Summary: Ribonucleotide reductase, small chain
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Ribonucleotide reductase Edit Wikipedia article
|PDB structures||RCSB PDB PDBe PDBsum|
|Gene Ontology||AmiGO / QuickGO|
Ribonucleotide reductase (RNR), also known as ribonucleoside diphosphate reductase (rNDP), is an enzyme that catalyzes the formation of deoxyribonucleotides from ribonucleotides. Deoxyribonucleotides in turn are used in the synthesis of DNA. The reaction catalyzed by RNR is strictly conserved in all living organisms. Furthermore, RNR plays a critical role in regulating the total rate of DNA synthesis so that DNA to cell mass is maintained at a constant ratio during cell division and DNA repair. A somewhat unusual feature of the RNR enzyme is that it catalyzes a reaction that proceeds via a free radical mechanism of action. The substrates for RNR are ADP, GDP, CDP and UDP. dTDP (deoxythymidine diphosphate) is synthesized by another enzyme (thymidylate kinase) from dTMP (deoxythymidine monophosphate).
The iron-dependent enzyme, ribonucleotide reductase (RNR), is essential for DNA synthesis. Class I RNR enzymes are constructed from large RNR1 and small RNR2 subunits which associate to form an active heterodimeric tetramer. Since the enzyme catalyses the de novo synthesis of deoxyribonucleotides (dNTPs), precursors to DNA synthesis, it is essential for cell proliferation.
In humans, the RNR1 subunit is encoded by the RRM1 gene while there are two isoforms of the RNR2 subunit, encoded by the RRM2 and RRM2B genes:
- one mainly helical domain comprising the 220 N-terminal residues,
- a second large ten-stranded α/β structure comprising 480 residues,
- and a third small five-stranded α/β structure comprising 70 residues.
In Pfam, the second domain has been interpreted as two separate domains:
- a shorter all-alpha N-terminal domain,
- and a longer barrel C-terminal domain.
RNR2 contains a diferric iron center and a stable tyrosyl radical. In E. coli, the tyrosyl radical is located at position 122 (Y122) providing the stable radical for the Class I RNR2 subunits. In A. aegypti, this tyrosyl radical is located at position 184 (Y184). The tyrosyl radical is deeply buried inside the protein in a hydrophobic environment, located close to the iron center that is used in the stabilization of a tyrosyl radical. The structure of two μ-oxo-linked irons is dominated by ligands that serve as iron binding sites: four carboxylates [aspartate (D146), glutamate (E177, E240, and E274)] and two histidines (H180 and H277). Association occurs between the C-terminus of RNR2 and the C-terminus of RNR1. Enzymatic activity is dependent on association of the RNR1 and RNR2 subunits. The active site consists of the active dithiol groups from the RNR1 as well as the diferric center and the tyrosyl radical from the RNR2 subunit.
Other residues of RNR2, such as aspartate (D273), tryptophan (W48), and tyrosine (Y356) further stabilize the active-site tyrosyl radical thus allowing electron transfer. These residues help in the transfer of the radical electron from tyrosine (Y122) of RNR2 to cysteine (C439) of RNR1. The electron transfer begins on RNR2 tyrosine (Y122) and continues in RNR2 to tryptophan (W48), which is separated from RNR1 tyrosine (Y731) by 2.5 nanometers. Electron transfer from RNR2 to RNR1 occurs via tyrosine (Y356 to Y731) and continues on through tyrosine (Y730) to cysteine (C439) in the active site. Site-directed mutations of the RNR primary structure indicate that all residues cited above participate in the long distance transfer of the free radical to the active site.
In A. aegypti mosquitoes, RNR1 retains most of the crucial amino acid residues, including aspartate (D64) and valine (V292 or V284), that are necessary in allosteric regulation; proline (P210 and P610), leucine (L453 and L473), and methionine (M603) residues that are located in the hydrophobic active site; cysteine (C225, C436 and C451) residues that are involved in removal of a hydrogen atom and transfer of the radical electron at the active site; cysteine (C225 and C436), asparagine (N434), and glutamate (E441) residues that bind the ribonucleotide substrate; tyrosine (Y723 and Y743) residues that dictate the radical transfer; and cysteine (C838 and C841) residues that are used in the regeneration of dithiol groups in the active site.
