Isolation of F1-ATPase from the Parasitic Protist Trypanosoma brucei
Summary
This protocol describes the purification of F1-ATPase from the cultured insect stage of Trypanosoma brucei. The procedure yields a highly pure, homogeneous, and active complex suitable for structural and enzymatic studies.
Abstract
F1-ATPase is a membrane-extrinsic catalytic subcomplex of F-type ATP synthase, an enzyme that uses the proton motive force across biological membranes to produce adenosine triphosphate (ATP). The isolation of the intact F1-ATPase from its native source is an essential prerequisite to characterize the enzyme's protein composition, kinetic parameters, and sensitivity to inhibitors. A highly pure and homogeneous F1-ATPase can be used for structural studies, which provide insight into molecular mechanisms of ATP synthesis and hydrolysis. This article describes a procedure for the purification of the F1-ATPase from Trypanosoma brucei, the causative agent of African trypanosomiases. The F1-ATPase is isolated from mitochondrial vesicles, which are obtained by hypotonic lysis from in vitro cultured trypanosomes. The vesicles are mechanically fragmented by sonication and the F1-ATPase is released from the inner mitochondrial membrane by the chloroform extraction. The enzymatic complex is further purified by consecutive anion exchange and size-exclusion chromatography. Sensitive mass spectrometry techniques showed that the purified complex is devoid of virtually any protein contaminants and, therefore, represents suitable material for structure determination by X-ray crystallography or cryo-electron microscopy. The isolated F1-ATPase exhibits ATP hydrolytic activity, which can be inhibited fully by sodium azide, a potent inhibitor of F-type ATP synthases. The purified complex remains stable and active for at least three days at room temperature. Precipitation by ammonium sulfate is used for long-term storage. Similar procedures have been used for the purification of F1-ATPases from mammalian and plant tissues, yeasts, or bacteria. Thus, the presented protocol can serve as a guideline for the F1-ATPase isolation from other organisms.
Introduction
The F-type ATP synthases are membrane-bound rotating multiprotein complexes that couple proton translocation across energy-transducing membranes of bacteria, mitochondria, and chloroplasts with the formation of ATP. Molecular details of the rotational mechanism of ATP synthesis are known mainly because of structural studies of purified bacterial and mitochondrial ATP synthases and their subcomplexes1. F-type ATP synthase is organized into membrane-intrinsic and membrane-extrinsic moieties. The membrane-extrinsic part, known as F1-ATPase, contains three catalytic sites, where the phosphorylation of adenosine diphosphate (ADP) to ATP or the reverse reaction occurs. F1-ATPase can be released experimentally from the membrane-intrinsic moiety while retaining its ability to hydrolyze, but not synthesize, ATP. The membrane-bound sector, called Fo, mediates protein translocation, which drives the rotation of the central part of the enzyme. The F1 and Fo sectors are connected by the central and peripheral stalks.
The first attempts to purify the F1-ATPase from budding yeast and bovine heart mitochondria date back to the 1960s. These protocols used extracted mitochondria, which were disrupted by sonication, fractionated by ammonium or protamine sulfate precipitation, followed by optional chromatography step(s) and heat treatment2,3,4,5,6. The purification was greatly improved and simplified by the use of chloroform, which readily releases the F1-ATPase from the mitochondrial membrane fragments7. The chloroform extraction was then used to extract F1-ATPases from various animal, plant, and bacterial sources (e.g., rat liver8, corn9, Arum maculatum10, and Escherichia coli11). Further purification of the chloroform-released F1-ATPase by affinity or size-exclusion chromatography (SEC) yielded a highly pure protein complex, which was suitable for high-resolution structure determination by X-ray crystallography, as documented by the structures of F1-ATPase from bovine heart12,13 and Saccharomyces cerevisiae14. F1-ATPase structures were also determined from organisms that are difficult to cultivate and, thus, the amount of the initial biological material was limited. In this case, the F1-ATPase subunits were artificially expressed and assembled into the complex in E. coli, and the whole heterologous enzyme was purified by affinity chromatography via a tagged subunit. Such approach led to the determination of F1-ATPase structures from two thermophilic bacterial species, Geobacillus stearothermophilus15 and Caldalkalibacillus thermarum16,17. However, this methodology is rather unsuitable for eukaryotic F1-ATPases since it relies on the prokaryotic protheosynthetic apparatus, posttranslational processing, and complex assembly.
