pathogen, £. oxysporum f. sp. aoii, on celery. He went on to show that a
soil suppressive to Fusarium yellows of celery had a higher proportion of
effective competitive strains as compared to a disease conducive soil.
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Preliminary competitive infection tests showed that there also are
differences within a collection of nonpathogenic isolates from symptomless
field-grown tomato plants in the ability to suppress infection by E-
oxysporum f. sp. lycopersici on tomato. These isolates may enhance,
suppress, or have a neutral effect on infection. Except for one example
(3.27), the use of nonpathogenic strains of E. oxysporum as biological
control agents against Fusarium w ilt of tomato has been largely unexplored.
The primary question to be addressed in this study is whether or not
competitive effectiveness is confined to discrete subpopulations within the
nonpathogenic, tomato root-infecting population of E. oxysporum. Having
already established the existence of vegetative compatibility groups (VCGs)
in this population (3.10, 3.11), it seemed intuitive that, if competitive
infection ability was to be confined to discrete subpopulations, VCGs
should function in this capacity because they form clonal, genetically
distinct groups.
Vegetative compatibility is assessed in E. oxysporum with
complementary nutritional mutants (3.25). Nitrate metabolism (n il) mutants
are selected from fast growing, chlorate resistant sectors growing on a
chlorate medium. When grown on a minimal medium containing nitrate as
a nitrogen source, the n il mutants grow very sparsely. N il mutants may
then be phenotypically classified by their growth on media which is
amended with one of several different nitrogen sources (3.9). When two
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36
complementary mutants are paired on minimal medium, heterokaryosis may
occur and is characterized by a zone of wild-type growth. This occurs as a
result of hyphal fusion, nuclear exchange, and nutritional complementation
(3.25). If two isolates are vegetatively compatible, these isolates must have
identical alleles at each vegetative incompatibility (vie) locus, and they are
considered to be closely related if not clonal derivatives (3.11, 3.25).
Vegetative compatibility groups have been used previously as a genetic
marker to distinguish between £. oxysporum and £. oxysporum f. sp.
vasinfectum (3.16).
The objective of this study was to determine if competitive
effectiveness is associated with VCGs or clonal populations. If effective,
ineffective, or neutral isolates are confined to different specific VCGs, this
would be evidence that the genetic traits for competitive effectiveness are
subject to selection pressures.
Materials and Methods
Fungal strains. Putative nonpathogenic strains of £. oxysporum were
collected from symptomless tomato roots in locations where tomatoes had
been grown in monoculture for many years. Root samples were taken from
the following sites: Oak Grove, LA (West Carroll Parish), Tombrallo Farm in
Shreveport, LA (Caddo Parish), Calhoun Research Station, Calhoun, LA
(Ouachita Parish), Sweet Potato Research Station, Chase, LA (Franklin
Parish), and the Citrus Research Station, Port Sulphur, LA (Plaquemines
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Parish) (Figure 3.1). Root pieces were surface-sterilized with 4% household
bleach (0.21% sodium hypochlorite) for 4 min, rinsed in sterile, distilled
water, plated on Komada's medium, which is selective for Fusarium spp.
(3.17), and incubated at room temperature. Resulting colonies were single-
spored, transferred to carnation leaf agar (CLA) (3.20) for identification,
and isolates of £. oxysporum were stored on silica gel at 4 C (3.23). A
total of 471 isolates was collected and tested for pathogenicity against a
susceptible cultivar by the root-dip method of inoculation (3.31). Seedlings
were grown in sterile, commercially prepared potting soil mix for 2 wk until
the first true leaves emerged. The tomato cultivars 'Fantastic' (susceptible
to races 1, 2, and 3); 'Supersonic' (resistant to race 1); and 'Walter'
(resistant to races 1 and 2) were used as hosts. Fungal strains were grown
in Czapek's solution for 5 days on an orbital shaker at room temperature.
The cultures were filtered through cheesecloth and the resulting spore
suspension was adjusted to about 106 spores per ml. Seedlings were gently
uprooted, and roots were pruned to about 3 cm in length. Six seedlings per
cultivar were dipped into spore suspensions of each strain for 30 sec and
transplanted to plastic cell trays pre-filled with soil-peat moss mix (50:50,
v:v) at the rate of one seedling per cell. Two controls were used: seedlings
with pruned roots were dipped in either sterile water or inoculum of a race
1 FPL isolate. Disease symptoms were recorded 10-14 days after
inoculation.
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38
S P H
•.-4 3
'n » v • » /— -1 \ ' *
1 = Oak Grove, West Carroll Parish, LA; 2 = Chase, Franklin Parish, LA; 3 = Shreveport, Caddo Parish, LA; 4 = Calhoun, Ouachita Parish, LA;5 = Citrus Station, Plaquemines Parish, LA.
Figure 3.1. Location of sites sampled in Louisiana for nonpathogenic strains of Fusarium oxysporum.
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The susceptibility of tomato cultivars to a particular isolate of E.
oxysporum was recorded after 14 days. Pathogenicity tests were
conducted at least twice. All of the nonpathogenic strains of E. oxysporum
were assessed for VCG (3.10, 3.11). \
Inoculum preparation. Orange mutant cultures were grown in PDB on a
rotary shaker for 72 hr at room temperature. One hundred grams of finely
ground corncob grit (Grit O'Cob, Nebraska) in 250-ml Erlenmeyer flasks
were moistened with 10 ml 0.025M L-asparagine, autoclaved for 1 hr on
each of two consecutive days, inoculated with a conidial suspension {106 /
ml) obtained from the PDB cultures, and incubated for 2 wk at room
temperature. The ground corncob cultures, hereafter referred to as
inoculum, were dried at room temperature in 100mm by 80mm deep petri
plates covered with cheesecloth, ground with a mortar and pestle, and
refrigerated until used.
Competitive root infection studies within vegetative compatibility groups.
Competitive infection experiments were conducted using members of VCGs
2028, 2035, 2050, and 2061 (Table 3.1). These VCGs were selected
because they were multiple member VCGs made up of isolates from more
than one location. One kg of a sterile Mississippi alluvial soil from St.
Gabriel, LA was amended with 0.5 g of ORA-22 inoculum and 0.5 g of
inoculum of each test isolate, mixed in a large plastic bag until well
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Table 3.1 Strains of Fusarium oxysporum used in the present study and their designation by vegetative compatibility group.
STRAIN ORIGIN
VCG2028
CH-51 * Franklin ParishCH-5 Franklin ParishCH-35 Franklin ParishCH-43 Franklin ParishCH-45 Franklin ParishCAL-11 Ouachita ParishCAL-13 Ouachita ParishCAL-14 Ouachita ParishCAL-17 Ouachita ParishCAL-18 Ouachita Parish
VCG 2035
TOM-32* Caddo ParishTOM-13 Caddo ParishTOM-14 Caddo ParishTOM-23 Caddo ParishTOM-29 Caddo ParishTOM-38 Caddo ParishTOM-44 Caddo ParishTOM-46 Caddo ParishTOM-51 Caddo ParishTOM-59 Caddo ParishCAL-2 Ouachita Parish
‘ Denotes tester strain
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Table 3.1 (cent.)
