Rhizoctonia solani

Last updated

Rhizoctonia solani
Rhizoctonia hyphae 160X.png
Microscopic image of Rhizoctonia solani hyphae showing typical right-angled branching
Scientific classification OOjs UI icon edit-ltr.svg
Domain: Eukaryota
Kingdom: Fungi
Division: Basidiomycota
Class: Agaricomycetes
Order: Cantharellales
Family: Ceratobasidiaceae
Genus: Rhizoctonia
Species:
R. solani
Binomial name
Rhizoctonia solani
J.G. Kühn, 1858
Synonyms
  • Moniliopsis solani(J.G. Kühn) R.T. Moore 1987

Rhizoctonia solani is a species of fungus in the order Cantharellales. Basidiocarps (fruit bodies) are thin, effused, and web-like, but the fungus is more typically encountered in its anamorphic state, as hyphae and sclerotia. The name Rhizoctonia solani is currently applied to a complex of related species that await further research. In its wide sense, Rhizoctonia solani is a facultative plant pathogen with a wide host range and worldwide distribution. It causes various plant diseases such as root rot, damping off, and wire stem. It can also form mycorrhizal associations with orchids.

Contents

Taxonomy

In 1858, the German plant pathologist Julius Kühn observed and described a fungus on diseased potato tubers and named it Rhizoctonia solani, the species epithet referring to Solanum tuberosum (potato). The disease caused was well known before the discovery and description of the fungus. [1] In 1956, Dutch mycologist M.A. Donk published the new name Thanatephorus cucumeris for the spore-bearing teleomorph of R. solani, based on the species Hypochnus cucumeris originally described from diseased cucumbers in Germany. [2]

Subsequent research has shown that Rhizoctonia solani is a complex of related species. [3] This was originally based on observing hyphal anastomosis (or lack of it) in paired isolates grown in culture. Successful anastomosis indicated that the isolates were genetically similar, whilst unsuccessful anastomosis indicated they were dissimilar and distinct. [4] As a result Rhizoctonia solani has been split into at least 25 different "anastomosis groups" (AGs) and sub-groups. [5] These AGs tend to be associated with different plant diseases. [4] [6]

Molecular research, based on cladistic analysis of DNA sequences, has largely supported the division of R. solani into AGs. [7] [8]

Following changes to the International Code of Nomenclature for algae, fungi, and plants, the practice of giving different names to teleomorph and anamorph forms of the same fungus was discontinued, meaning that Thanatephorus became a synonym of the earlier name Rhizoctonia. [9] In its current sense, therefore, Rhizoctonia solani includes both anamorphic and teleomorphic forms of the fungus. Thanatephorus cucumeris is part of the R. solani species complex, but since it is based on a different type species, it may not be a synonym of R. solani sensu stricto.

Hosts and symptoms

Rhizoctonia solani sensu lato causes a wide range of commercially significant plant diseases. It is one of the fungi responsible for brown patch (a turfgrass disease), damping off (e.g. in soybean seedlings), [10] black scurf of potatoes, [11] bare patch of cereals, [12] root rot of sugar beet, [13] belly rot of cucumber, [14] banded leaf and sheath blight in maize, [15] sheath blight of rice, [16] and many other pathogenic conditions. The fungus, therefore, has a wide host range and strains of R. solani may differ in the hosts they are able to infect, the virulence of infection, selectivity for a given host (which may range from nonpathogenic to highly virulent), the temperature at which infection occurs, the ability to develop in lower soil levels, the ability to form sclerotia, the growth rate, and survival in a certain area. These factors may not always be distinctive in every host that Rhizoctonia attacks or in every strain thereof. [4]

R. solani causing crown rot infection on Beta vulgaris, common beet Rhizoctonia solani symptoms beet.jpg
R. solani causing crown rot infection on Beta vulgaris, common beet

R. solani primarily attacks seeds of plants below the soil surface, but can also infect pods, roots, leaves, and stems. The most common symptom of Rhizoctonia is "damping off", or the failure of infected seeds to germinate. R. solani may invade the seed before it has germinated to cause this pre-emergent damping off, or it can kill very young seedlings soon after they emerge from the soil. Seeds that do germinate before being killed by the fungus have reddish-brown lesions and cankers on stems and roots.

