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. 2004 Dec 6;290(1):179–185. doi: 10.1016/0003-9861(91)90605-I

Phospholipid vesicles containing bovine heart mitochondrial cytochrome c oxidase exhibit proton translocating activity in the presence of gramicidin☆

Lawrence J Prochaska 1,2, Kathryn S Wilson 1,3
PMCID: PMC7124189  PMID: 1716878

Abstract

Phospholipid vesicles containing bovine heart mitochondrial cytochrome c oxidase (COV) were characterized for electron transfer and proton translocating activities in the presence of the mobile potassium ionophore, valinomycin, and the channel-forming ionophore, gramicidin, in order to determine if the ionophores modify the functional properties of the enzyme. In agreement with previous work, incubation of COV with valinomycin resulted in a perturbation of the absorbance spectrum of oxidized heme aa3 in the Soret region (430 nm); gramicidin had no effect on the heme aa3 absorbance spectrum. Different concentrations of the two ionophores were required for maximum respiratory control ratios in COV; 40- to 70-fold higher concentrations of valinomycin were required to completely uncouple electron transfer activity when compared to gramidicin. The proton translocating activity of COV incubated with each ionophore gave a similar apparent proton translocated to electron transferred stoichiometry (H+e− ratio) of 0.66 ± 0.10. However, COV treated with low concentrations of gramicidin (0.14 mg/g phospholipid) exhibited 1.5- to 2.5-fold higher rates of alkalinization of the extravesicular media after the initial proton translocation reaction than did COV treated with valinomycin, suggesting that gramicidin allows more rapid equilibration of protons across the phospholipid bilayer during the proton translocation assay. Moreover, at higher concentrations of gramicidin (1.4 mg/g phospholipid), the observed H+e− ratio decreased to 0.280 ± 0.020, while the rate of alkalinization increased an additional 2-fold, suggesting that at higher concentrations, gramicidin acts as a proton ionophore. These results support the hypothesis that cytochrome c oxidase is a redox-linked proton pump that operates at similar efficiencies in the presence of either ionophore. Low concentrations of gramicidin dissipate the membrane potential in COV most likely by a channel mechanism that is different from the carrier mechanism of valinomycin, yet does not make the phospholipid bilayer freely permeable to protons.

Footnotes

☆

Supported by a grant from the American Heart Association—Ohio Affiliate.