The chloroform-based extraction was previously used to isolate F1-ATPases from unicellular digenetic parasites Trypanosoma cruzi18 and T. brucei19, important mammalian pathogens causing American and African trypanosomiases, respectively, and from monogenic insect parasite Crithidia fasciculata20. These purifications led only to a simple description of the F1-ATPases, since no downstream applications were used to fully characterize the composition, structure, and enzymatic properties of the complex. This article describes an optimized method for F1-ATPase purification from the cultured insect life cycle stage of T. brucei. The method is developed based on the established protocols for isolation of bovine and yeast F1-ATPases21,22. The procedure yields highly pure and homogeneous enzyme suitable for in vitro enzymatic and inhibitory assays, detailed proteomic characterization by mass spectrometry23, and structure determination24. The purification protocol and the knowledge of the F1-ATPase structure at the atomic level opens a possibility to design screens to identify small-molecule inhibitors, and aid in the development of new drugs against African trypanosomiases. Moreover, the protocol can be adapted to purify F1-ATPase from other organisms.
Protocol
1. Buffers and Solutions
- Prepare the solutions listed below. Degas all buffers for liquid chromatography. Add ADP, benzamidine, and protease inhibitors just before use.
- Prepare buffer A: 50 mM Tris buffer with hydrochloric acid (Tris-HCl) pH 8.0, 0.25 M sucrose, 5 mM benzamidine, 5 mM aminocaproic acid (ACA), and protease inhibitors (10 µM amastatin, 50 µM bestatin, 50 µM pepstatin, 50 µM leupeptin, and 50 µM diprotin A).
- Prepare buffer B: 50 mM Tris-HCl pH 8.0, 0.25 M sucrose, 4 mM ethylenediaminetetraacetic acid (EDTA), 5 mM benzamidine, 5 mM ACA, 1 mM ADP, and protease inhibitors (10 µM amastatin, 50 µM bestatin, 50 µM pepstatin, 50 µM leupeptin, and 50 µM diprotin A).
- Prepare Q-column buffer: 20 mM Tris-HCl pH 8.0, 4 mM EDTA, 10 mM MgSO4, 5 mM benzamidine, 5 mM ACA, and 1 mM ADP.
- Prepare Q-column elution buffer: Q-column buffer with 1 M NaCl.
- Prepare SEC buffer: 20 mM Tris-HCl pH 8.0, 10 mM MgSO4, 100 mM NaCl, 1 mM ADP.
- Prepare chloroform saturated with 2 M Tris-HCl pH 8.5. Mix chloroform with 2 M Tris-HCl pH 8.5 in approximately 1:1 ratio in a screw-cap bottle, shake, let the organic and aqueous phases separate, and measure pH in the upper aqueous layer with a strip of pH-indicator paper. Store at room temperature. Just before use, shake again and let the phases separate. Use the lower chloroform layer.
CAUTION: Chloroform is volatile and irritating to eyes and skin. Work in a fume hood. Use safety spectacles when shaking.
2. Preparation of sub-mitochondrial Particles
- Resuspend mitochondrial vesicles (mitoplasts) isolated by hypotonic lysis25 from 1 x 1011 to 2 x 1011 cells of procyclic T. brucei in 5 mL of ice-cold buffer A. Keep the sample chilled until step 3.2.
- Determine the protein concentration in the suspension by the bicinchoninic acid (BCA) protein assay26 according to the manufacturer's instructions.
- Use a bovine serum albumin (BSA) dilution series in ultrapure water to construct the standard curve. Dilute a small amount of sample 20 – 100 times with ultrapure water to fit into the range of BSA standards.
- Calculate the total protein amount in the sample and bring the protein concentration to 16 mg/mL by diluting it with additional buffer A.
- Fragment mitoplasts into inverted vesicles and membrane pieces by sonication of the suspension 7x for 15 s with a total energy of 70 to 100 J per impulse with a microtip with a diameter of 3.9 mm. If the ultrasonic homogenizer does not display the energy output, start the optimization at 50% of the maximal power. Incubate the sample on ice for 30 s between impulses. After the sonication, the suspension becomes slightly darker.
- Sediment the membrane fragments by ultracentrifugation at 54,000 x g for 16 h or at 98,000 x g for 5 h at 4 °C. Decant the supernatant and proceed with the chloroform extraction, or flash-freeze the sediment in liquid nitrogen and store it at -80 °C.