STRAIN ORIGIN
VCG 2050
CS3-27* Plaquemines ParishCS3-6 Plaquemines ParishCS3-14 Plaquemines ParishCS3-19 Plaquemines ParishCS3-22 Plaquemines ParishCS3-26 Plaquemines ParishCS3-28 Plaquemines ParishCS3-37 Plaquemines ParishCS3-39 Plaquemines ParishCS3-42 Plaquemines ParishCS3-43 Plaquemines ParishCAL-23 Ouachita Parish
VCG 2061
CAL-64* Ouachita ParishCAL-6 Ouachita ParishCAL-29 Ouachita ParishCAL-32 Ouachita ParishCAL-33 Ouachita ParishCAL-44 Ouachita ParishCAL-47 Ouachita ParishCAL-51 Ouachita ParishCAL-56 Ouachita ParishCAL-69 Ouachita ParishOG-37 West Carroll Parish
* Denotes tester strain
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42
blended, and dispensed into 10-cm clay pots. Tomato seedlings, cultivar
'Supersonic', were transplanted into the pots and grown for 4
wk in the greenhouse. At harvest, the plants were removed from the pots,
and the soil was carefully washed from the roots. The roots were surface-
sterilized for 4 min in 0.21 % NaOCI (3.27), rinsed in three changes of
sterile water, plated on Komada's medium (3.17), and incubated at room
temperature for 1 wk. The number of orange and wild-type colonies was
determined on each plate. Root lengths on each plate were estimated using
a line intersect grid method (3.21, 3.29). These data were used to
calculate the number of colonies per 100 cm of root according to the
method of Schneider (3.27). All competitive infection tests were performed
initially within each VCG and repeated using all isolates. Analyses of
variance were performed and means were compared by Duncan's multiple,
range test (E = 0.05) using pc SAS (3.26).
Results
Pathogenicity of fungal strains. None of the putative nonpathogenic strains
of E. oxysporum isolated from symptomless tomato roots caused disease
symptoms on the appropriate differential tomato cultivars used in the
pathogenicity tests. Based on these results, they are assumed to be
nonpathogenic E. oxysporum.
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43
Competitive root infection studies within vegetative compatibility groups.
Coinoculation of the pathogen with nonpathogenic members of VCGs 2028
and 2035 resulted in significantly suppressed infection by the pathogenic
orange mutant, ORA-22, at P = 0.05 and P = 0.01, respectively (Tables
3.2 and 3.3). Mean root infection by ORA-22 was reduced by 68.9% and
82.8% across all members of VCGs 2028 and 2035, respectively (Table
3.4). In VCGs 2050 and 2061, individual isolates caused statistically
significant reductions in infection by ORA-22 relative to the inoculated
control, but, as a group, these VCGs did not significantly affect infection by
the pathogen (Tables 3.5 and 3.6). There were no significant correlations
between root infection by the pathogen and nonpathogens in any of the
VCGs (Tables 3.2, 3.3, 3.4, and 3.5). Taken as a whole, members of VCG
2061 had no significant effect on infection by the pathogen; however,
isolate CAL-51 caused a significant increase in infection relative to the
inoculated control. When viewed as subpopulations, VCGs 2061 and 2050
were significantly different from VCGs 2035 and 2028 in their interaction
with the pathogen (Table 3.6). The latter three VCGs caused a significant
reduction in infection by the pathogen with VCG 2035 causing more than
80% reduction in infection by ORA-22. VCGs 2035 and 2028 are not
significantly different; however, they are significantly different from VCG
2050 and VCG 2061.
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Table 3.2. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of £. oxysporum for members of VCG 2028.
ISOLATE NUMBER OF COLONIES PER 100 CM ROOT
.0RA:22 NQNRAIHD.GENS
ORA-22 13.68 0.24CH-51 10.45 0.06CH-43 6.76 5.72CH-35 5.51 9.60CH-5 4.12 3.98CAL-11 3.09 6.03CAL-13 2.77 3.64CH-45 2.72 12.49CAL-18 2.70 4.73CAL-17 2.41 3.70CONTROL 2.05 0.49CAL-14 1.96 5.66
LSDa 7.11 5.63
ALeast significant difference ( P = 0.05 ), R2 = -0.185.
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45
Table 3.3. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of F. oxysporum for members of VCG 2035.
ISOLATE NUMBER OF COLONIES PER 100 CM ROOT
QBAi22 NONPATHOGENS
ORA-22 22.49 0.05TOM-46 12.62 11.27CAL-2 5.50 2.30TOM-13 5.20 7.79TOM-29 5.01 8.55TOM-51 3.65 5.83TOM-32 2.67 12.81TOM-44 2.23 6.31TOM-38 1.84 0.37TOM-14 1.62 2.79TOM-23 1.36 4.32TOM-59 0.81 1.31CONTROL 0.58 0.00
LSDA 10.49 6.21
ALeast significant difference ( P = 0.05 )f R2 = -0.001.
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Table 3.4. Relative competitive infection of nonpathogenic Fusarium oxysporum isolated from tomato roots.
VCG MeanA SEM
2035 0.15 a 0.052028 0.19 ab 0.072050 0.36 b 0.062061 0.96 c 0.18
Source of Variation DF SS MSBetween Treatments 3 4.60 1.53Residual 40 4.81 0.12Total 43 9.41
F P12.73 < 0.001
AMeans with a common letter are not significantly different at P = 0.05 based on the Student-Newman-Keuls test (Sigma Stat).
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Table 3.5. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of E. oxysporum for members of VCG 2050.
ISOLATE NUMBER OF COLONIES PER 100 CM ROOT
ORA-22 NONPATHOGENS
ORA-22 6.86 0.00CS3-6 6.62 1.29CS3-37 3.00 1.59CS3-22 2.88 0.50CS3-28 2.87 1.68CS3-39 2.70 4.23CS3-27 2.08 1.78CS3-42 1.99 1.26CS3-14 1.84 2.12CS3-26 1.63 1.47CAL-23 1.54 2.01CS3-19 1.29 1.60CS3-43 0.82 1.35CONTROL 0.00 2.23
LSDa 2.85 2.19
ALeast significant difference ( P = 0.05 ), R2 = -0.176.
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Table 3.6. Rate of infection by the orange mutant (ORA-22) in the presence of nonpathogenic isolates of £. oxysporum for members of VCG 2061.