References

  • 1.Capaldi R.A. Annu. Rev. Biochem. 1990;59:569–596. doi: 10.1146/annurev.bi.59.070190.003033. [DOI] [PubMed] [Google Scholar]
  • 2.Wikstrom M.K.F., Saari H.T. Biochim. Biophys. Acta. 1977;462:347–361. doi: 10.1016/0005-2728(77)90133-5. [DOI] [PubMed] [Google Scholar]
  • 3.Krab K., Wikstrom M. Biochim. Biophys. Acta. 1978;504:200–214. doi: 10.1016/0005-2728(78)90018-x. [DOI] [PubMed] [Google Scholar]
  • 4.Casey R.P., Azzi A. FEBS Lett. 1983;154:237–242. doi: 10.1016/0014-5793(83)80156-2. [DOI] [PubMed] [Google Scholar]
  • 5.Wikstrom M. Nature (London) 1984;308:558–560. doi: 10.1038/308558a0. [DOI] [PubMed] [Google Scholar]
  • 6.Thelen M., O'Shea P.S., Petrone G., Azzi A. J. Biol. Chem. 1985;260:3626–3631. [PubMed] [Google Scholar]
  • 7.Proteau G., Wrigglesworth J.M., Nicholls P. Biochem. J. 1983;210:199–205. doi: 10.1042/bj2100199. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 8.Nicholls P., Shaughnessy S. Biochem. J. 1985;228:201–210. doi: 10.1042/bj2280201. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 9.Moroney P., Scholes T.A., Hinkle P.C. Biochemistry. 1984;23:4991–4997. doi: 10.1021/bi00316a025. [DOI] [PubMed] [Google Scholar]
  • 10.Singh A.P., Nicholls P. Arch. Biochem. Biophys. 1986;245:436–445. doi: 10.1016/0003-9861(86)90235-3. [DOI] [PubMed] [Google Scholar]
  • 11.Pressman B.C. Annu. Rev. Biochem. 1976;45:501–531. doi: 10.1146/annurev.bi.45.070176.002441. [DOI] [PubMed] [Google Scholar]
  • 12.Steverding D., Kadenbach B. Biochem. Biophys. Res. Commun. 1990;160:1132–1139. doi: 10.1016/s0006-291x(89)80121-4. [DOI] [PubMed] [Google Scholar]
  • 13.Steverding D., Kadenbach B. J. Bioenerg. Biomembr. 1990;22:197–205. doi: 10.1007/BF00762946. [DOI] [PubMed] [Google Scholar]
  • 14.Gregory L.C., Ferguson-Miller S. Biochemistry. 1989;28:2655–2662. doi: 10.1021/bi00432a044. [DOI] [PubMed] [Google Scholar]
  • 15.Nicholls P., Cooper C.E., Kjarsgaard J. In: Advances in Membrane Biochemistry and Bioenergetics. Kim C.H., Tedeschi H., Diwan J.J., Salerno J.C., editors. A. R. Liss; New York: 1988. pp. 311–321. [Google Scholar]
  • 16.Wilson K.S., Prochaska L.J. Arch. Biochem. Biophys. 1990;282:413–420. doi: 10.1016/0003-9861(90)90137-n. [DOI] [PubMed] [Google Scholar]
  • 17.Andersen O.S. Annu. Rev. Physiol. 1984;46:531–548. doi: 10.1146/annurev.ph.46.030184.002531. [DOI] [PubMed] [Google Scholar]
  • 18.Wallace B.A. Annu. Rev. Biophys. Chem. 1990;19:127–157. doi: 10.1146/annurev.bb.19.060190.001015. [DOI] [PubMed] [Google Scholar]
  • 19.Azzone G.F., Colonna R., Ziche B. In: 3rd ed. Fleischer S., Packer L., editors. Vol. 55. Academic Press; New York: 1979. pp. 46–50. (Methods in Enzymology). [DOI] [PubMed] [Google Scholar]
  • 20.Yonetani T. In: 3rd ed. Estabrook R.W., Pullman M.E., editors. Vol. 10. Academic Press; New York: 1967. pp. 332–336. (Methods in Enzymology). [Google Scholar]
  • 21.Briggs M.M., Capaldi R.A. Biochemistry. 1977;16:73–77. doi: 10.1021/bi00620a012. [DOI] [PubMed] [Google Scholar]
  • 22.Van Gelder B.F. Biochim. Biophys. Acta. 1966;118:36–48. doi: 10.1016/s0926-6593(66)80142-x. [DOI] [PubMed] [Google Scholar]
  • 23.Margoliash E., Frohwirt N. Biochem. J. 1959;71:570–577. doi: 10.1042/bj0710570. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Lowry O.H., Rosebrough N.J., Farr A.L., Randall R.J. J. Biol. Chem. 1951;193:265–275. [PubMed] [Google Scholar]
  • 25.DiBiase V.A., Prochaska L.J. Arch. Biochem. Biophys. 1985;243:668–677. doi: 10.1016/0003-9861(85)90545-4. [DOI] [PubMed] [Google Scholar]
  • 26.Nicholls P., Hildebrandt V., Wrigglesworth J.M. Arch. Biochem. Biophys. 1980;204:533–543. doi: 10.1016/0003-9861(80)90065-x. [DOI] [PubMed] [Google Scholar]
  • 27.Prochaska L.J., Reynolds K.A. Biochemistry. 1986;25:781–787. doi: 10.1021/bi00352a007. [DOI] [PubMed] [Google Scholar]
  • 28.Bauer K., Roskoski R., Kleinkauf H., Lipmann F. Biochemistry. 1972;11:3266–3271. doi: 10.1021/bi00767a022. [DOI] [PubMed] [Google Scholar]
  • 29.Casey R.P. In: 3rd ed. Fleischer S., Fleischer B., editors. Vol. 126. Academic Press; New York: 1986. pp. 13–21. (Methods in Enzymology). [Google Scholar]
  • 30.Wrigglesworth J.M., Cooper C.C., Sharpe M.A., Nicholls P. Biochem. J. 1990;270:109–118. doi: 10.1042/bj2700109. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 31.Mueller M., Azzi A. J. Bioenerg. Biomembr. 1985;17:385–393. doi: 10.1007/BF00743111. [DOI] [PubMed] [Google Scholar]
  • 32.Hladky S.B., Haydon D.A. Biochim. Biophys. Acta. 1972;274:294–312. doi: 10.1016/0005-2736(72)90178-2. [DOI] [PubMed] [Google Scholar]
  • 33.Myers V.B., Haydon D.A. Biochim. Biophys. Acta. 1972;274:312–322. doi: 10.1016/0005-2736(72)90179-4. [DOI] [PubMed] [Google Scholar]
  • 34.Deamer D.W. J. Bioenerg. Biomembr. 1987;19:457–479. doi: 10.1007/BF00770030. [DOI] [PubMed] [Google Scholar]
  • 35.Casey R.P., Chappell J.B., Azzi A. Biochem. J. 1979;182:149–156. doi: 10.1042/bj1820149. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 36.Bano M.C., Braco L., Abad C. Biochemistry. 1991;30:886–894. doi: 10.1021/bi00218a002. [DOI] [PubMed] [Google Scholar]
  • 37.O'Connell A.M., Koeppe R.E., Andersen O.S. Science. 1990;250:1256–1259. doi: 10.1126/science.1700867. [DOI] [PubMed] [Google Scholar]
  • 38.Clement N.R., Gould J.M. Biochemistry. 1981;20:1544–1548. doi: 10.1021/bi00509a021. [DOI] [PubMed] [Google Scholar]

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