Various environmental conditions put plants at higher risk of infection. The pathogen prefers warmer, wet climates for infection and growth. Seedlings are most susceptible to disease in their early stages. [3]

Cereals in regions of England, South Australia, Canada, and India experience losses caused by R. solani every year. Roots are killed back, causing plants to be stunted and spindly. Other non-cereal plants in those regions can experience brown stumps as another symptom of the pathogen. R. solani can also cause hypocotyl and stem cankers on mature plants of tomatoes, potatoes, and cabbages. Strands of mycelium and sometimes sclerotia appear on their surfaces. Roots turn brown and die after a period of time. The best known symptom of R. solani is black scurf on potato tubers, the scurf being the sclerotia of the fungus.

Symptoms on common beans, Rhizoctonia damping off, blight, and rot Rhizoctonia solani symptoms on bean roots.jpg
Symptoms on common beans, Rhizoctonia damping off, blight, and rot

Disease cycle

Rhizoctonia solani can survive in the soil for many years in the form of sclerotia. Sclerotia of Rhizoctonia have thick outer layers to allow for survival, and they function as the overwintering structure for the pathogen. In some rare cases (such as the teleomorph) the pathogen may also take on the form of mycelia that reside in the soil, as well. The fungus is attracted to the plant by chemical stimuli released by a growing plant and/or decomposing plant residue. The process of penetration of a host can be accomplished in a number of ways. Entry can occur through direct penetration of the plant cuticle/epidermis or by means of natural openings in the plant. Hyphae come in contact with the plant and attach to the plant by which through growth they begin to produce an appressorium which penetrates the plant cell and allows for the pathogen to obtain nutrients from the plant cell. The pathogen can also release enzymes that break down plant cell walls, and continues to colonize and grow inside dead tissue. This breakdown of the cell walls and colonization of the pathogen within the host forms the sclerotia. New inoculum is produced on or within the host tissue, and a new cycle is repeated when new plants become available. The disease cycle begins as such:

  1. Sclerotia/mycelium overwinter in plant debris, soil, or host plants.
  2. The young hyphae and fruiting basidia (rare) emerge and produce mycelia and rarely basidiospores.
  3. The very rare production of the germinating basidiospores penetrate the stoma, whereas the mycelia land on the plant surface and secrete the necessary enzymes onto the plant surface to initiate invasion of the host plant.
  4. After the mycelia successfully invade the host, necrosis and sclerotia form in and around the infected tissue which then leads to the various symptoms associated with the disease, such as soil rot, stem rot, damping off, etc. and the process begins all over again. [17]

Environment

The pathogen is known to prefer warm, wet weather, and outbreaks typically occur in the early summer months. Most symptoms of the pathogen do not occur until late summer, thus most farmers do not become aware of the diseased crop until harvest. A combination of environmental factors has been linked to the prevalence of the pathogen, such as presence of host plant, frequent rainfall/irrigation, and increased temperatures in spring and summer. In addition, poor drainage of the soil (whether caused by parent soil texture, or by compaction) is also known to create favorable environments for the pathogen. [18] The pathogen is dispersed as sclerotia, and these sclerotia can travel by means of wind, water, or soil movement between host plants.