ISOLATE NUMBER OF COLONIES PER 100 CM ROOT
O.RA-22 NONPATHOGENS
CAL-51 4.23 4.66CAL-64 2.38 1.92CAL-33 2.15 2.17CAL-56 2.02 1.12ORA-22 1.74 0.06CAL-29 1.59 1.88CAL-6 1.32 3.22OG-37 1.17 1.95CAL-47 1.07 1.83CAL-69 1.02 2.81CAL-44 0.88 2.16CAL-32 0.57 1.28CONTROL 0.04 0.24
LSDA 2.16 2.29
ALeast significant difference ( P = 0.05 ), R2 - -0.36.
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49
LUCC
2.5
zg 1.5oLUL l.
? 1LU>H
0.5
laIfnmirTv
MEANS
E3 VCG 2035 , 0.15 a
CD VCG 2028 , 0.19 ab
0 VCG 2050 , 0.36 b
□ VCG 2061 , 0.96 c
T-Ttco(DO)(Oh~h'0 )^toj «Db~c\icoo>r^.cv^ftocoo)co T-eoinini-coincor>.’5i- (DOJcoaii-cv^co^tcoo) in cocoinc\)_,co^-<£>■<*« pjCoojojcocv^-t-ojojt-^ in^co^-T-i-TtT-r-r- ^■_JT-cvinco'5rcoT-ciiio_ ^ _____ C/5 CO CO CO CO CO CO CO CO—I CO CO T T T f i J J I T —!1—•—Ii ^
o a o o o °°o o o o ° ^ o o o o o 8 o o oo o°< <o< << oooooooooooC X T 'O O O
ISOLATES
Figure 3.2. Rate of infection by an orange mutant (ORA-22) of Fusarium oxysporum f. sp. lycopersici in the presence of nonpathogenic isolates of E. oxysporum in all VCGs.
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50
Discussion
Cook and Baker (3.8) listed three general approaches to biological
control of plant pathogens: (i) control of pathogen inoculum, (ii)
protection against infection, and (iii) cross-protection or induced resistance.
With diseases caused by £. oxysporum. two models have been proposed;
enhanced resistance of the host induced by nonpathogenic Fusarium spp.
(3.4, 3.6, 3.18, 3.22, 3.32), and competition between pathogenic and
nonpathogenic strains of £. oxysporum for niches or limiting substrates as a
means for biological control (3.1, 3.27).
Using a pigmented mutant of £. oxysporum. Schneider (3.27)
demonstrated considerable variability in competitive infection within a
nonpathogenic population collected from symptomless celery roots. Some
of the nonpathogenic, parasitic strains of £. oxysporum predisposed celery
root to infection by the pathogenic forma, £. fl. f. sp. apii. while others
competitively suppressed infection. On the basis of a mathematical
analysis, he theorized that these nonpathogens competed with the
pathogen for the same ecological niche-namely, the infection court.
Garibaldi et al (3.12) determined the ability of £. oxysporum and E. solani to
compete with pathogenic Fusaria and speculated that effective strains were
able to rapidly follow root growth, preceding the pathogen in occupation of
infection sites. Finally, Paulitz, Park and Baker (3.24) documented very
large differences in biocontrol ability in their collection of nonpathogenic
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51
strains of E. oxysporum. While the above cited researchers showed that
there is variability in competitive infection ability within populations of
nonpathogens, they did not determine if this trait is associated with
discrete populations or if the trait is randomly distributed in the population
of nonpathogens.
Results from competitive root infection tests performed with
nonpathogenic strains of E. oxysporum from tomato, regardless of VCG, in
sterilized soils showed a range of effectiveness from no effect to
suppression and enhancement of root infection by the pathogen, E.
oxysporum f. sp. lycopersici. However, when categorized by VCG, there
were significant differences in competitive infection ability among these
clonal populations. In VCGs 2028, 2035, and 2050, the majority of isolates
acted similarly and suppressed infection by the pathogen. Members of VCG
2061 were not significantly different from the orange mutant control and
did not significantly suppress or enhance the rate of infection. This VCG
may be thought of as neutral. Vegetatively compatible strains are thought
to represent clonal populations and members of these VCG do act as
discrete units in their effect on infection of tomato roots by the orange
mutant. This theory will be tested by isozyme analysis to determine actual
genetic relatedness. These results suggest that competitive infection ability
is subject to selection pressures. Otherwise, one would expect to see this
trait randomly distributed across all VCGs. Clearly, these strains establish a
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52
parasitic relationship with the host, and it is to be expected that the host
would exert a significant selective force on the populations that are capable
of establishing such a relationship. In addition, if there is host specificity
within the nonpathogenic population, it would be expected to contribute to
differences in competitive infection abilities among VCGs. Because the role
of nonpathogens has been unrecognized and undefined in the past, little is
known of the effects of breeding tomato for resistance to Fusarium w ilt on
evolution of the nonpathogenic population. Future research should examine
the role of host genotype and crop rotation on the development of the
pathogenic and nonpathogenic populations using VCG as a genetic marker.
A possible evolutionary scenario is that competitive infection ability
provides a selective advantage to those strains that are able to parasitize
roots of specific plant species. These strains would be competing for a
specific niche, and selection pressure exerted by the host would favor
those strains that are most competitively fit. These strains would share
genetic traits associated with competitive infection ability and thus would
be more closely related than those that are less competitively fit. Those
strains that lost one or more of these traits would eventually be lost from
the population. The question arises as to why strains were recovered that
have substantially less competitive infection ability from tomato roots. It is
possible that these isolates would be more competitively f it on other hosts,
but, as has been established for pathogenic formae (3.2, 3.7, 3.13, 3.14,
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53
3.15), they are able to colonize other hosts as well. This scenario parallels
that which is already established for the pathogenic formae in which host
specificity is confined to unique VCGs (3.10).
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54
Literature Cited in Chapter 3
3.1. Alabouvette, C., Y. Couteaudier, and J. Louvet. 1984. Recherches sur la resultant de sols aux maladies, IX Dynamiques des populations du Fusarium spp. et de Fusarium oxysporum f. sp. meionis dans un sol resultant et dans un sol sensible aux fusarioses vasculaires. Agronomie 4:729-733.
3.2. Armstrong, G. M. and J. K. Armstrong. 1948. Nonsusceptible hosts as carriers of w ilt fusaria. Phytopathology 38:808-826.
3.3. Armstrong, G. M. and J. K. Armstrong. 1981. Formae speciales and races of Fusarium oxysporum causing w ilt diseases. Pages 391 - 399 in Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. Pennsylvania State University Press, University Park.
3.4. Baker, R., P. Hanchey, and S. D. Dottarar. 1978. Protection of carnation against Fusarium stem rot by fungi. Phytopathology 68:1495-1501.
3.5. Beckman, C. H. 1987. The Nature of Wilt Diseases in Plants. American Phytopathological Society, St. Paul. 175 pp.
3.6. Biles, C. L., and R. D. Martyn. 1989. Local and systemic resistance induced in watermelons by formae speciales of Fusarium oxysporum. Phytopathology 79:856-860.
3.7. Burgess, L. W. 1981. General ecology of the Fusaria. Pages 225- 235 in Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. Pennsylvania State University Press, University Park.