The enzyme ribonucleotide reductase (RNR) catalyzes the de novo synthesis of dNDPs. Catalysis of ribonucleoside 5’-diphosphates (NDPs) involves a reduction at the 2’-carbon of ribose 5-phosphate to form the 2’-deoxy derivative-reduced 2’-deoxyribonucleoside 5’-diphosphates (dNDPs). This reduction is initiated with the generation of a free radical. Following a single reduction, RNR requires electrons donated from the dithiol groups of the protein thioredoxin. Regeneration of thioredoxin occurs when nicotinamide adenine dinucleotide phosphate (NADPH) provides two hydrogen atoms that are used to reduce the disulfide groups of thioredoxin.
Three classes of RNR have similar mechanisms for the reduction of NDPs, but differ in the domain that generates the free radical, the specific metal in the metalloprotein structure, and the electron donors. All classes use free-radical chemistry. Class I reductases use an iron center with ferrous to ferric conversion to generate a tyrosyl free radical. Reduction of NDP substrates occurs under aerobic conditions. Class I reductases are divided into IA and IB due to differences in regulation. Class IA reductases are distributed in eukaryotes, eubacteria, bacteriophages, and viruses. Class IB reductases are found in eubacteria. Class IB reductases can also use a radical generated with the stabilization of a binuclear manganese center. Class II reductases generate a free radical by mechanisms involving 5’-deoxyadenosyl cobalamin (coenzyme B12) and have a simpler structure than class I and class III reductases. Reduction of NDPs or ribonucleotide 5’-triphosphates (NTPs) occurs under either aerobic or anaerobic conditions. Class II reductases are distributed in archaebacteria, eubacteria, and bacteriophages. Class III reductases use a glycine radical generated with the help of an S-adenosyl methionine and an iron sulphur center. Reduction of NTPs is limited to anaerobic conditions. Class III reductases are distributed in archaebacteria, eubacteria, and bacteriophages. Organisms are not limited to having one class of enzymes. For example, E. coli have both class I and class III RNR.
Catalytic reduction mechanism
The mechanism that is currently accepted for the reduction of ribonucleotides to deoxyribonucleotides is depicted in the following scheme. The first step involves the abstraction of the 3’- H of substrate 1 by radical Cys439. Subsequently, the reaction involves the elimination of one water molecule from carbon C-2’ of the ribonucleotide, catalyzed by Cys225 and Glu441. In the third step there is a hydrogen atom transfer from Cys225 to carbon C-2’ of the 2’-ketyl radical 3, after previous proton transfer from Cys462 to Cys225. At the end of this step, a radical anionic disulfide bridge and the closed-shell ketone intermediate 4 are obtained. This intermediate has been identified during the conversion of several 2’-substituted substrate analogues, as well as with the natural substrate interacting with enzyme mutants. The next step is the oxidation of the anionic disulfide bridge, with concomitant reduction of the substrate, generating 5. The spin density shifts from the sulphur atoms to the C-3' atom of the substrate, with simultaneous proton transfer from Glu441 to carbon C-3'. The last step is the reverse of the first step and involves a hydrogen transfer from Cys439 to C-3’, regenerating the initial radical and resulting in the final product 6.
Class I RNR comprises RNR1 and RNR2 subunits, which can associate to form a heterodimeric tetramer. RNR1 contains both allosteric sites, mediating regulation of substrate specificity and activity. Depending on the allosteric configuration, one of the four ribonucleotides binds to the active site.
Regulation of RNR is designed to maintain balanced quantities of dNTPs. Binding of effector molecules either increases or decreases RNR activity. When ATP binds to the allosteric activity site, it activates RNR. In contrast, when dATP binds to this site, it deactivates RNR. In addition to controlling activity, the allosteric mechanism also regulates the substrate specificity and ensures the enzyme produces an equal amount of each dNTP for DNA synthesis. In all classes, binding of ATP or dATP to the allosteric site induces reduction of cytidine 5’-diphosphate (CDP) and uridine 5’-diphosphate (UDP); 2’-deoxyguanosine 5’-triphosphate (dGTP) induces reduction of adenosine 5’-diphosphate (ADP); and 2’-deoxythymidine 5’-triphosphate (dTTP) induces reduction of guanosine 5’-diphosphate (GDP) (Figure 1).