3. Release of F1-ATPase from Membrane by Chloroform
- Resuspend the pellet of mitochondrial membranes in buffer B with the aid of a small Dounce homogenizer. Calculate the volume of buffer B based on the total amount of buffer A used in steps 2.1 and 2.2 using the following formula: volume (buffer B) = volume (buffer A) x 12/21. Transfer the suspension to a 15- or 50-mL conical tube.
- Remove the sample from ice and, from now on, keep the sample and all solutions to be used at room temperature.
- Add chloroform saturated with 2 M Tris-HCl pH 8.5; the volume of chloroform to be added equals half the volume of the suspension. Close the cap tightly. Shake it vigorously for exactly 20 s. Centrifuge it immediately at 8,400 x g for 5 min at room temperature.
- Transfer the upper cloudy aqueous phase to 1.6-mL microtubes. Add protease inhibitors (10 µM amastatin, 50 µM bestatin, 50 µM pepstatin, 50 µM leupeptin, and 50 µM diprotin A) to replace the inhibitors removed by the chloroform treatment. Centrifuge the samples at 13,000 x g for 30 min at room temperature. Transfer the supernatant to fresh microtubes and repeat the centrifugation to remove any insoluble material.
4. Anion-exchange Chromatography
- Equilibrate the 5-mL anion exchange (Q) column attached to a fast-protein liquid chromatography system with the Q-column buffer at a flow rate of 5 mL/min until the absorbance at 280 nm and the conductivity stabilize (approximately 50 mL of buffer).
- Load the supernatant from step 3.3 on the equilibrated column at a flow rate of 1 mL/min. Wait until the absorbance at 280 nm stabilizes at the background. Apply a 25-mL linear gradient of the Q-column elution buffer from 0% to 100% at a flow rate of 0.5 mL/min. Collect 1-mL fractions.
- Assay the individual fractions corresponding to the major elution peak for ATP hydrolytic activity by the Pullman ATPase assay2 at pH 8.0. Use 10 µL of each fraction per 1 mL of reaction mixture.Pool the fractions that exhibit ATPase activity. Optionally, separate 10 µL of each fraction on sodium dodecyl phosphate polyacrylamide gel electrophoresis (SDS-PAGE) and stain the gel by Coomassie Blue to visualize individual F1-ATPase subunits and contaminating proteins.
- Concentrate the pooled sample by membrane ultrafiltration using a spin column with a 100,000 MWCO PES filter to 200 – 500 µL. Proceed to SEC or store the sample overnight at room temperature.
5. Size-exclusion Chromatography
- Equilibrate the SEC column attached to a liquid chromatography system with at least 48 mL (two column volumes) of the SEC buffer at a flow rate of 0.5 mL/min.
- Apply the sample on the column and run chromatography at a flow rate of 0.25 mL/min. Collect 0.25-mL fractions.
- Run 10 µL of the fractions that correspond to the peaks of the UV280nm absorbance trace on SDS-PAGE and stain them by Coomassie Blue. The first major peak contains the F1-ATPase. Assay the fractions corresponding to this peak for the ATP hydrolytic activity and azide sensitivity by the Pullman ATPase assay. Determine the protein concentration by the BCA assay.
- Keep the purified F1-ATPase at room temperature and use it within 3 d after purification for downstream applications. Alternatively, concentrate the sample using a spin column with a 100,000 MWCO PES filter to > 1.5 mg/mL, precipitate it by mixing it with saturated ammonium sulfate adjusted to pH 8.0 (1.2x the volume), and store it at 4 °C.
Representative Results
A typical purification (Figure 1) starts with mitochondrial vesicles (mitoplasts) isolated on the Percoll gradient from hypotonically lysed 1 x 1011 to 2 x 1011 procyclic T. brucei cells25 cultured in standard glucose-rich SDM-79 medium27. The mitoplasts are fragmented by sonication, spun, and the matrix-containing supernatant is discarded. Mitochondrial membranes are treated with chloroform to release the F1-ATPase. After centrifugation, the organic phase and precipitated interphase are discarded. The aqueous phase is fractionated by ion-exchange chromatography on quaternary ammonium, a strong anion exchanger (Figure 2A). The fractions that correspond to the major elution peak and contain the F1-ATPase are pooled and concentrated. This material serves as the input for SEC, which eliminates residual impurities. The major contaminant is dihydrolipoyl dehydrogenase, which elutes from the SEC column as a discrete peak, marked by the dark green bar in Figure 2B. The F1-ATPase elutes in the first dominant, largely symmetric peak (Figure 2B).