3.8. Cook, R. J. and K. F. Baker. 1983. The Nature and Practice of Biological Control of Plant Pathogens. The American Phytopathological Society, St. Paul. 539 pp.
3.9. Correll, J. C., C. J. R., Klittich, and J. F. Leslie. 1987. Nitrate nonutilizing mutants of Fusarium oxysporum and their use in vegetative incompatibility tests. Phytopathology 77:1640-1646.
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55
3.10. Elias, K. S. 1989. Vegetative compatibility groups of Fusarium oxysporum f. sp. lycopersici and nonpathogenic strains of £. oxysporum and a isozyme analysis of pathogenic populations. Ph.D. dissertation, Louisiana State University, Baton Rouge. 93 pp.
3.11. Elias, K. S., R. W. Schneider, and M. M. Lear. 1991. Analysis of vegetative compatibility groups in nonpathogenic populations of Fusarium oxysporum isolated from symptomless tomato roots. Can. J. Bot. 69:2089-2094.
3.12. Garibaldi, A., L. Gugliemone, and M. L. Gulino. 1990. Rhizosphere competence of antagonistic Fusaria isolated from suppressive soils. Symbiosis 9:401-404.
3.13. Gordon, T. R., D. Okamoto, and D. J. Jacobson. 1989.Colonization of muskmelon and nonsusceptible crops by Fusarium oxysporum f. sp. melonis and other species of Fusarium. Phytopathology 79: 1095-1100.
3.14. Hendrix, D. L., and L. W. Nielsen. 1958. Invasion and infection by crops other than the forma suscept by Fusarium oxysporum f. sp. batatas and other formae. Phytopathology 48: 224-228.
3.15. Katan, J. 1971. Symptomless carriers of the tomato Fusarium w ilt pathogen. Phytopathology 61: 1213-1217.
3.16. Katan, T., and Katan, J. 1988. Vegetative compatibility grouping of Fusarium oxysporum f. sp. vasinfectum from tissue and the rhizosphere of cotton plants. Phytopathology 78:852-855.
3.17. Komada, H. 1975. Development of a selective medium for quantitative isolation of Fusarium oxysporum from natural soil. Rev. Plant Protection Res. 8:114-124.
3.18. Larkin, R. P., D. L. Hopkins, and F. N. Martin. 1993. Effect of successive watermelon plantings on Fusarium oxysporum and other microorganisms in soils suppressive and conducive to Fusarium w ilt of watermelon. Phytopathology 83:1097-1105.
3.19. Mandeel, Q., and R. Baker. 1991. Mechanisms involved in biological control of Fusarium w ilt of cucumber with strains of Fusarium oxysporum. Phytopathology 81: 462-469.
Reproduced with permission of the copyright owner. Further reproduction prohibited without permission.
3.20. Nelson, P. E., T. A. Toussoun, and W. F. 0. Marasas. 1983. Fusarium Species: An Illustrated Manual of Identification. Pennsylvania State University Press, University Park. 193 pp.
3.21. Newman, E. I. 1966. A method of estimating the total length of root in a sample. J. Appl. Ecol. 3:139-145.
3.22. Ogawa, K. and H. Komada. 1985. Biological control of Fusarium w ilt with cross-protection by nonpathogenic Fusarium oxysporum. Pages 121-123 in: Ecology and Management of Soilborne Plant Pathogens . C. A. Parker, A. D. Rovira, K. J. Moore and P. T. W. Wong, eds. The American Phytopathological Society, St. Paul.
3.23. Perkins, D. D. 1962. Preservation of Neurospora stock cultures with anhydrous silica gel. Can J. Microbiol. 8:591-594.
3.24. Paulitz, T. C., C. S. Park, and R. Baker. 1987. Biological control of Fusarium wilt of cucumber with nonpathogenic isolates of Fusarium oxysporum. Can. J. Microbiol. 33:349-353.
3.25. Puhalla, J. E. 1985. Classification of strains of Fusarium oxysporum on the basis of vegetative compatibility. Can. J. Bot. 63:179-183.
3.26. SAS Institute Inc. 1987. SAS/STAT Guide for Personal Computers, Version 6 Edition. J. Chris Parker, ed. SAS Institute Inc., Cary.1028 pp.
3.27. Schneider, R. W. 1984. Effects of nonpathogenic strains of Fusarium oxysporum on celery root infection by Fusarium oxysporum f. sp. apii and a novel use of the Lineweaver-Burk double reciprocal plot technique. Phytopathology 74:646-653.
3.28. Stoner, M. F. 1981. Ecology of Fusarium in noncultivated soils. Pages 276-286 in: Fusarium: Diseases, Biology and Taxonomy. P. E. Nelson, T. A. Toussoun, and R. J. Cook, eds. The Pennsylvania State University Press, University Park.
3.29. Torssell, W. R., J. E. Begg, C. W. Rose, and G. F. Byrne. 1968. Stand morphology of Townsville lucerne (Stylosanthes humilis). Seasonal growth and root development. Aust. J. Exp. Agric. Anim. Hub. 8:532-543.
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3.30. Toussoun, T. A. 1975. Fusarium-suppressive soils. Pages 145-151 in: Biology and Control of Soil-Borne Plant Pathogens. G. W.Bruehl, ed. American Phytopathological Society, St. Paul.
3.31. Williams, P. H. 1981. Fusarium yellows. Pages 124-129 in: Screening Crucifers for Multiple Disease Resistance. P. H. Williams, ed. University of Wisconsin Press, Madison.
3.32. Wymore, L. A., and R. Baker. 1982. Factors affecting crossprotection in control of Fusarium w ilt of tomato. Plant Dis. 6:908- 910.
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CHAPTER 4
ISOZYME ANALYSIS OF SELECTED VEGETATIVE COMPATIBILITY GROUPS OF NONPATHOGENIC FUSARIUM OXYSPORUM
58
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Introduction
Puhalla (4.20) developed a technique to assign fungi to vegetative
compatibility (heterokaryon) groups (VCG) using nitrate metabolism (nit)
mutants. In Gibberella fujikuroi (Fusarium moniliforme) (4.5, 4.16, 4.21), it
has been shown that a minimum of ten yic loci control vegetative
compatibility. It is generally assumed that £. oxysporum has a set of
vegetative incompatibility loci which are similar to <£. fujikuroi (4.21). In
order for tw o isolates to be vegetatively compatible, alleles at each of the
vie loci must be identical (4.16, 4.21). Puhalla and Spieth (4.21) showed,
using sexual crosses between vegetatively incompatible strains of Q..
fujikuroi. that yic genes are not expressed in the sexual phase, and they
theorized that vegetative incompatibility is independent of the factors
governing sexual reproduction.