Interestingly, class IB reductases are not inhibited by dATP because they lack approximately 50 N-terminal amino acids required for the allosteric activity site. Eukaryotic cells with class IA reductases have a mechanism of negative control to turn off synthesis of dNTPs as they accumulate. This mechanism protects the cell from toxic and mutagenic effects that can arise from the overproduction of dNTPs because changes in balanced dNTP pools lead to DNA damage and cell death.
RNR1 and RNR2 inhibitors
Generally Class I RNR inhibitors can be divided in three main groups: translation inhibitors, which block the synthesis of the enzyme; dimerization inhibitors that prevent the association of the two RNR subunits (R1 and R2); and catalytic inhibitors that inactivate the subunit R1 and/or subunit R2.
Class I RNR can be inhibited by peptides similar to the C-terminus of RNR2. These peptides can compete with RNR2 for binding to RNR1, and as a result RNR1 does not form an enzymatically active complex with RNR2. Although the C-terminus of RNR2 proteins is different across species, RNR2 can interact with RNR1 across species. When the mouse RNR2 C-terminus was replaced with the E. coli RNR2 C-terminal (7 or 33) amino acid residues, the chimeric RNR2 subunit still binds to mouse RNR1 subunits. However, they lack enzymatic activity due probably to the elimination of residues involved in the transfer of the free radical electron from the RNR2 to the RNR1 subunit.
Small peptides can specifically inhibit the RNR2 subunits from binding with RNR1 when they share a significant similarity with the normal RNR2 C-terminus. This inhibition RNR2 binding to RNR1 has been tested successfully in herpes simplex virus (HSV) RNR. When a 7 amino acid oligomer (GAVVNDL) truncated from the C-terminus of the RNR2 subunit was used in competition assays, it prevented the normal RNR2 from forming an enzymatically active complex with RNR1. Other small peptide inhibitors similar to the RNR2 C-terminus have also been used successfully to inhibit HSV RNR enzymatic activity and thus HSV replication. In mice models of stromal keratitis and corneal neovascularization (HSV ocular disease), a small RNR2 C-terminal analog BILD 1263 has been reported to inhibit RNR and is effective in preventing these diseases. In some cases, although treatment with small C-terminal analogs may not stop disease spreading, they can still help in healing. In the acyclovir-resistant HSV (PAAr5), a small peptide inhibitor BILD 1633 has been reported to be 5 to 10 times more potent than BILD 1263 against cutaneous PAAr5 infection. A combination therapy approach (BILD 1633 and acyclovir) is more effective to heal topical lesions in mice. These data suggest that small peptide inhibitors that compete with RNR2 for binding to RNR1 are useful in preventing the spread of HSV.
Gallium inhibits RNR2 by substituting for Fe3+ in the active site. Gallium maltolate is an orally bioavailable form of gallium that exploits this inhibitory activity to treat cancer, infections, and other diseases.
- Elledge SJ, Zhou Z, Allen JB (March 1992). "Ribonucleotide reductase: regulation, regulation, regulation". Trends Biochem. Sci. 17 (3): 119–23. PMID 1412696. doi:10.1016/0968-0004(92)90249-9.
- Torrents E, Aloy P, Gibert I, Rodríguez-Trelles F (August 2002). "Ribonucleotide reductases: divergent evolution of an ancient enzyme". J. Mol. Evol. 55 (2): 138–52. PMID 12107591. doi:10.1007/s00239-002-2311-7.
- Herrick J, Sclavi B (January 2007). "Ribonucleotide reductase and the regulation of DNA replication: an old story and an ancient heritage". Mol. Microbiol. 63 (1): 22–34. PMID 17229208. doi:10.1111/j.1365-2958.2006.05493.x.
- Eklund H, Eriksson M, Uhlin U, Nordlund P, Logan D (August 1997). "Ribonucleotide reductase--structural studies of a radical enzyme". Biol. Chem. 378 (8): 821–5. PMID 9377477. doi:10.1515/bchm.1997.378.8.815.