The progress of purification is followed by the BCA protein assay (or another common protein assay), SDS-PAGE, and the monitoring of ATPase activity. The rate of ATP hydrolysis is measured by the Pullman ATP regenerating assay2, based on the decrease of absorbance of NADH in the coupled reaction. Sodium azide, an established inhibitor of F1-ATPase, is used at a 2-mM concentration to determine the proportion of the F1-ATPase-specific ATP hydrolysis. Typically, the input material contains roughly 150 – 300 mg of mitochondrial protein, depending on the number of cells used as the source of mitochondrial vesicles. The azide-sensitive proportion of the total ATPase activity is around 30% to 40% at this stage. After the chloroform extraction, more than 90% of ATPase activity in the sample is contributed to the F1-ATPase. The purified F1-ATPase is virtually completely sensitive to the azide treatment (the minimal residual ATPase activity can be attributed to the background ATP autolysis) and represents around 1% of the input protein mass, with an approximate yield of 1 – 1.5 mg of F1-ATPase per 1 x 1011 cells (Table 1). A typical band pattern after the separation of the purified F1-ATPase on SDS-PAGE gel followed by Coomassie Blue staining is shown in Figure 2C. The proteins were identified by peptide mass fingerprinting and characterized in detail by various mass spectrometry approaches23. Sporadic weak bands visible above the β-subunit band represent subcomplexes of the α3β3 headpiece (dimers and oligomers of α- and β-subunits) and are devoid of any contaminants detectable by sensitive mass spectrometry techniques. The purified F1-ATPase can be stored for up to several days in the SEC buffer at room temperature. Alternatively, the F1-ATPase concentrated to ≥2 mg/mL can be precipitated by an equal volume of saturated ammonium sulfate in the SEC buffer, with pH adjusted to 8.0, and stored at 4 °C. For at least six months after the precipitation, the active enzyme with no obvious degradation of any subunit can be obtained by redissolving the precipitated material in the SEC buffer or similar solution. However, storage longer than one month is not suitable for crystallization, as determined empirically.
Figure 1: Scheme of the purification procedure. Please click here to view a larger version of this figure.
Figure 2: Two-step purification of the chloroform-released F1-ATPase by liquid chromatography. (A) Elution profile of anion-exchange chromatography (upper panel) and selected fractions separated on the 10% – 20% Tris-glycine SDS-PAGE gel stained with Coomassie Blue dye (lower panel). Blue trace: UV absorbance at 280 nm; red trace: concentration of NaCl in the elution buffer; Input: the F1-ATPase released by chloroform; FT: flow-through. (B) Elution profile of SEC (upper panel) and selected fractions separated on the SDS-PAGE gel stained with Coomassie Blue dye (lower panel). Input: pooled fractions from anion-exchange chromatography containing F1-ATPase. The color-coded bars in panels A and B mark the fractions in the elution profiles that were analyzed by SDS-PAGE and the corresponding lanes in the respective gel. (C) Identities of individual proteins of the isolated F1-ATPase as identified by mass spectrometry. Please click here to view a larger version of this figure.
| Protein concentration (mg/mL) | Total protein (mg) | Proportion of input material (%) | Activity (μmolATP x mg-1 x min-1) |
Azide sensitivity (%) | |
| Mitochondrial vesicles in buffer A | 16.2 | 170 | 100 | 1.3 | 25-35 |
| Mitochondrial membranes in buffer B | 18.6 | 97 | 57 | 2.4 | 35-45 |
| Chloroform extracted fractions | 2.5 | 7.9 | 4.7 | 12 | 91-95 |
| F1-ATPase after Q-column | – | 2.2 | 1.3 | 23 | 92-96 |
| F1-ATPase after gel filtration | – | 1.6 | 0.93 | 48 | 93-98 |
Table 1: An example of the typical progress and yield of the F1-ATPase purification from mitochondria isolated from 1 x 1011 procyclic T. brucei cells.