Correll, Puhalla and Schneider (4.6) first utilized VCG analysis to
examine a collection of £. £. f. sp. apii. Since then, VCG analysis has been
used to delimit populations of many formae speciales of £. oxysporum (4.2,
4.6, 4.8, 4.10, 4.12, 4.13, 4.15, 4.19, 4.20), but few populations of
nonpathogenic £. oxysporum have been studied (4.7, 4.9). VCG analysis
provides categorical evidence for genetic relatedness but does not address
genetic diversity in a quantitative manner. That is, if two populations are
vegetatively compatible, additional experimental analysis would have to be
conducted in order to establish how diverse the two populations are.
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Analysis of enzyme polymorphisms, as defined by isozyme
electrophoresis, can be used to estimate the amount of genetic variation
among organisms. Having established that competitive infection ability is
associated with specific VCGs, the objective of this study was to estimate
genetic diversity within and among these clonal populations using starch
gel electrophoresis.
Materials and Methods
Fungal strains. Isolates used for isozyme analysis were members of the
following VCGs: 2028, 2035, 2050, and 2061 (Table 4.1). One isolate of
E. oxysporum (OG-15), one isolate of FPL (LSU-2), and the orange mutant
(ORA-22) were included as standards in all assays.
Tissue preparation. Each fungal strain was grown in four 250-ml
Erlenmeyer flasks containing 100 ml each of potato dextrose broth for 4-5
days on an orbital shaker at room temperature. Mycelial mats were
centrifuged at 5,000 rpm at 4 C in sterilized centrifuge bottles, and the
supernatant was discarded. One hundred ml of sterile, distilled water was
added to the mycelial pellet, and the suspension was shaken and
centrifuged again at 5,000 rpm at 4 C. The mycelial pellet was placed in a
sealed plastic petri dish and frozen at - 70 C overnight before lyophilization.
Protein extraction. Lyophilized mycelium was ground to a fine powder with
an ice cold mortar and pestle. A suspension of 0.6 g of the mycelial
powder and 2.25 ml of 0.05M Tris-HCI (pH 7.1) was mixed in a small
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61
centrifuge tube and incubated for 15 min on ice. Samples were centrifuged
for 27 min at 18,000 rpm at 4 C. The supernatant was withdrawn from the
tube using a Pasteur pipette without disturbing the lipid layer at the top of
the tube or the pellet at the bottom. The supernatant was dispensed into
microfuge tubes in 100 //I aliquots and stored at -70 C. Enough extract
was prepared for 10 electrophoretic runs. Extra mycelial powder was
stored in small vials at -70 C.
Electrophoresis. Ten-//I aliquots of the extracts were absorbed onto filter
paper wicks (Whatman No. 3). The wicks were loaded onto a 15 cm by 20
cm horizontal potato starch gel (12% w/v), and the extracts were subjected
to electrophoresis at 50mAmp for 4 to 6 hr depending on the buffer system
used (Appendix B). Gels were cooled with ice packs for the duration of the
run. After completion of electrophoresis, six 1.5 mm-thick horizontal slabs
were cut from each gel, each slab was treated with a specific enzyme
visualization reagent, and fixed using a 5:5:1 glacial acetic acid/methyl
alcohol/water solution (4.11, 4.17, 4.22, 4.23) (Table 4.2). Up to 15
samples, including one standard isolate with known banding patterns, were
analyzed on each gel slab. All isolates were analyzed at least tw ice in
separate gel runs.
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Table 4.1 Strains of Fusarium oxysporum used in the present study and their designation by vegetative compatibility group.
STRAIN ORIGIN
VCG 2028
CH-51 * Franklin ParishCH-5 Franklin ParishCH-35 Franklin ParishCH-43 Franklin ParishCH-45 Franklin ParishCAL-11 Ouachita ParishCAL-13 Ouachita ParishCAL-14 Ouachita ParishCAL-17 Ouachita ParishCAL-18 Ouachita Parish
VCG 2035
TOM-32* Caddo ParishTOM-13 Caddo ParishTOM-14 Caddo ParishTOM-23 Caddo ParishTOM-29 Caddo ParishTOM-38 Caddo ParishTOM-44 Caddo ParishTOM-46 Caddo ParishTOM-51 Caddo ParishTOM-59 Caddo ParishCAL-2 Ouachita Parish
'Denotes tester strain
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Table 4.1 (cont.)
STRAIN ORIGIN
VCG 2050
CS3-27* Plaquemines ParishCS3-6 Plaquemines ParishCS3-14 Plaquemines ParishCS3-19 Plaquemines ParishCS3-22 Plaquemines ParishCS3-26 Plaquemines ParishCS3-28 Plaquemines ParishCS3-37 Plaquemines ParishCS3-39 Plaquemines ParishCS3-42 Plaquemines ParishCS3-43 Plaquemines ParishCAL-23 Ouachita Parish
VCG 2061 -
CAL-64* Ouachita ParishCAL-6 Ouachita ParishCAL-29 Ouachita ParishCAL-32 Ouachita ParishCAL-33 Ouachita ParishCAL-44 Ouachita ParishCAL-47 Ouachita ParishCAL-51 Ouachita ParishCAL-56 Ouachita ParishCAL-69 Ouachita ParishOG-37 West Carroll Parish
'Denotes tester strain
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Table 4.2. Enzymes, abbreviations, Enzyme Commission (E.C.) numbers, and buffer systems used in this study.
Enzyme E. C. Number
Buffer
Aspartate amino transferase (AAT) 2.6.1.1 AAEsterase (EST) 3.1.1.1 CFumarase (FUM) 4.2.1.2 CGlucose-6-phosphate dehydrogenase (G6PDH) 1.1.1.1.49 CGlucose phosphate isomerase (GPI) 5.3.1.9 ALactate dehydrogenase (LDH) 1.1.1.27 CPhosphoglucomutase (PGM) 2.7.5.1 A
AA = amine citrate, pH 6.1; C = Tris-citrate/lithium borate, pH 8.5 (Appendix B).
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Analysis. The intensity and electrophoretic mobility, or the distance of
migration from the origin, were recorded for all bands. Bands on the gels
were numbered in the order of the fastest to slowest migration. A
composite of all bands for each isolate was tabulated, and these data were
used to calculate simple matching coefficients between isolates according
to the equation:
(+ +) + (- -)
Sm = -------------------------------
( + + ) + (--) + ( + -) + (- + )
where Sm = simple matching coefficient; + + = positive matches;
- - = negative matches; and (+ -) and (- + ) = mismatches. The
coefficients were then used to construct a similarity matrix (4.1) among the
electrophoretic phenotypes (EPs). Principal components analysis (PCA)
was employed to resolve phylogenetic groups. The computer program
NTSYS-pc, ver. 1.60 (Exeter Software, Setauket, NY) was used for these
analyses.
Results
Electrophoresis and analysis. Since optimal gel, electrode buffers and pH
had been previously determined for each enzyme assayed (4.8),
electrophoresis and data collection proceeded smoothly. Most of the
enzymes observed had multiple bands which indicate different loci, and/or
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66
alleles (Table 4.3). Results from the present study cannot be used to
distinguish alleles from loci because sexual crosses cannot be made.