- Stubbe J, Riggs-Gelasco P (November 1998). "Harnessing free radicals: formation and function of the tyrosyl radical in ribonucleotide reductase". Trends Biochem. Sci. 23 (11): 438–43. PMID 9852763. doi:10.1016/S0968-0004(98)01296-1.
- Jordan A, Reichard P (1998). "Ribonucleotide reductases". Annu. Rev. Biochem. 67 (1): 71–98. PMID 9759483. doi:10.1146/annurev.biochem.67.1.71.
- PMID 12818204. doi:10.1016/S0022-2836(03)00538-2.; Uppsten M, Färnegårdh M, Jordan A, Eliasson R, Eklund H, Uhlin U (June 2003). "Structure of the Large Subunit of Class Ib Ribonucleotide Reductase from Salmonella typhimurium and its Complexes with Allosteric Effectors". J. Mol. Biol. 330 (1): 87–97.
- Uhlin U, Eklund H (August 1994). "Structure of ribonucleotide reductase protein R1". Nature. 370 (6490): 533–9. PMID 8052308. doi:10.1038/370533a0.
- Nordlund P, Eklund H (July 1993). "Structure and Function of the Escherichia coli Ribonucleotide Reductase Protein R2". J. Mol. Biol. 232 (1): 123–64. PMID 8331655. doi:10.1006/jmbi.1993.1374.
- Högbom M, Andersson ME, Nordlund P (March 2001). "Crystal structures of oxidized dinuclear manganese centres in Mn-substituted class I ribonucleotide reductase from Escherichia coli: carboxylate shifts with implications for O2 activation and radical generation". J. Biol. Inorg. Chem. 6 (3): 315–23. PMID 11315567. doi:10.1007/s007750000205.
- Pham DQ, Blachuta BJ, Nichol H, Winzerling JJ (September 2002). "Ribonucleotide reductase subunits from the yellow fever mosquito, Aedes aegypti: cloning and expression". Insect Biochem. Mol. Biol. 32 (9): 1037–44. PMID 12213240. doi:10.1016/S0965-1748(02)00041-3.
- Chang MC, Yee CS, Stubbe J, Nocera DG (May 2004). "Turning on ribonucleotide reductase by light-initiated amino acid radical generation". Proc. Natl. Acad. Sci. U.S.A. 101 (18): 6882–7. PMC . PMID 15123822. doi:10.1073/pnas.0401718101.
- Cox, Michael; Nelson, David R. (2008). Lehninger Principles of Biochemistry. San Francisco: W. H. Freeman. ISBN 0-7167-7108-X.
- Cerqueira NM, Fernandes PA, Eriksson LA, Ramos MJ (December 2004). "Ribonucleotide activation by enzyme ribonucleotide reductase: understanding the role of the enzyme". J Comput Chem. 25 (16): 2031–7. PMID 15481089. doi:10.1002/jcc.20127.
- Cerqueira NM, Pereira S, Fernandes PA, Ramos MJ (2005). "Overview of ribonucleotide reductase inhibitors: an appealing target in anti-tumour therapy". Curr. Med. Chem. 12 (11): 1283–94. PMID 15974997. doi:10.2174/0929867054020981.
- Cerqueira NM, Fernandes PA, Eriksson LA, Ramos MJ (March 2006). "Dehydration of ribonucleotides catalyzed by ribonucleotide reductase: the role of the enzyme". Biophys. J. 90 (6): 2109–19. PMC . PMID 16361339. doi:10.1529/biophysj.104.054627.
- Eliasson R, Pontis E, Jordan A, Reichard P (October 1996). "Allosteric regulation of the third ribonucleotide reductase (NrdEF enzyme) from enterobacteriaceae". J. Biol. Chem. 271 (43): 26582–7. PMID 8900130. doi:10.1074/jbc.271.43.26582.
- Kunz BA (1988). "Mutagenesis and deoxyribonucleotide pool imbalance". Mutat. Res. 200 (1–2): 133–47. PMID 3292903. doi:10.1016/0027-5107(88)90076-0.
- Meuth M (April 1989). "The molecular basis of mutations induced by deoxyribonucleoside triphosphate pool imbalances in mammalian cells". Exp. Cell Res. 181 (2): 305–16. PMID 2647496. doi:10.1016/0014-4827(89)90090-6.
