Photosynthetic reaction centre protein family

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Type II reaction centre protein
Photosynthetic Reaction Center Drawing.png
Structure of the photosynthetic reaction centre from Rhodopseudomonas viridis (PDB: 1PRC​). Middle transmembrane section is the two subunits in this family; green blocks represent chlorophyll. Top section is the 4-heme (red) cytochrome c subunit (infobox below). The bottom section along with its connected TM helices is the H subunit.
Identifiers
SymbolPhoto_RC
PfamPF00124
InterProIPR000484
PROSITEPDOC00217
SCOPe1prc / SUPFAM
TCDB3.E.2
OPM superfamily2
OPM protein1dxr
Type I reaction centre protein
1jb0 opm.png
Side view of Cyanobacterial photosystem I. Large near-symmetrical proteins in the center, colored blue and pink, are the two subunits of this family.
Identifiers
SymbolPsaA_PsaB
PfamPF00223
InterProIPR001280
PROSITEPDOC00347
SCOPe1jb0 / SUPFAM
TCDB5.B.4
OPM superfamily2
OPM protein1jb0
Membranome535
Bacterial type II reaction centre, cytochrome c subunit
Identifiers
SymbolCytoC_RC
PfamPF02276
Pfam clanCL0317
InterProIPR003158
SCOPe1prc / SUPFAM

Photosynthetic reaction centre proteins are main protein components of photosynthetic reaction centres (RCs) of bacteria and plants. They are transmembrane proteins embedded in the chloroplast thylakoid or bacterial cell membrane.

Plants have one type of PRC for each of its two photosystems. Non-oxygenic bacteria, on the other hand, have an RC resembling either the Photosystem I centre (Type I) or the Photosystem II centre (Type II). In either case, PRCs have two related proteins (L/M; D1/D2; PsaA/PsaB) making up a qausi-symmetrical 5-helical core complex with pockets for pigment binding. The two types are structually related and share a common ancestor.[1][2] Each type have different pockets for ligands to accomendate their specific reactions: while Type I RCs use iron sulfur clusters to accept electrons, Type II RCs use quinones. The centre units of Type I RCs also have six extra transmembrane helices for gathering energy.[2]

In bacteria[edit]

The Type II photosynthetic apparatus in non-oxygenic bacteria consists of light-harvesting protein-pigment complexes LH1 and LH2, which use carotenoid and bacteriochlorophyll as primary donors.[3] LH1 acts as the energy collection hub, temporarily storing it before its transfer to the photosynthetic reaction centre (RC).[4] Electrons are transferred from the primary donor via an intermediate acceptor (bacteriophaeophytin) to the primary acceptor (quinine Qa), and finally to the secondary acceptor (quinone Qb), resulting in the formation of ubiquinol QbH2. RC uses the excitation energy to shuffle electrons across the membrane, transferring them via ubiquinol to the cytochrome bc1 complex in order to establish a proton gradient across the membrane, which is used by ATP synthetase to form ATP.[5][6][7]

The core complex is anchored in the cell membrane, consisting of one unit of RC surrounded by LH1; in some species there may be additional subunits.[8] A type II RC consists of three subunits: L (light), M (medium), and H (heavy; InterProIPR005652). Subunits L and M provide the scaffolding for the chromophore, while subunit H contains a cytoplasmic domain.[9] In Rhodopseudomonas viridis, there is also a non-membranous tetrahaem cytochrome (4Hcyt) subunit on the periplasmic surface.

The structure for a type I system in the anaerobe Heliobacterium modesticaldum was resolved in 2017 (PDB: 5V8K​). As a homodimer consisting of only one type of protein in the core complex, it is considered a closer example to what an ancestral unit before the Type I/II split is like compared to all heterodimeric systems.[2]

Oxygenic systems[edit]

The D1 (PsbA) and D2 (PsbD) photosystem II (PSII) reaction centre proteins from cyanobacteria, algae and plants only show approximately 15% sequence homology with the L and M subunits, however the conserved amino acids correspond to the binding sites of the photochemically active cofactors. As a result, the reaction centres (RCs) of purple photosynthetic bacteria and PSII display considerable structural similarity in terms of cofactor organisation.

The D1 and D2 proteins occur as a heterodimer that form the reaction core of PSII, a multisubunit protein-pigment complex containing over forty different cofactors, which are anchored in the cell membrane in cyanobacteria, and in the thylakoid membrane in algae and plants. Upon absorption of light energy, the D1/D2 heterodimer undergoes charge separation, and the electrons are transferred from the primary donor (chlorophyll a) via phaeophytin to the primary acceptor quinone Qa, then to the secondary acceptor Qb, which like the bacterial system, culminates in the production of ATP. However, PSII has an additional function over the bacterial system. At the oxidising side of PSII, a redox-active residue in the D1 protein reduces P680, the oxidised tyrosine then withdrawing electrons from a manganese cluster, which in turn withdraw electrons from water, leading to the splitting of water and the formation of molecular oxygen. PSII thus provides a source of electrons that can be used by photosystem I to produce the reducing power (NADPH) required to convert CO2 to glucose.[10][11]