The thirty-six isolates of FPL which make up VCGs 2028, 2035,
2050, and 2061 were assigned to 39 electrophoretic phenotypes (EP).
Principle components analysis (PCA) of isozyme polymorphisms in this
nonpathogenic population was performed, and the results showed that each
VCG was unique and clearly separated from the other VCGs. All
nonpathogenic VCGs were separated from the race 1 pathogenic isolates
used as controls (Figure 4.1).
Discussion
Nonpathogenic populations of £. oxysporum have not been
characterized because of problems in identification and separation. Elias,
Schneider and Lear (4.9) conducted a large survey and VCG analysis of
nonpathogenic isolates of £. oxysporum from tomato collected from 8
locations in Louisiana. Of 317 nonpathogenic isolates from symptomless
tomato roots, 186 isolates were in 48 multiple member VCGs and 131
isolates belonged to single member VCGs. Twenty one VCGs contained
members from more than one collection site. The nonpathogenic
population was found to be quite diverse.
Competitive infection test results show that there is an association
between competitive effectiveness or ineffectiveness and VCG. All VCGs
used in the present study contained members from two collection sites
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67
Table 4.3. Putative distribution for 15 putative enzyme loci in 36 isolates of Fusarium oxysporum isolated from symptomless tomato roots.
LocusA 1 2 3 4
AAT/GOT-1 3.0(10)B 2.5(20)AAT/GOT-2 0.7(10) 0.5(20)PGM-1 3.4(10) 3.0(10)PGM-2 1.3(10) 1.2(10)GPI-1 3.4(10) 2.8(19) 1.7(10)GPI-2 0.8(10)G6PDH 4.2(10) 3.3(10) 3.0(10) 2.5(9)FUM 3.4(10) 2.4(10)LDH-1 5.5(10) 2.6(10) 2.1(10) 1.9(9)LDH-2 3.3(10) 1.8(10) 1.7(9)LDH-3 2.7(10)EST-1 6.2(10) 4.6(13) 3.7(9)EST-2 3.3(10) 2.7(10) 2.1(9)EST-3 1.3(10) 1.1(10) 0.7(9)EST-4 0.8(13)
Abbreviations for enzyme loci according to Richardson (4.22). BDistance from origin (cm) (number of isolates).
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68
CM
j_O
" oo
Li_
0.8
0.6
0.4
0.2
0.0
- 0.2 •
-0 .4
0.6
- 0.8
Pathogens VCG 2028 VCG 2035 VCG 2050 VGG 2061
1.0 -0 .5 0.0 0.5
Factor 11.0 1.5
Figure 4.1. Principal components analysis of isozyme polymorphisms in nonpathogenic populations of Fusarium oxysporum. Numerals indicate the number of isolates in each cluster. Several symbols are representative of more than one isolate.
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69
(Table 4.1). Each population was clearly separated from the pathogenic
standards and was unique. These results provide strong evidence that the
genetic traits associated with competitive infection, beneficial, neutral or
detrimental, are confined to genetically isolated populations of
nonpathogenic £. oxysporum as delimited by VCG in much the same way
as pathogenicity is confined to specific VCGs (4.14, 4.16, 4.20).
Nonpathogens are possibly subject to the same selection pressures that
pathogens. Puhalla and Spieth (4.21) suggested that, in fungi, if the
sexual cycle is lost or ceases to occur, yic genotypes could be viewed as
separate "vegetative compatibility groups" each with a chance combination
of alleles from the last round of sexual reproduction. Any newly arising
variability would be confined to the VCG in which it originates. Normal
selection pressure would lead to the loss of some VCGs. Caten (4.3)
reported that isolates which belong to the same VCG are near isogenic and
probably clonally related, even though they may have been isolated
hundreds or thousands of miles apart.
Future research should include ecological studies to determine the
role of nonpathogenic Fusaria in agricultural systems. Attention should be
shifted to determining the population biology of nonpathogens. Now that
we are aware that the nonpathogenic population of Fusarium oxysporum is
composed of unique subpopulations, more research is needed to investigate
how they interact with the pathogen and host population and affect disease
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70
development. Long-term greenhouse experiments or outdoor microplot
experiments are needed to determine what effect the environment and /or
the combination of the host and environment have on competitive infection
ability of nonpathogenic £. oxysporum isolates and the development of host
specificity. Long-term greenhouse experiments using susceptible tomato
varieties in rotation with commonly grown crops should determine the
effect of crop rotation on VCG stability. In addition, colonization levels of
nonpathogens in soil in the absence of the pathogen should be monitored.
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71
Literature Cited in Chapter 4
4.1. Atlas, R. M., and R. Bartha. 1981. Microbial Ecology:Fundamentals and Applications. Addison-Wesley Publishing Co., Reading. 560 pp.
4.2. Bosland, P. W., and P. H. Williams. 1987. An evaluation of Fusarium oxysporum from crucifers based on pathogenicity, isozyme polymorphism, vegetative compatibility, and geographic origin. Can. J. Bot. 65:2067-2073.
4.3. Caten, C. E. 1987. Genetic integration of fungal life styles. Pages215-229 in: Evolutionary biology of the fungi. A. D. M. Rayner, C.M. Brasier, and David Moore, eds. Cambridge University,Cambridge. 465 pp.
4.4. Cornell, J. C. 1991. The relationship between formae speciales,races and vegetative compatibility groups in Fusarium oxysporum.Phytopathology 81:10061-1064.
4.5. Cornell, J. C., C. J. R. Klittich, and J. F. Leslie. 1989. Heterokaryon self-incompatibility in Gibbfi.rella fujikuroi (Fusarium moniliforme). Mycol. Res. 93:21-27.
4.6. Correll, J. C., J. E. Puhalla, and R. W. Schneider. 1986. Identification of Fusarium oxysporum f. sp. apii on the basis of colony size, virulence, and vegetative compatibility. Phytopathology 76:396-400.
4.7. Correll, J. C., J. E. Puhalla , and R. W. Schneider. 1986. Vegetative compatibility groups among nonpathogenic root-colonizing strains of Fusarium oxvsporum. Can. J. Bot. 64:2358-2361.
4.8. Elias, K. S. 1989. Vegetative compatibility groups of Fusarium oxysporum f. sp. lycopersici and nonpathogenic strains of £. oxysporum and a isozyme analysis of pathogenic populations. Ph.D. dissertation, Louisiana State University, Baton Rouge. 93 pp.
4.9. Elias, K. S., R. W. Schneider, and M. M. Lear. 1991. Analysis of vegetative compatibility groups in nonpathogenic populations of Fusarium oxysporum isolated from symptomless tomato roots. Can.J. Bot. 69:2089-2094.
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72
4.10. Elmer, W. H., and C. T. Stephens. 1989. Classification of Fusarium oxysporum f. sp. asparagi into vegetative compatibility groups. Phytopathology 79:88-93.