Identification

R. solani infection on cucumber Rhizoctonia solani.jpg
R. solani infection on cucumber

Basidiocarps (fruit bodies) are thin, effused, web-like, corticioid, smooth, and ochraceous. Microscopically they have comparatively wide hyphae without clamp connections. Basidia bear 2 to 4 sterigmata. Basidiospores are ellipsoid to oblong, smooth, and colourless, 7 to 10 x 4 to 5.5 μm. They frequently produce secondary spores and germinate by hyphal tubes. The anamorphs consist of hyphae and occasionally sclerotia (small propagules composed of thick-walled hyphae). [6] The fungus produces white to deep brown mycelium when grown on an artificial medium and can often be recognized by the hyphae which are frequently monilioid (forming chains of swollen hyphal compartments), 4 to 15 μm wide, multinucleate, and tend to branch at right angles.

Management

Complete control of Rhizoctonia solani is not possible, but the severity of the pathogen can be limited. Successful control depends on characteristics of the pathogen, host crops, and the environment. [19] Controlling the environment, crop rotation, using resistant varieties, [4] and minimizing soil compaction are effective and non-invasive ways to manage disease. Planting seedlings in warmer soil and getting plants to emerge quickly helps minimize damage. Crop rotation also helps minimize the amount of inoculum that results in infection. A few resistant varieties with moderate resistance to R. solani can be used, but they produce lower yields and quantity than standard varieties. Minimizing soil compaction helps water infiltration, drainage, and aeration for the plants.

One specific chemical option is a chemical spray pentachloronitrobenzene (PCNB), which is known to be the best solution to reducing damping-off of seeds on host plants. To minimize this soil-borne disease, certified seed free of sclerotia can be planted. Although fungicides are not the most effective way to manage this pathogen, a few have been approved in the United States by the USDA for control of the pathogen.

As long as seed growers stay clear of wet, poorly drained areas while also avoiding susceptible crops, R. solani is not usually a problem. Diseases caused by this pathogen are more severe in soils that are moderately wet and a temperature range of 15–18 °C (59–64 °F). [20]

Rice genetically engineered for overexpression of oxalate oxidase has increased in vivo resistance. [21]

Economic importance

In the United States, Rhizoctonia solani can be found across all areas (environmental conditions permitting) where its host crops are located. The severity of infection can vary. Consequences include major yield losses (from 25% to 100%), increased soil tare (because the soil sticks to the fungal mycelium), and poor industrial quality of the crops based on increased levels of sodium, potassium, and nitrogen. Due to the number of hosts that the pathogen attacks, these consequences are numerous and detrimental to a variety of crops. Sheath blight caused by this pathogen is the second-most devastating disease after rice blast. [22]

Mycorrhizal association with orchids

Rhizoctonia solani is one of several Rhizoctonia species forming mycorrhizal associations with orchids. This association includes plant pathogenic strains of the fungus [23] as well as non-pathogenic strains. [24]

Genome

The draft genome of R. solani strain Rhs1AP covers 51.7 Mbp, although the heterokaryotic genome of this strain was estimated at 86 Mb, based on an optical map of the chromosomes. The discrepancy is explained by the aneuploid, highly repetitive genome of this species which prevented sequencing (or assembling) the complete DNA. The genome is predicted to encode 12,726 genes. [25] Another strain,  AG1-IB 7/3/14, was recently sequenced too. [26]

Related Research Articles

<span class="mw-page-title-main">Texas root rot</span> Pathogenic fungus

Texas root rot is a disease that is fairly common in Mexico and the southwestern United States resulting in sudden wilt and death of affected plants, usually during the warmer months. It is caused by a soil-borne fungus named Phymatotrichopsis omnivora that attacks the roots of susceptible plants. It was first discovered in 1888 by Pammel and later named by Duggar in 1916.

<i>Aspergillus flavus</i> Species of fungus

Aspergillus flavus is a saprotrophic and pathogenic fungus with a cosmopolitan distribution. It is best known for its colonization of cereal grains, legumes, and tree nuts. Postharvest rot typically develops during harvest, storage, and/or transit. Its specific name flavus derives from the Latin meaning yellow, a reference to the frequently observed colour of the spores. A. flavus infections can occur while hosts are still in the field (preharvest), but often show no symptoms (dormancy) until postharvest storage or transport. In addition to causing preharvest and postharvest infections, many strains produce significant quantities of toxic compounds known as mycotoxins, which, when consumed, are toxic to mammals. A. flavus is also an opportunistic human and animal pathogen, causing aspergillosis in immunocompromised individuals.