- T. Selwood; E. K. Jaffe. (2011). "Dynamic dissociating homo-oligomers and the control of protein function.". Arch. Biochem. Biophys. 519 (2): 131–43. PMC . PMID 22182754. doi:10.1016/j.abb.2011.11.020.
- Climent I, Sjöberg BM, Huang CY (May 1991). "Carboxyl-terminal peptides as probes for Escherichia coli ribonucleotide reductase subunit interaction: kinetic analysis of inhibition studies". Biochemistry. 30 (21): 5164–71. PMID 2036382. doi:10.1021/bi00235a008.
- Hamann CS, Lentainge S, Li LS, Salem JS, Yang FD, Cooperman BS (March 1998). "Chimeric small subunit inhibitors of mammalian ribonucleotide reductase: a dual function for the R2 C-terminus?". Protein Eng. 11 (3): 219–24. PMID 9613846. doi:10.1093/protein/11.3.219.
- Cosentino G, Lavallée P, Rakhit S, Plante R, Gaudette Y, Lawetz C, Whitehead PW, Duceppe JS, Lépine-Frenette C, Dansereau N (January 1991). "Specific inhibition of ribonucleotide reductases by peptides corresponding to the C-terminal of their second subunit". Biochem. Cell Biol. 69 (1): 79–83. PMID 2043345. doi:10.1139/o91-011.
- Cooperman BS (2003). "Oligopeptide inhibition of class I ribonucleotide reductases". Biopolymers. 71 (2): 117–31. PMID 12767114. doi:10.1002/bip.10397.
- Filatov D, Ingemarson R, Gräslund A, Thelander L (August 1992). "The role of herpes simplex virus ribonucleotide reductase small subunit carboxyl terminus in subunit interaction and formation of iron-tyrosyl center structure". J. Biol. Chem. 267 (22): 15816–22. PMID 1322407.
- Cohen EA, Gaudreau P, Brazeau P, Langelier Y (1986). "Specific inhibition of herpesvirus ribonucleotide reductase by a nonapeptide derived from the carboxy terminus of subunit 2". Nature. 321 (6068): 441–3. PMID 3012360. doi:10.1038/321441a0.
- Brandt CR, Spencer B, Imesch P, Garneau M, Déziel R (May 1996). "Evaluation of a peptidomimetic ribonucleotide reductase inhibitor with a murine model of herpes simplex virus type 1 ocular disease". Antimicrob. Agents Chemother. 40 (5): 1078–84. PMC . PMID 8723444.
- Duan J, Liuzzi M, Paris W, Lambert M, Lawetz C, Moss N, Jaramillo J, Gauthier J, Déziel R, Cordingley MG (July 1998). "Antiviral activity of a selective ribonucleotide reductase inhibitor against acyclovir-resistant herpes simplex virus type 1 in vivo". Antimicrob. Agents Chemother. 42 (7): 1629–35. PMC . PMID 9660995.
- Bernstein LR (1998). "Mechanisms of therapeutic activity for gallium" (PDF). Pharmacol. Rev. 50 (4): 665–682. PMID 9860806.
- "Information on EC 220.127.116.11 - ribonucleoside-diphosphate reductase". Brenda. Retrieved 25 July 2015.
- Hashemy SI, Ungerstedt JS, Zahedi Avval F, Holmgren A (April 2006). "Motexafin gadolinium, a tumor-selective drug targeting thioredoxin reductase and ribonucleotide reductase". J. Biol. Chem. 281 (16): 10691–7. PMID 16481328. doi:10.1074/jbc.M511373200.
This tab holds the annotation information that is stored in the Pfam database. As we move to using Wikipedia as our main source of annotation, the contents of this tab will be gradually replaced by the Wikipedia tab.