4.11. Harris, H., and D. A. Hopkinson. 1976. Handbook of enzyme electrophoresis in human genetics. North-Holland Bionedical Press, Amsterdam.
4.12. Jacobson, D. J., and T. R. Gordon. 1988. Vegetative compatibility and self-incompatibility within Fusarium oxysporum f . sp. melonis. Phytopathology 78:668-672.
4.13. Katan, T., and Katan, J. 1988. Vegetative compatibility grouping of Fusarium oxysporum f . sp. vasinfectum from tissue and the rhizosphere of cotton plants. Phytopathology 78:852-855.
4.14. Kistler, H. C., and E. A. Momol. 1990. Molecular genetics of plant pathogenic Fusarium oxysporum. Pages 49-54 in : Fusarium Wilt of Banana. R. C. Ploetz, ed. APS Press, St. Paul.
4.15. Larkin, R. P., D. L. Hopkins , and F. N. Martin. 1990. Vegetative compatibility within Fusarium oxysporum f. sp. niveum and its relationship to virulence, aggressiveness and race. Can. J. Microbiol. 36:352-358.
4.16. Leslie, J. F. 1990. Genetic exchange within sexual and asexual populations of the genus Fusarium. Pages 37-48 in: Fusarium Wilt of Banana. R. C. Ploetz, ed. APS Press, St. Paul.
4.17. Micales, J. A., M. R. Bonde, and G. L. Petterson. 1986. The use of isozyme analysis in fungal taxonomy and genetics. Mycotaxon 27:405-449.
4.18. Perkins, D. D., and B. C. Turner. 1988. Neurospora from natural populations: toward the population biology of a haploid eukaryote. Exper. Mycol. 12:91-131.
4.19. Ploetz, R. C., and J. C. Correll. 1988. Vegetative compatibility among races of Fusarium oxvsporum f. sp. cubense. Plant Dis. 72:325-328.
4.20. Puhalla, J. E. 1985. Classification of strains of Fusarium oxysporum on the basis of vegetative compatibility. Can. J. Bot. 63:179-183.
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73
4.21. Puhalla, J. E., and P. T. Spieth. 1985. A comparison of heterokaryosis and vegetative incompatibility among varieties of GibbeteJIa fujikuroi (Fusarium moniliforme). Exp. Mycol. 9:39-47.
4.22. Richardson, B. J., P. R. Braverstock, and M. Adams. 1986. Allozyme electrophoresis. Academic Press, New York. 410 pp.
4.23. Shaw, C. R., and R. Prasad. 1970. Starch gel electrophoresis of enzymes - a compilation of recipes. Biochem. Genet. 4:297-320.
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APPENDIX A.
MEDIA RECIPES
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Carnation Leaf Agar (CLA) (Nelson et al, 1983)
Carnation leaf agar is prepared by sprinkling treated (oven dried, dessicated with propylene oxide) carnation leaf tissue on freshly poured 2% water agar plates. The plates should be incubated at room temperature.
Czapek’s Solution (Tuite. 1969)
To 1 L of glass distilled water add:
NaNOg 2.0 g
K2HP04 1.0 g
MgS04-7H20 0.5 g
KCI 0.5 g
FeS04-7H20 10.0 mg (1 ml stock solution)*
Sucrose 30.0 g
Decant 100 ml solution into 250-ml Erlenmeyer flasks. Sterilize by autoclaving for 15 min. *Stock solution is made by adding 1 g to 100 ml water. This equals .01 g/ml or 10 mg/ml.
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Komada's Medium (Komada, 1975)
KH2P04 1.0 g
KCI 0.5 g
MgS04-7H20 0.5 g
FeNa EDTA 0.01 g
D - galactose 2.0 g
L - asparagine 2.0 g
Na2B40 7 1.0 g
PCNB 1.0 g(dissolve in 95% ETOH for 1 hr) orTerraclor 1.35 g
Oxgall (Bile Bovine) 0.5 g
Agar 15.0g
In separate flasks, sterilize 250 ml distilled water plus agar and 750 ml water. Autoclave for 15 min. Immediately after removal, add remaining ingredients to the flask containing the water and agar and bring to 1 L with additional sterilized H20.When cool add the following ingredients:
10% phosphoric acid 7.5 ml
Tergitol 0.5 ml
Tetracycline 0.3 g
Streptomycin 0.3 g
Pour into sterile petri dishes and cool.
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Minimal Medium (MM) (Puhalla, 1985)
To 1 L of glass-distilled water add:
Sucrose 30.0 g
NaNOg 2.0 g
KH2P04 1.0 g
MgS04-7H20 0.5 g
KCI 0.5 g
FeS04-7H20 0.1 g
Trace elements so l.** 0.2 g
Bacto agar 20.0 g
* * Trace elements solution
To 95 ml of distilled water add:
Citric acid 5.0 g
ZnS04-7H20 5.0 g
Fe(NH4)2(S04)2-6H20 1.0 g
CuS04-5H20 0.25 g
MnS04-H20 50.0 mg
H3B04 50.0 mg
NaMo04-2H20 50.0 mg
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78
For the other nitrogen source media (Correll et al, 1987), substitute one of these five nitrogen sources for nitrate as in MM described above:
1. Nitrate medium - use MM
2. Nitrite medium - add 0.5 g/L NaN02
3. Hypoxanthine medium - add 0.2 g/L hypoxanthine
4. Ammonium medium - add 1.0 g/L ammonium tartrate
5. Uric acid medium - add 0.2 g/L uric acid
Potato Dextrose Agar (PDA)
1. Cook 200 g peeled potatoes in 1 L of glass-distilled water for 15 min in the autoclave.
2. Strain the potatoes from broth using cheesecloth.
3. Bring to 1 L with glass-distilled water and add:
Dextrose 20.0 gBacto Agar 17.0 g
4. Autoclave for 15 min, cool and pour into sterile petri dishes.
Potato Dextrose Broth (PDB)
1. Cook 200 g peeled, sliced potatoes in 1 L of glass-distilled water for 15 min in the autoclave.
2. Strain the potatoes from the broth using cheesecloth.
3. Bring to 1 L with glass-distilled water and add:
Dextrose 18.0 g
4. Decant into 250-ml Erlenmeyer flasks, seal, and autoclave for 15 min.
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Potato Sucrose Medium (KPS) (Puhalla, 1985)
1. Cook 200 g peeled, sliced potatoes in I L of glass-distilled water for15 min in the autoclave.
2. Strain the potatoes from broth using cheesecloth.
3. Bring to 1 L w ith glass-distilled water and add:
4. Autoclave for 15 min, cool, and pour into sterile petri dishes.
Sucrose Bacto Agar KCI03
20.0 g20.0 g15.0 g
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80
Literature Cited in Appendix A
1. Correll, J. C., C. J. R. Klittich, and J. F. Leslie. 1987. Nitratenonutilizing mutants of Fusarium oxvsporum and their use in vegetative compatibility tests. Phytopathology 77:1640-1646.