Discussion
The protocol for F1-ATPase purification from T. brucei was developed based on previously published methods for the isolation of F1-ATPase complexes from other species13,14. The method does not require any genetic modification (e.g., tagging) and yields a fully active complex with all subunits present. The crucial step is the chloroform-facilitated release of the F1-ATPase from the membrane-attached part of the enzyme. In purifications from all eukaryotic species described so far, the released subcomplex contained subunits α, β, γ, δ, and ε in a stoichiometry of 3:3:1:1:1. In T. brucei, the F1-ATPase contains an additional three copies of the subunit p18, a novel component restricted to euglenozoan protists23. Furthermore, the euglenozoan α-subunit is proteolytically split into two fragments, both stably associated with the complex24,28,29. The subunit OSCP (oligomycin-sensitivity-conferring protein), which links the F1-moiety to the peripheral stalk30, is absent from the released complex, which is in agreement with F1-ATPase purifications by chloroform extraction from other species13,14.
The chloroform-released F1-ATPase is further purified by liquid chromatography. In the case of the bovine F1-ATPase, only one chromatography step, size-exclusion chromatography, suffices to obtain a highly pure and active complex31. However, the single SEC set-up was insufficient for the purification of the T. brucei F1-ATPase, as the fractions enriched for F1-ATPase contained additional protein contaminants, mainly delta-1-pyrroline-5-carboxylate dehydrogenase. Therefore, anion-exchange chromatography was introduced before the SEC as the first and major purifying step, and the SEC serves as the subsequent polishing procedure. For crystallization experiments, the use of the Superdex 200 Increase column proved to be essential, since this column provided material that allowed growing crystals of good quality. It is likely that the resolution of the column enabled the separation of a small proportion of incomplete complexes that interfered with crystallization. However, for applications other than crystallization, the separation using the Superdex 200 column was equally satisfactory.
To protect the F1-ATPase complex from partial proteolysis by unknown protease(s) present in the mitochondrial lysate, the initial buffers A and B contained a wide range of protease inhibitors. The impact of individual inhibitors on the proteolysis of F1-ATPase subunits has not been tested and, most likely, the presence of some of the inhibitors is redundant. For the SEC step, the inhibitors are not added anymore, as the contaminating proteases are removed from the F1-ATPase sample by the chloroform extraction or the first chromatography step.
The multistep protocol inevitably leads to partial losses of the F1-ATPase. The most significant loss (25% – 45% of the total amount) occurs during the concentration step by membrane ultrafiltration on a spin column after the anion-exchange chromatography. The F1-ATPase likely adheres to the membrane of the spin column. Thus, for some downstream applications that do not demand a highly pure and concentrated sample (e.g., enzymatic assays and inhibitory screens), the F1-ATPase can be used immediately after the anion-exchange chromatography (see Figure 2B, Input lane).
Although the purification of F1-ATPase from different organisms varies in detail, the general workflow remains the same. Therefore, this protocol can serve as a guideline for the development of the F1-ATPase isolation protocol of other abundant sources, such as tissues or cells cultivatable on a large scale.
Disclosures
The authors have nothing to disclose.
Acknowledgements
This work was funded by the Ministry of Education ERC CZ grant LL1205, the Grant Agency of Czech Republic grant 18-17529S, and by ERDF/ESF project Centre for research of pathogenicity and virulence of parasites (No. CZ.02.1.01/0.0/0.0/16_019/0000759).
