A Microbial Biorealm page on the Chytridiomycota
Higher order taxa:
Eukaryota; Fungi/Metazoa group; Fungi
Batrachochytrium dendrobatidis, Spizellomyces punctatus, Rhizophydium sphaerotheca
Description and Significance
Chytridiomycota are the smallest and simplest fungi. They emerged soon after the Precambrian period, and are ancestors to all Fungi. The first Chitridiomycota were found in northern Russia. There are three orders within Chytridiomycota: Chytridiales, Blastocadiales, and Monoblepharidales.
There are many different species within the classification of Chytridiomycota, and all have different genomes. For example, the species , there are eight mitochondrially-encoded tRNAs, and it is believed that they have at least one base pair mismatch at the first three positions of their aminoacyl acceptor stems. Bullerwell and Gray (2005) have developed a method of tRNA editing using the mitochondiral extract of S. punctatus. 5' tRNA editing occurs in the mitochondria of this species, as well as in the chytridiomycete order Monoblepharidales. However, it does not occur in Rhizophydium brooksianum. Laforest et. al. (2004) believe that 5' tRNA edition evolved twice independently within Chytridiomycota. The genome structure of Batrachochytrium dendrobatidis shows only five variable nucleotide positions, meaning it has a low level of genetic variation. Other characteristics of the B. dendrobatidis genome include nearly fixed heterozygous genotypes as well as chromosome lengtgh polymorphisms. The genes that encode alpha- and beta-tubulins are useful for encoding fungal phylogeny. Corradi et. al. (2004) studied the genetic similarities between members of Chrytidiomycota and arbuscular mycorrhizal fungi (AMF). They found large evolutionary differences at the amino-acid level, but at the mitochondiral level, differences were significantly smaller. Anaerobic chytridiomycetes contain an enzyme called pyruvate formate lyase, which is essential for f.ermentative formate production. This enzyme exists in the genetic structure of only one other eukaryotic lineage, chlorophytes.
Cell Structure and Metabolism
Chytridiomycota have unicellular or mycelial thalli. Cell walls are made of chitin, although one group has walls made of cellulose. Cell growth can be unicellular, or it can occur in the multicellular mycelium of aseptate hyphae. The thallus is typcially unicellular; it may also have limited hyphal growth. It is not considered mycelial. Hyphal cells are coenocytic, although this is not the case where there are reproductive structures. The ultrastructure of the zoospore is a definitve characteristic of Chytridiomycota. In the structure, ribosomes are aggregated around a nucule that is not enclosed in a nuclear cap. A nuclear cap is an extension of the nuclear membrane. Chytridiomycota have one or two flagella.
Chytridiomycota feed on both living and decaying organisms. They are heterotrophic.
Asexually, Chytridiomycota reproduce through the use of zoospores. In asexual reproduction, zoospores will swim until a desireable substrate is located. The zoospore attaches itself, feeds off its host; the cytoplasm grows, meiotic divisions occur, and a cell wall forms around the original zoospore. Protoplasm increases as the cell continues to develop. Finally, cleavage of the protoplasm occurs, which produces individual zoospores that are released through a pore. Sexual reproduction is haploid dominant. It also depends on the isomorphic alternation of generations. The haploid thallus, called the gametothallus, produces female and male gametes. These occur in pairs and are terminal and subterminal. Male gametes are orange-colored, while female gametes are colorless. In addition, female gametes are much larger than male gametes. Males are attracted to females when they produce the hormone sirenin, and females are attracted to males when they produce the hormone parisin.
The diploid thallus is called the sporothallus. The sporothallus produces two types of zoosporgia: zoosporgangium (meitosporangium) and resistant sporangium (meiosporangium). Zoosporangia produce diploid zoospores, which can function as a means of asexual reproduction. Sexual reproduction may be isogamous, anisogamous, or oogamous. One species, Allomyces macrogynus, has a sporic life cycle, something that occurs in plants but is rare to fungi. A. macrogynus is an example of an anisogamous species.
Chytridomycota usually inhabit freshwater ecosystems. In fact, they are dependent on the presence of water to survive. However, Chytridiomycota often dwell within host organisms, which can be plants or animals. They live saprophytically and parasitically. Because Chytridiomycota often feed on decaying organisms, they are important decomposers. While this is an important function, Chytridiomycota can also have a negative impact on human produce, particularly Synchytrium endobioticum, the species that causes potato wart. Others, such as Olpidium brassicae(the "Big Vein" virus in lettuce), are parasitic, but actually do little damage to the host organism as a whole. While this is not true of all species, some, such as Rhizophlyctis rosea and Allomyces anomalus have structures that allow them to survive draughts or excessive heat.
Anaerobic rumen fungi, such as Orpinomyces joyonii, inhabit the guts of cattle, sheep, and goats. These fungi live in anaerobic conditions and play an imporant part in the digestive process. They help process plant matter while obtaining food. They are so effective that they make their hosts some of the most effective animals at utilizing cellulose. In addition, some species of anaerobic rumen fungi are used for other purposes. Xue et. al. (1996) cloned microbial non-starch polysaccharide hydrolases from Neocallimastix patriciarum. They found that the genes within these hydrolases were valuable for the production of genetically-engineered cereal crops.