2. Komada, H. 1975. Development of a selective medium for quantitative isolation of Fusarium oxysporum from natural soil. Rev. Plant Protection Res. 8:114-124.
3. Nelson, P. E., T. A. Toussoun, and W. F. 0 . Marasas. 1983.Fusarium Species: An Illustrated Manual of Identification. Pennsylvania State University Press, University Park. 193 pp.
4. Puhalla, J. E. 1985. Classification of strains of Fusariumoxysporum on the basis of vegetative compatibility. Can. J. Bot. 63:179-183.
5. Tuite, J. 1969. Plant Pathological Methods: Fungi and Bacteria. Burgess Publishing Co., Minnesota. 239 pp.
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APPENDIX B.
BUFFER SYSTEMS AND ENZYME STAINING SYSTEMS
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Buffer Systems
A. Amine-citrate Buffer (pH 6.1)
Electrode buffer
.04M citrate (C-0759) N-(3-amino-propyl)-morpholine (A-9028)
Adjust pH of citrate to 6.1 with morpholine.
fiaLbuffer
1:20 dilution of the electrode buffer.
Run at 50mAmp for 4 hours.
B. Tris-citrate/lithium-borate Buffer
Electrode buffer
.06M lithium hydroxide (L-4256),3M boric acid (B-0252)
Adjust to pH 8.1.
Gel buffer
.03M Tris (T-1503)
.005M citrate (C-0759)1 % electrode buffer
Adjust to pH 8.5.
Run at 50 mAmp for 6 hours.
Fixer
5:5:1 glacial acetic acid/ methyl alcohol/water
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83
Enzyme Staining Systems
Aspartate Aminotransferase (AAT/GOT)
0.1 M Tris-HCI (pH 8.0) 40.0 ml
Stock solution: 2.5 ml10 g Aspartate (A-9006)5 g alpha ketoglutyrate (K-1750)
in 100 ml H20 plus 25 ml 5N NaOH to pH 7.0
Pyridoxal-5-P04> dry (P-9255) 5.0 mg
FastBlue BB Salt (100 mg/ml) (F-0250) 0.75 ml
Incubate at room temperature for 15 min prior to adding FB. Incubate at 37 C for 30-60 min, rinse and fix.
Esterase (EST)
.2M monobasic sodium phosphate adjusted to pH 5.8 with .2M dibasic sodium phosphate 40.0 ml
a Naphthyl Acetate 7.5 mg (N-7000) 1.0 ml.15 g in 20 ml (10 ml acetone & 10 ml water)
P Naphthyl Acetate 7.5 mg (N-6875) 1.0 ml
1-propanol 2.5 ml
FastBlue RR Salt (50mg/ml) (F-0500) 1.0 ml
Incubate for 30-60 min at 37 C, rinse and fix.
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Fumarase (FUM)
0.1MTris-HCI 40.0 ml
1M Fumaric Acid, pH 7.0 with NaOH 5.0 ml
Malate dehydrogenase 100 units
NAD 10 mg (10mg/ml) (N-7004) 1.0 ml
MTT (5 mg/ml) 1.0 ml
PMS (1 mg/ml) 1.0 ml
Incubate for 30-60 min at 37 C, rinse and fix.
g iu c Q s e - 6 - p h o s D h a te d e h y d ro g e n a s e (G6PDH)
0.1M Tris-HCI, pH 8.0 40.0 ml
Glucose-6-phosphate, dry (G-7250) 100 mg
1M MgCI2 50 mg (100 mg/ml) 0.5 ml
NADP 10 mg (5 mg/ml) 2.0 ml
MTT 5 mg (5 mg/ml) 1.0 ml
PMS 2 mg (1 mg/ml) 2.0 ml
Incubate for 30-60 min at 37 C, rinse and fix.
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85
Glucose phosphate isomerase (GPI)
0.1 M Tris-HCI, pH 8.0 15.0 ml
Fructose-6-Phosphate 12 mg/ml (F-3627) 1.0 ml
Glucose-6-phosphate dehydrogenase 2.5 ml(G6PDH) 25 units (10 units/ml) (G-8878)
NADP 5 mg (5 mg/ml) 1.0 ml
1MMgCI2 0.5 ml
MTT (5 mg/ml) 1.0 ml
PMS (1 mg/ml) 1.0 ml
Incubate for 15-30 min at 37 C, bands appear quickly. Do not overstain. Rinse and fix.
Lactate Dehydrogenase (LDH)
0.1 M Tris-HCI, pH 8.5 40.0 ml
1M Lactate, pH 7.0 5.0 ml
NAD 10 mg (10 mg/ml) 1.0 ml
MTT (5 mg/ml) 1.0 ml
PMS (1 mg/ml) 1.0 ml
Incubate for 30-60 min at 37 C, rinse and fix.
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Phosphoglucomutase (PGM)
0.1 M Tris-HCI, pH 8.0 5.0 ml
Glucose-1-phosphate (G-1-P) 1.0 ml(100 mg/ml) (G-7000)
Glucose-1,6 diphosphate (.2 mg/ml) (G-7137) 1.0 ml
G6PDH 25 units (10 units/ml) 2.5 ml
1M MgCI2 1.0 ml
NADP 5 mg (5 mg/ml) 1.0 ml
MTT 5 mg (5 mg/ml) 1.0 ml
PMS 1 mg (1 mg/ml) 1.0 ml
Agar overlay. Add 20 ml molten agar just prior to pouring over gel. Incubate for 30-60 min at 37 C and fix.
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Literature Cited in Appendix B
1. Harris, H., and D. A. Hopkinson. 1976. Handbook of Enzyme Electrophoresis in Human Genetics. North-Holland Biomedical Press, Amsterdam.
2. Micales, J. A., M. R. Bonde, and G. L. Petterson. 1986. The use of isozyme analysis in fungal taxonomy and genetics. Mycotaxon 27:405-449.
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VITA
Monica Michelle Lear was born on May 30, 1959 in New Orleans,
Louisiana. She received a B. S. in Horticulture in May, 1982 and a M. S. in
Plant Health in August 1986 from Louisiana State University. In August,
1986, she enrolled in the Ph.D. program in the Department of Plant
Pathology and Crop Physiology. In April, 1991, she was employed as
Assistant Director of Horticulture and Quarantine Programs/Louisiana
Horticulture Commission at the Louisiana Department of Agriculture and
Forestry.
88
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DOCTORAL E X A M IN A T IO N AND D IS S E R T A T IO N REPORT
Candidate: Monica Michelle Lear
Major Field: Plant Health
Title of Dissertation: Interactions Between Fusarium oxysporum f . sp.lycopersici and Nonpathogenic Strains o f Fusarium oxysporum
Approved:
Major Bfofessor and chairman
EXAMINING COMMITTEE:
q w - hLyQ £.C l%6. <p.
W l . C .
n.
Date of Examination:
November 3, 1993
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