Ribonucleotide reductase, small chain Provide feedback
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InterPro entry IPR000358
Ribonucleotide reductase (RNR), also known as ribonucleoside diphosphate reductase, (EC) [PUBMED:3286319, PUBMED:8511586] catalyses the reductive synthesis
of deoxyribonucleotides from their corresponding ribonucleotides:
RNR provides the precursors necessary for DNA synthesis. RNRs divide into three classes on the basis of their metallocofactor usage. Class I RNRs, found in eukaryotes, bacteria, bacteriophage and viruses, use a diiron-tyrosyl radical, Class II RNRs, found in bacteria, bacteriophage, algae and archaea, use coenzyme B12 (adenosylcobalamin, AdoCbl). Class III RNRs, found in anaerobic bacteria and bacteriophage, use an FeS cluster and S-adenosylmethionine to generate a glycyl radical. Many organisms have more than one class of RNR present in their genomes.
Class I ribonucleotide reductase is an oligomeric enzyme composed of a large subunit (700 to 1000 residues) and a small subunit (300 to 400 residues) - class II RNRs are less complex, using the small molecule B12 in place of the small chain [PUBMED:11875520]. The small chain binds two iron atoms [PUBMED:2190093] (three Glu, one Asp, and two His are involved in metal binding) and contains an active site tyrosine radical. The regions of the sequence that contain the metal-binding residues and the active site tyrosine are conserved in ribonucleotide reductase small chain from prokaryotes, eukaryotes and viruses.
This family consist of the small subunit of class I ribonucleotide reductases. It also includes R2-like ligand-binding oxidase, which is homologous to the ribonucleotide reductase small subunit (R2), but whose function is still unknown [PUBMED:19321420, PUBMED:22976985].
The mapping between Pfam and Gene Ontology is provided by InterPro. If you use this data please cite InterPro.
|Biological process||oxidation-reduction process (GO:0055114)|
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The members of this clan all share a distinctive four helical bundle. The four helices are arranged antiparallel with a left-handed twist. This helical bundle is distinguished from others by the long connection between the second and third helices. Some of the members contain a Fe or Mn dimer at the centre of the helical bundle. The ferritin fold was first described by Murzin AG and Chothia C, Cur Opin Struc Biol 1992, 2:895-903.
The clan contains the following 24 members:Ald_deCOase AOX AurF Coat_F COQ7 DUF2202 DUF2383 DUF305 DUF3231 DUF4142 DUF4439 DUF455 DUF892 FA_desaturase_2 Ferritin Ferritin-like Ferritin_2 MiaE MiaE_2 Mn_catalase PaaA_PaaC Phenol_Hydrox Ribonuc_red_sm Rubrerythrin
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|Previous IDs:||ribonuc_red; ribonuc_red_sm;|
|Author:||Finn RD, Griffiths-Jones SR|
|Number in seed:||327|
|Number in full:||4425|
|Average length of the domain:||265.30 aa|
|Average identity of full alignment:||29 %|
|Average coverage of the sequence by the domain:||77.13 %|
|HMM build commands:||
build method: hmmbuild -o /dev/null HMM SEED
search method: hmmsearch -Z 26740544 -E 1000 --cpu 4 HMM pfamseq
|Family (HMM) version:||20|
|Download:||download the raw HMM for this family|
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This chart is a modified "sunburst" visualisation of the species tree for this family. It shows each node in the tree as a separate arc, arranged radially with the superkingdoms at the centre and the species arrayed around the outermost ring.
How the sunburst is generated
The tree is built by considering the taxonomic lineage of each sequence that has a match to this family. For each node in the resulting tree, we draw an arc in the sunburst. The radius of the arc, its distance from the root node at the centre of the sunburst, shows the taxonomic level ("superkingdom", "kingdom", etc). The length of the arc represents either the number of sequences represented at a given level, or the number of species that are found beneath the node in the tree. The weighting scheme can be changed using the sunburst controls.
In order to reduce the complexity of the representation, we reduce the number of taxonomic levels that we show. We consider only the following eight major taxonomic levels:
Colouring and labels
Segments of the tree are coloured approximately according to their superkingdom. For example, archeal branches are coloured with shades of orange, eukaryotes in shades of purple, etc. The colour assignments are shown under the sunburst controls. Where space allows, the name of the taxonomic level will be written on the arc itself.
As you move your mouse across the sunburst, the current node will be highlighted. In the top section of the controls panel we show a summary of the lineage of the currently highlighed node. If you pause over an arc, a tooltip will be shown, giving the name of the taxonomic level in the title and a summary of the number of sequences and species below that node in the tree.