There is a disease that comes from the Chytridiomycota classification. Chytridiomycosis is a fungal infection of amphibians. The disease is found in keratinised tissue, which includes the mouthparts of tadpoles. One of the main symptoms of chytridiomycosis is a thickened epidermis (hyperkeratosis). It is fatal, and has caused amphibian population decline on several continents. Treatment is possible if the infection is caught early, but not always effective. One important characteristic of chytridiomycosis is the way it behaves at different temperatures. The pathogenicity of the disease is enhanced at lower tempeartures, as is victim mortality rate. The origin of the disease has been unknown for quite some time. However, the work of Weldon et. al. (2004) has posed several theories about the disease. They found that the earliest known case of chytridiomycosis occurred in 1938. They also discovered that this infection existed in Africa for 23 years before any reported cases outside of Africa. They concluded that the fungus originated in Africa, and was introduced to other continents in the mid-1930s.
Through their research with chytridiomycosis, Olsen et. al. (2004) have developed a staining protocol to facilitate the often difficult diagnosis of this disease. The difficulty lies in the invasiveness and insensitivity of standard detection methods, which usually involve taking toe clippings from the amphibian. Other researchers have been working in the field of detection as well. Annis et. al. (2004) have developed a method of detection which is a polymerase chain-reaction based assay. Boyle et. al. (2004) have also developed a new method of detection, a real-time PCR Taquin assay. Van Ells et. al. (2003) developed a method of immunohistochemical staining which proved to be a very effective method of diagnosis, because infected was made highly visible. Some researchers focus on treatment instead of detection. Johnson et. al. (2003) compared the efficacy of chemical disinfectants, UV light, dessication, and heat in treating chytridiomycosis. Most methods were effective; cultures did not survive drying and were sensitive to heat. Chemical treatments were also highly effective, although concentration and exposure were critical factors in their efficacy. The only treatment method that did not work was exposing the cultures to UV light. Other researchers have not looked at either detection or treatment, but instead studied the effects of the virus on community interactions between the gray treefrog, Hyla chrysoscelis, and eastern newts, Notophthalmus viridescens. Their work indicates that the effects are complex and indirect.
Berger L, Speare R, Hines HB, Marantelli G, Hyatt AD, McDonald KR, Skerratt LF, Olsen V, Clarke JM, Gillespie G, Mahony M, Sheppard N, Williams C, Tyler MJ. "Effect of season and temperature on mortality in amphibians due to chytridiomycosis." Australian veterinary journal. 2004 Jul;82(7):434-9.
Boyle DG, Boyle DB, Olsen V, Morgan JA, Hyatt AD. "Rapid quantitative detection of chytridiomycosis (Batrachochytrium dendrobatidis) in amphibian samples using real-time Taqman PCR assay." Diseases of aquatic organisms. 2004 Aug 9;60(2):141-8.
Bullerwell CE, Gray MW. "In vitro characterization of a tRNA editing activity in the mitochondria of Spizellomyces punctatus, a Chytridiomycete fungus." The Journal of biological chemistry. 2005 Jan 28;280(4):2463-70. Epub 2004 Nov 15.
Corradi N, Hijri M, Fumagalli L, Sanders IR. "Arbuscular mycorrhizal fungi (Glomeromycota) harbour ancient fungal tubulin genes that resemble those of the chytrids (Chytridiomycota)." Fungal genetics and biology : FG & B. 2004 Nov;41(11):1037-45.
Gelius-Dietrich G, Henze K. "Pyruvate formate lyase (PFL) and PFL activating enzyme in the chytrid fungus Neocallimastix frontalis: a free-radical enzyme system conserved across divergent eukaryotic lineages." The Journal of eukaryotic microbiology. 2004 Jul-Aug;51(4):456-63.
Johnson ML, Berger L, Philips L, Speare R. "Fungicidal effects of chemical disinfectants, UV light, desiccation and heat on the amphibian chytrid Batrachochytrium dendrobatidis." Diseases of aquatic organisms. 2003 Dec 29;57(3):255-60.
Morehouse EA, James TY, Ganley AR, Vilgalys R, Berger L, Murphy PJ, Longcore JE. "Multilocus sequence typing suggests the chytrid pathogen of amphibians is a recently emerged clone." Molecular ecology. 2003 Feb;12(2):395-403.
Olsen V, Hyatt AD, Boyle DG, Mendez D. "Co-localisation of Batrachochytrium dendrobatidis and keratin for enhanced diagnosis of chytridiomycosis in frogs." Diseases of aquatic organisms. 2004 Oct 21;61(1-2):85-8.
Van Ells T, Stanton J, Strieby A, Daszak P, Hyatt AD, Brown C. "Use of immunohistochemistry to diagnose chytridiomycosis in dyeing poison dart frogs (Dendrobates tinctorius)." Journal of wildlife diseases. 2003 Jul; 39(3): 742-5.