<span class="mw-page-title-main">Sclerotium</span> Mycelial mass

A sclerotium, is a compact mass of hardened fungal mycelium containing food reserves. One role of sclerotia is to survive environmental extremes. In some higher fungi such as ergot, sclerotia become detached and remain dormant until favorable growth conditions return. Sclerotia initially were mistaken for individual organisms and described as separate species until Louis René Tulasne proved in 1853 that sclerotia are only a stage in the life cycle of some fungi. Further investigation showed that this stage appears in many fungi belonging to many diverse groups. Sclerotia are important in the understanding of the life cycle and reproduction of fungi, as a food source, as medicine, and in agricultural blight management.

<span class="mw-page-title-main">White onion</span> Onion cultivar

White onion or Allium cepa are a cultivar of dry onion which have a distinct light and mild flavour profile. Much like red onions, they have a high sugar and low sulphur content, and thus have a relatively short shelf life. White onions are used in a variety of dishes, such as those of Mexican and European origin. Their uses in dishes often relate to their mild nature, they are often included in dishes to provide a light, fresh and sour taste to dishes and are often added uncooked to dishes such as salads.

Phytophthora sojae is an oomycete and a soil-borne plant pathogen that causes stem and root rot of soybean. This is a prevalent disease in most soybean growing regions, and a major cause of crop loss. In wet conditions the pathogen produces zoospores that move in water and are attracted to soybean roots. Zoospores can attach to roots, germinate, and infect the plant tissues. Diseased roots develop lesions that may spread up the stem and eventually kill the entire plant. Phytophthora sojae also produces oospores that can remain dormant in the soil over the winter, or longer, and germinate when conditions are favourable. Oospores may also be spread by animals or machinery.

<i>Trichoderma viride</i> Species of fungus

Trichoderma viride is a fungus and a biofungicide.

This is a glossary of some of the terms used in phytopathology.

<span class="mw-page-title-main">Damping off</span> Horticultural disease or condition

Damping off is a horticultural disease or condition, caused by several different pathogens that kill or weaken seeds or seedlings before or after they germinate. It is most prevalent in wet and cool conditions.

Pythium ultimum is a plant pathogen. It causes damping off and root rot diseases of hundreds of diverse plant hosts including corn, soybean, potato, wheat, fir, and many ornamental species. P. ultimum belongs to the peronosporalean lineage of oomycetes, along with other important plant pathogens such as Phytophthora spp. and many genera of downy mildews. P. ultimum is a frequent inhabitant of fields, freshwater ponds, and decomposing vegetation in most areas of the world. Contributing to the widespread distribution and persistence of P. ultimum is its ability to grow saprotrophically in soil and plant residue. This trait is also exhibited by most Pythium spp. but not by the related Phytophthora spp., which can only colonize living plant hosts.

<i>Macrophomina phaseolina</i> Species of fungus

Macrophomina phaseolina is a Botryosphaeriaceae plant pathogen fungus that causes damping off, seedling blight, collar rot, stem rot, charcoal rot, basal stem rot, and root rot on many plant species.

<i>Stemphylium solani</i> Species of fungus

Stemphylium solani is a plant pathogen fungus in the phylum Ascomycota. It is the causal pathogen for grey leaf spot in tomatoes and leaf blight in alliums and cotton, though a wide range of additional species can serve as hosts. Symptoms include white spots on leaves and stems that progress to sunken red or purple lesions and finally leaf necrosis. S. solani reproduces and spreads through the formation of conidia on conidiophores. The teleomorph name of Stemphyllium is Pleospora though there are no naturally known occurrences of sexual reproduction. Resistant varieties of tomato and cotton are common, though the pathogen remains an important disease in Chinese garlic cultivation.