Instead of assigining specialized roles to quinones, the PsaA-PsaB photosystem I centre evolved to make both quinones immobile. It also recruited the iron-sulphur PsaC subunit to further mitigate the risk of oxidative stress.[2]

In viruses[edit]

Photosynthetic reaction centre genes from PSII (PsbA, PsbD) have been discovered within marine bacteriophage.[12][13][14] Though it is widely accepted dogma that arbitrary pieces of DNA can be borne by phage between hosts (transduction), one would hardly expect to find transduced DNA within a large number of viruses. Transduction is presumed to be common in general, but for any single piece of DNA to be routinely transduced would be highly unexpected. Instead, conceptually, a gene routinely found in surveys of viral DNA would have to be a functional element of the virus itself (this does not imply that the gene would not be transferred among hosts - which the photosystem within viruses is[15] - but instead that there is a viral function for the gene, that it is not merely hitchhiking with the virus). However, free viruses lack the machinery needed to support metabolism, let alone photosynthesis. As a result, photosystem genes are not likely to be a functional component of the virus like a capsid protein or tail fibre. Instead, it is expressed within an infected host cell.[16][17] Most virus genes that are expressed in the host context are useful for hijacking the host machinery to produce viruses or for replication of the viral genome. These can include reverse transcriptases, integrases, nucleases or other enzymes. Photosystem components do not fit this mould either. The production of an active photosystem during viral infection provides active photosynthesis to dying cells. This is not viral altruism towards the host, however. The problem with viral infections tends to be that they disable the host relatively rapidly. As protein expression is shunted from the host genome to the viral genome, the photosystem degrades relatively rapidly (due in part to the interaction with light, which is highly corrosive), cutting off the supply of nutrients to the replicating virus.[18] A solution to this problem is to add rapidly degraded photosystem genes to the virus, such that the nutrient flow is uninhibited and more viruses are produced. One would expect that this discovery will lead to other discoveries of a similar nature; that elements of the host metabolism key to viral production and easily damaged during infection are actively replaced or supported by the virus during infection.

Indeed, recently, PSI gene cassettes containing whole gene suites [(psaJF, C, A, B, K, E and D) and (psaD, C, A and B)] were also reported to exist in marine cyanophages from the Pacific and Indian Oceans [19][20][21]

Subfamilies[edit]

Notes[edit]