Anomalies in the taxonomy tree
There are some situations that the sunburst tree cannot easily handle and for which we have work-arounds in place.
Missing taxonomic levels
Some species in the taxonomic tree may not have one or more of the main eight levels that we display. For example, Bos taurus is not assigned an order in the NCBI taxonomic tree. In such cases we mark the omitted level with, for example, "No order", in both the tooltip and the lineage summary.
Unmapped species names
The tree is built by looking at each sequence in the full alignment for the family. We take the name of the species given by UniProt and try to map that to the full taxonomic tree from NCBI. In some cases, the name chosen by UniProt does not map to any node in the NCBI tree, perhaps because the chosen name is listed as a synonym or a misspelling in the NCBI taxonomy.
So that these nodes are not simply omitted from the sunburst tree, we group them together in a separate branch (or segment of the sunburst tree). Since we cannot determine the lineage for these unmapped species, we show all levels between the superkingdom and the species as "uncategorised".
Since we reduce the species tree to only the eight main taxonomic levels, sequences that are mapped to the sub-species level in the tree would not normally be shown. Rather than leave out these species, we map them instead to their parent species. So, for example, for sequences belonging to one of the Vibrio cholerae sub-species in the NCBI taxonomy, we show them instead as belonging to the species Vibrio cholerae.
Too many species/sequences
For large species trees, you may see blank regions in the outer layers of the sunburst. These occur when there are large numbers of arcs to be drawn in a small space. If an arc is less than approximately one pixel wide, it will not be drawn and the space will be left blank. You may still be able to get some information about the species in that region by moving your mouse across the area, but since each arc will be very small, it will be difficult to accurately locate a particular species.
The tree shows the occurrence of this domain across different species. More...
We show the species tree in one of two ways. For smaller trees we try to show an interactive representation, which allows you to select specific nodes in the tree and view them as an alignment or as a set of Pfam domain graphics.
Unfortunately we have found that there are problems viewing the interactive tree when the it becomes larger than a certain limit. Furthermore, we have found that Internet Explorer can become unresponsive when viewing some trees, regardless of their size. We therefore show a text representation of the species tree when the size is above a certain limit or if you are using Internet Explorer to view the site.
If you are using IE you can still load the interactive tree by clicking the "Generate interactive tree" button, but please be aware of the potential problems that the interactive species tree can cause.
For all of the domain matches in a full alignment, we count the number that are found on all sequences in the alignment. This total is shown in the purple box.
We also count the number of unique sequences on which each domain is found, which is shown in green. Note that a domain may appear multiple times on the same sequence, leading to the difference between these two numbers.
Finally, we group sequences from the same organism according to the NCBI code that is assigned by UniProt, allowing us to count the number of distinct sequences on which the domain is found. This value is shown in the pink boxes.
We use the NCBI species tree to group organisms according to their taxonomy and this forms the structure of the displayed tree. Note that in some cases the trees are too large (have too many nodes) to allow us to build an interactive tree, but in most cases you can still view the tree in a plain text, non-interactive representation. Those species which are represented in the seed alignment for this domain are highlighted.
You can use the tree controls to manipulate how the interactive tree is displayed:
- show/hide the summary boxes
- highlight species that are represented in the seed alignment
- expand/collapse the tree or expand it to a given depth
- select a sub-tree or a set of species within the tree and view them graphically or as an alignment
- save a plain text representation of the tree
Please note: for large trees this can take some time. While the tree is loading, you can safely switch away from this tab but if you browse away from the family page entirely, the tree will not be loaded.
There are 5 interactions for this family. More...
We determine these interactions using iPfam, which considers the interactions between residues in three-dimensional protein structures and maps those interactions back to Pfam families. You can find more information about the iPfam algorithm in the journal article that accompanies the website.
For those sequences which have a structure in the Protein DataBank, we use the mapping between UniProt, PDB and Pfam coordinate systems from the PDBe group, to allow us to map Pfam domains onto UniProt sequences and three-dimensional protein structures. The table below shows the structures on which the Ribonuc_red_sm domain has been found. There are 215 instances of this domain found in the PDB. Note that there may be multiple copies of the domain in a single PDB structure, since many structures contain multiple copies of the same protein sequence.
Loading structure mapping...