<i>Ceratobasidium cornigerum</i> Species of fungus

Ceratobasidium cornigerum is a species of fungus in the order Cantharellales. Basidiocarps are thin, spread on the substrate out like a film (effused) and web-like. An anamorphic state is frequently obtained when isolates are cultured. Ceratobasidium cornigerum is saprotrophic, but is also a facultative plant pathogen, causing a number of economically important crop diseases, and an orchid endomycorrhizal associate. The species is genetically diverse and is sometimes treated as a complex of closely related taxa. DNA research shows the species actually belongs within the genus Rhizoctonia.

<i>Alternaria solani</i> Species of fungus

Alternaria solani is a fungal pathogen that produces a disease in tomato and potato plants called early blight. The pathogen produces distinctive "bullseye" patterned leaf spots and can also cause stem lesions and fruit rot on tomato and tuber blight on potato. Despite the name "early," foliar symptoms usually occur on older leaves. If uncontrolled, early blight can cause significant yield reductions. Primary methods of controlling this disease include preventing long periods of wetness on leaf surfaces and applying fungicides. Early blight can also be caused by Alternaria tomatophila, which is more virulent on stems and leaves of tomato plants than Alternaria solani.

<i>Colletotrichum coccodes</i> Pathogenic fungus

Colletotrichum coccodes is a plant pathogen, which causes anthracnose on tomato and black dot disease of potato. Fungi survive on crop debris and disease emergence is favored by warm temperatures and wet weather.

<i>Rhizoctonia</i> Genus of fungi

Rhizoctonia is a genus of fungi in the order Cantharellales. Species form thin, effused, corticioid basidiocarps, but are most frequently found in their sterile, anamorphic state. Rhizoctonia species are saprotrophic, but some are also facultative plant pathogens, causing commercially important crop diseases. Some are also endomycorrhizal associates of orchids. The genus name was formerly used to accommodate many superficially similar, but unrelated fungi.

<i>Helicobasidium</i> Genus of fungi


Helicobasidium is a genus of fungi in the subdivision Pucciniomycotina. Basidiocarps are corticioid (patch-forming) and are typically violet to purple. Microscopically they have auricularioid basidia. Asexual anamorphs, formerly referred to the genus Thanatophytum, produce sclerotia. Conidia-bearing anamorphs are parasitic on rust fungi and are currently still referred to the genus Tuberculina.

Stromatinia cepivora is a fungus in the division Ascomycota. It is the teleomorph of Sclerotium cepivorum, the cause of white rot in onions, garlic, and leeks. The infective sclerotia remain viable in the soil for many years and are stimulated to germinate by the presence of a susceptible crop.

<span class="mw-page-title-main">Collar rot</span> Disease of plants

Collar rot is a symptomatically described disease that is usually caused by any one of various fungal and oomycete plant pathogens. It is present where the pathogen causes a lesion localized at or about the collet between the stem and the root. The lesions develop around the stem eventually forming a "collar". Observationally, collar rot grades into "basal stem rot", and with some pathogens is the first phase of "basal stem rot" often followed by "root rot". Collar rot is most often observed in seedings grown in infected soil. The pathogens that cause collar rot may be species or genera specific. But generalist pathogens such as Agroathelia rolfsii are known to attack over 200 different species. While bacteria caused collar rot is not common, trees infected with Fire blight may develop collar rot. Non-parasitic collar rot may be caused by winter damage.

<span class="mw-page-title-main">Sheath blight of rice</span> Fungal disease of rice

Rice-sheath blight is a disease caused by Rhizoctonia solani, a basidiomycete, that causes major limitations on rice production in India and other countries of Asia. It is also a problem in the southern US, where rice is also produced. It can decrease yield up to 50%, and reduce its quality. It causes lesions on the rice plant, and can also cause pre- and post-emergence seedling blight, banded leaf blight, panicle infection and spotted seed.