  1. ^ Sadekar S, Raymond J, Blankenship RE (November 2006). "Conservation of distantly related membrane proteins: photosynthetic reaction centers share a common structural core". Molecular Biology and Evolution. 23 (11): 2001–7. doi:10.1093/molbev/msl079. PMID 16887904.
  2. ^ a b c d Orf GS, Gisriel C, Redding KE (October 2018). "Evolution of photosynthetic reaction centers: insights from the structure of the heliobacterial reaction center". Photosynthesis Research. 138 (1): 11–37. doi:10.1007/s11120-018-0503-2. PMID 29603081.
  3. ^ Lancaster CR, Bibikova MV, Sabatino P, Oesterhelt D, Michel H (December 2000). "Structural basis of the drastically increased initial electron transfer rate in the reaction center from a Rhodopseudomonas viridis mutant described at 2.00-A resolution". The Journal of Biological Chemistry. 275 (50): 39364–8. doi:10.1074/jbc.M008225200. PMID 11005826.
  4. ^ Bahatyrova S, Frese RN, Siebert CA, Olsen JD, Van Der Werf KO, Van Grondelle R, Niederman RA, Bullough PA, Otto C, Hunter CN (August 2004). "The native architecture of a photosynthetic membrane" (PDF). Nature. 430 (7003): 1058–62. Bibcode:2004Natur.430.1058B. doi:10.1038/nature02823. PMID 15329728.
  5. ^ Scheuring S (October 2006). "AFM studies of the supramolecular assembly of bacterial photosynthetic core-complexes". Current Opinion in Chemical Biology. 10 (5): 387–93. doi:10.1016/j.cbpa.2006.08.007. PMID 16931113.
  6. ^ Remy A, Gerwert K (August 2003). "Coupling of light-induced electron transfer to proton uptake in photosynthesis". Nature Structural Biology. 10 (8): 637–44. doi:10.1038/nsb954. PMID 12872158.
  7. ^ Deisenhofer J, Michel H (August 1989). "Nobel lecture. The photosynthetic reaction centre from the purple bacterium Rhodopseudomonas viridis". The EMBO Journal. 8 (8): 2149–70. doi:10.1002/j.1460-2075.1989.tb08338.x. PMC 401143. PMID 2676514.
  8. ^ Miki K, Kobayashi M, Nogi T, Fathir I, Nozawa T (2000). "Crystal structures of photosynthetic reaction center and high-potential iron-sulfur protein from Thermochromatium tepidum: thermostability and electron transfer". Proc. Natl. Acad. Sci. U.S.A. 97 (25): 13561–13566. Bibcode:2000PNAS...9713561N. doi:10.1073/pnas.240224997. PMC 17615. PMID 11095707.
  9. ^ Michel H, Ermler U, Schiffer M (1994). "Structure and function of the photosynthetic reaction center from Rhodobacter sphaeroides". J. Bioenerg. Biomembr. 26 (1): 5–15. doi:10.1007/BF00763216. PMID 8027023.
  10. ^ Kamiya N, Shen JR (2003). "Crystal structure of oxygen-evolving photosystem II from Thermosynechococcus vulcanus at 3.7-A resolution". Proc. Natl. Acad. Sci. U.S.A. 100 (1): 98–103. doi:10.1073/pnas.0135651100. PMC 140893. PMID 12518057.
  11. ^ Schroder WP, Shi LX (2004). "The low molecular mass subunits of the photosynthetic supracomplex, photosystem II". Biochim. Biophys. Acta. 1608 (2–3): 75–96. doi:10.1016/j.bbabio.2003.12.004. PMID 14871485.
  12. ^ Sharon I, Tzahor S, Williamson S, Shmoish M, Man-Aharonovich D, Rusch DB, Yooseph S, Zeidner G, Golden SS, Mackey SR, Adir N, Weingart U, Horn D, Venter JC, Mandel-Gutfreund Y, Béjà O (2007). "Viral photosynthetic reaction center genes and transcripts in the marine environment". ISME J. 1 (6): 492–501. doi:10.1038/ismej.2007.67. PMID 18043651.
  13. ^ Millard A, Clokie MR, Shub DA, Mann NH (2004). "Genetic organization of the psbAD region in phages infecting marine Synechococcus strains". Proc. Natl. Acad. Sci. U.S.A. 101 (30): 11007–12. Bibcode:2004PNAS..10111007M. doi:10.1073/pnas.0401478101. PMC 503734. PMID 15263091.
  14. ^ Sullivan MB, Lindell D, Lee JA, Thompson LR, Bielawski JP, Chisholm SW (2006). "Prevalence and evolution of core photosystem II genes in marine cyanobacterial viruses and their hosts". PLoS Biol. 4 (8): e234. doi:10.1371/journal.pbio.0040234. PMC 1484495. PMID 16802857. open access
  15. ^ Lindell D, Sullivan MB, Johnson ZI, Tolonen AC, Rohwer F, Chisholm SW (2004). "Transfer of photosynthesis genes to and from Prochlorococcus viruses". Proc. Natl. Acad. Sci. U.S.A. 101 (30): 11013–8. Bibcode:2004PNAS..10111013L. doi:10.1073/pnas.0401526101. PMC 503735. PMID 15256601.
  16. ^ Lindell D, Jaffe JD, Johnson ZI, Church GM, Chisholm SW (2005). "Photosynthesis genes in marine viruses yield proteins during host infection". Nature. 438 (7064): 86–9. Bibcode:2005Natur.438...86L. doi:10.1038/nature04111. PMID 16222247.
  17. ^ Clokie MR, Shan J, Bailey S, Jia Y, Krisch HM, West S, Mann NH (2006). "Transcription of a 'photosynthetic' T4-type phage during infection of a marine cyanobacterium". Environ. Microbiol. 8 (5): 827–35. doi:10.1111/j.1462-2920.2005.00969.x. PMID 16623740.
  18. ^ Bailey S, Clokie MR, Millard A, Mann NH (2004). "Cyanophage infection and photoinhibition in marine cyanobacteria". Res. Microbiol. 155 (9): 720–5. doi:10.1016/j.resmic.2004.06.002. PMID 15501648.
  19. ^ Sharon I, Alperovitch A, Rohwer F, Haynes M, Glaser F, Atamna-Ismaeel N, Pinter RY, Partensky F, Koonin EV, Wolf YI, Nelson N, Béjà O (2009). "Photosystem-I gene cassettes are present in marine virus genomes". Nature. 461 (7261): 258–262. Bibcode:2009Natur.461..258S. doi:10.1038/nature08284. PMC 4605144. PMID 19710652.
  20. ^ Alperovitch-Lavy A, Sharon I, Rohwer F, Aro EM, Glaser F, Milo R, Nelson N, Béjà O (2011). "Reconstructing a puzzle: existence of cyanophages containing both photosystem-I and photosystem-II gene suites inferred from oceanic metagenomic datasets". Environ. Microbiol. 13 (1): 24–32. doi:10.1111/j.1462-2920.2010.02304.x. PMID 20649642.
  21. ^ Béjà O, Fridman S, Glaser F (2012). "Viral clones from the GOS expedition with an unusual photosystem-I gene cassette organization". ISME J. 6 (8): 1617–20. doi:10.1038/ismej.2012.23. PMC 3400403. PMID 22456446.

References[edit]

  • Deisenhofer J, Epp O, Miki K, Huber R, Michel H (December 1984). "X-ray structure analysis of a membrane protein complex. Electron density map at 3 A resolution and a model of the chromophores of the photosynthetic reaction center from Rhodopseudomonas viridis". Journal of Molecular Biology. 180 (2): 385–98. doi:10.1016/s0022-2836(84)80011-x. PMID 6392571.