<i>Agroathelia rolfsii</i> Pathogen fungus

Agroathelia rolfsii is a corticioid fungus in the order Amylocorticiales. It is a facultative plant pathogen and is the causal agent of "southern blight" disease in crops.

References

  1. [Parmeter, J. R. Rhizoctonia solani, Biology and Pathology. London, UK: University of California, 1970. Print.], University of California Biology and Pathology.
  2. Donk MA (1956). "Notes on resupinate fungi II. The tulasnelloid fungi". Reinwardtia. 3: 363–379.
  3. 1 2 Cubeta MA, Vilgalys R (1997). "Population biology of the Rhizoctonia solani complex". Phytopathology. 87 (4): 480–84. doi:10.1094/PHYTO.1997.87.4.480. PMID   18945130.
  4. 1 2 3 4 Ogoshi, A (1987). "Ecology and Pathogenicity of Anastomosis and Intraspecific Groups of Rhizoctonia Solani Kuhn". Annual Review of Phytopathology . 25 (1). Annual Reviews: 125–143. doi:10.1146/annurev.py.25.090187.001013.
  5. Ogoshi A (1996). "Introduction—the genus Rhizoctonia". Rhizoctonia Species: Taxonomy, Molecular Biology, Ecology, Pathology and Disease Control: 1–9.
  6. 1 2 Roberts P. (1999). Rhizoctonia-forming fungi. Kew: Royal Botanic Gardens. p. 239. ISBN   1-900347-69-5.
  7. Gonzalez D, Carling DE, Kuninaga S, Vilgalys R, Cubeta MA (2001). "Ribosomal DNA systematics of Ceratobasidium and Thanatephorus with Rhizoctonia anamorphs". Mycologia. 93 (6): 1138–1150. doi:10.1080/00275514.2001.12063247. S2CID   196619800.{{cite journal}}: CS1 maint: multiple names: authors list (link)
  8. Sharon M, Sneh B, Kuninaga S, Hyakumachi M, Naito S (2008). "Classification of Rhizoctonia spp. using rDNA-ITS sequence analysis supports the genetic basis of the classical anastomosis grouping". Mycoscience. 49 (2): 93–114. doi:10.1007/S10267-007-0394-0. S2CID   86120090.{{cite journal}}: CS1 maint: multiple names: authors list (link)
  9. Oberwinkler F, Riess K, Bauer R, Kirschner R, Garnica S (2013). "Taxonomic re-evaluation of the Ceratobasidium-Rhizoctonia complex and Rhizoctonia butinii, a new species attacking spruce". Mycological Progress. 12 (4): 763–776. doi:10.1007/s11557-013-0936-0. S2CID   255319267.{{cite journal}}: CS1 maint: multiple names: authors list (link)
  10. Shanmugasundaram, S.; Yeh, C.C.; Hartman, G.L.; Talekar, N.S. (1991). Vegetable Soybean Research Needs for Production and Quality Improvement (PDF). Taipei: Asian Vegetable Research and Development Center. pp. 86–87. ISBN   9789290580478 . Retrieved 6 February 2016.
  11. Rhizoctonia disease of potato http://vegetablemdonline.ppath.cornell.edu/factsheets/Potato_Rhizoctonia.htm
  12. Rhizoctonia root rot http://cbarc.aes.oregonstate.edu/rhizoctonia-root-rot-bare-patch
  13. Rhizoctonia diseases of sugar beet "Management of Rhizoctonia Root Rot of Sugarbeet". Archived from the original on 19 June 2010. Retrieved 5 August 2010.
  14. Rhizoctonia disease of cucumber http://cuke.hort.ncsu.edu/cucurbit/cuke/dshndbk/br.html
  15. Yasmin, Humaira; Shah, Zafar Abbas; Mumtaz, Saqib; Ilyas, Noshin; Rashid, Urooj; Alsahli, Abdulaziz Abdullah; Chung, Yong Suk (13 September 2023). "Alleviation of banded leaf and sheath blight disease incidence in maize by bacterial volatile organic compounds and molecular docking of targeted inhibitors in Rhizoctonia solani". Frontiers in Plant Science. 14. doi: 10.3389/fpls.2023.1218615 . ISSN   1664-462X. PMC   10588623 . PMID   37868311.
  16. Rhizoctonia sheath blight https://onlinelibrary.wiley.com/doi/full/10.1111/pbi.13312
  17. Ceresini, Paulo. Rhizoctonia Solani. Rhizoctonia Solani. NC State University. Web. 4 November 2011 <http://www.cals.ncsu.edu/course/pp728/Rhizoctonia/Rhizoctonia.html>, NC State University Rhizoctonia Solani.
  18. "Rhizoctonia Diseases." Michigan Potato Diseases. P.S. Wharton, Michigan State University, 2 May 2011. Web. 4 October 2011. <http://www.potatodiseases.org/rhizoctonia.html>, P.S Wharton Michigan State University.
  19. Uchida, Janice Y. "Rhizoctonia Solani." Knowledge Master. Web. 4 Oct 2011. <http://www.extento.hawaii.edu/kbase/crop/type/r_solani.htm>, Janice Uchilda Knowledge Master.
  20. Anderson, Neil A (1982). "The Genetics and Pathology of Rhizoctonia Solani". Annual Review of Phytopathology . 20 (1). Annual Reviews: 329–347. doi:10.1146/annurev.py.20.090182.001553. ISSN   0066-4286.
  21. Molla, Kutubuddin A.; Karmakar, Subhasis; Chanda, Palas K.; Ghosh, Satabdi; Sarkar, Sailendra N.; Datta, Swapan K.; Datta, Karabi (1 July 2013). "Rice oxalate oxidase gene driven by green tissue-specific promoter increases tolerance to sheath blight pathogen (Rhizoctonia solani) in transgenic rice". Molecular Plant Pathology . 14 (9). Wiley: 910–922. doi:10.1111/mpp.12055. ISSN   1464-6722. PMC   6638683 . PMID   23809026. S2CID   38358538.
  22. Molecular Plant Pathology (2013) 14(9), 910–922
  23. Williamson B. Hadley G (1970). "Penetration and infection of orchid protocorms by Thanatephorus cucumeris". Pathology. 60: 1092–1096.
  24. Carling DE, Pope EJ, Brainard KA, Carter DA (1999). "Characterization of mycorrhizal isolates of Rhizoctonia solani from an orchid, including AG-12, a new anastomosis group". Phytopathology. 89 (10): 942–946. doi:10.1094/PHYTO.1999.89.10.942. PMID   18944739.{{cite journal}}: CS1 maint: multiple names: authors list (link)
  25. Cubeta MA, Thomas E, Dean RA, Jabaji S, Neate SM, Tavantzis S, Toda T, Vilgalys R, Bharathan N, Fedorova-Abrams N, Pakala SB, Pakala SM, Zafar N, Joardar V, Losada L, Nierman WC (2014). "Draft Genome Sequence of the Plant-Pathogenic Soil Fungus Rhizoctonia solani Anastomosis Group 3 Strain Rhs1AP". Genome Announc. 2 (5): e01072-14. doi:10.1128/genomeA.01072-14. PMC   4214984 . PMID   25359908.
  26. Wibberg D, Rupp O, Jelonek L, Kröber M, Verwaaijen B, Blom J, Winkler A, Goesmann A, Grosch R, Pühler A, Schlüter A (2015). "Improved genome sequence of the phytopathogenic fungus Rhizoctonia solani AG1-IB 7/3/14 as established by deep mate-pair sequencing on the MiSeq (Illumina) system". J. Biotechnol. 203: 19–21. doi:10.1016/j.jbiotec.2015.03.005. PMID   25801332.