Materials
| Chemicals | |||
| Adenosin Diphosphate Disodium Salt (ADP) | Applichem | A0948 | |
| Amastatin Hydrochloride | Glantham Life Sciences | GA1330 | |
| Aminocaproic Acid | Applichem | A2266 | |
| BCA Protein Assay Kit | ThermoFischer Scientific/Pierce | 23225 | |
| Benzamidine Hydrochloride | Calbiochem | 199001 | |
| Bestatin Hydrochloride | Sigma Aldrich/Merck | B8385 | |
| Chloroform | Any supplier | ||
| cOmplete Tablets, Mini EDTA-free | Roche | 4693159001 | Protease inhibitor cocktail tablets |
| Ethylenediaminetetraacetic Acid (EDTA) | Any supplier | ||
| Hydrochloric Acid | Any supplier | For pH adjustment | |
| Ile-Pro-Ile | Sigma Aldrich/Merck | I9759 | Alias Diprotin A |
| Leupeptin | Sigma Aldrich/Merck | L2884 | |
| Magnesium Sulfate Heptahydrate | Any supplier | ||
| Pepstatin A | Sigma Aldrich/Merck | P5318 | |
| Protein Electrophoresis System | Any supplier | ||
| Sodium Chloride | Any supplier | ||
| Sucrose | Any supplier | ||
| Tris | Any supplier | ||
| Name | Company | Catalog Number | Comments |
| Consumables | |||
| Centrifuge Tubes for SW60Ti, Polyallomer | Beckman Coulture | 328874 | |
| DounceTissues Homogenizer 2 mL | Any supplier | ||
| Glass Vacuum Filtration Device | Sartorius | 516-7017 | Degasing solutions for liquid chromatography |
| HiTrap Q HP, 5 mL | GE Healthcare Life Sciences | 17115401 | Anion exchange chromatography column |
| Regenaretad Cellulose Membrane Filters, pore size 0.45 μm, diameter 47 mm | Sartorius | 18406–47——N | Degasing solutions for liquid chromatography |
| Superdex 200 Increase 10/300 GL | GE Healthcare Life Sciences | 29091596 | Size-exclusion chromatography column |
| Vivaspin 6 MWCO 100 kDa PES | Sartorius | VS0641 | |
| Name | Company | Catalog Number | Comments |
| Equipment | |||
| AKTA Pure 25 | GE Healthcare Life Sciences | 29018224 | Or similar FPLC system |
| Spectrophotometer Shimadzu UV-1601 | Shimadzu | Or similar spectrophotometer with kinetic assay mode | |
| Ultracentrifuge Beckman Optima with SW60Ti Rotor | Beckman Coulture | Or similar ultracentrifuge and rotor | |
| Ultrasonic Homogenizer with Thin Probe, Model 3000 | BioLogics | 0-127-0001 | Or similar ultrasonic homogenizer |
References
- Walker, J. E., Wikström, M. Structure, mechanism and regulation of ATP synthases. Mechanisms of Primary Energy Transduction in Biology. , 338-373 (2017).
- Pullman, M. E., Penefsky, H. S., Datta, A., Racker, E. Partial resolution of the enzymes catalyzing oxidative phosphorylation. I. Purification and properties of soluble dinitrophenol-stimulated adenosine triphosphatase. The Journal of Biological Chemistry. 235, 3322-3329 (1960).
- Schatz, G., Penefsky, H. S., Racker, E. Partial resolution of the enzymes catalyzing oxidative phosphorylation. XIV. The Journal of Biological Chemistry. 242 (10), 2552-2560 (1967).
- Racker, E., Horstman, L. L. Partial resolution of the enzymes catalyzing oxidative phosphorylation. 13. Structure and function of submitochondrial particles completely resolved with respect to coupling factor. The Journal of Biological Chemistry. 242 (10), 2547-2551 (1967).
- Senior, A. E., Brooks, J. C. Studies on the mitochondrial oligomycin-insensitive ATPase. I. An improved method of purification and the behavior of the enzyme in solutions of various depolymerizing agents. Archives of Biochemistry and Biophysics. 140 (1), 257-266 (1970).
- Tzagoloff, A., Meagher, P. Assembly of the mitochondrial membrane system. V. Properties of a dispersed preparation of the rutamycin-sensitive adenosine triphosphatase of yeast mitochondria. The Journal of Biological Chemistry. 246 (23), 7328-7336 (1971).
- Beechey, R. B., Hubbard, S. A., Linnett, P. E., Mitchell, A. D., Munn, E. A. A simple and rapid method for the preparation of adenosine triphosphatase from submitochondrial particles. Biochemical Journal. 148 (3), 533-537 (1975).
- Tyler, D. D., Webb, P. R. Purification and properties of the adenosine triphosphatase released from the liver mitochondrial membrane by chloroform. Biochemical Journal. 178 (2), 289-297 (1979).
- Hack, E., Leaver, C. J. The alpha-subunit of the maize F1-ATPase is synthesised in the mitochondrion. The EMBO Journal. 2 (10), 1783-1789 (1983).
- Dunn, P. P., Slabas, A. R., Moore, A. L. Purification of F1-ATPase from cuckoo-pint (Arum maculatum) mitochondria. A comparison of subunit composition with that of rat liver F1-ATPase. Biochemical Journal. 225 (3), 821-824 (1985).
- Satre, M., Bof, M., Vignais, P. V. Interaction of Escherichia coli adenosine triphosphatase with aurovertin and citreoviridin: inhibition and fluorescence studies. Journal of Bacteriology. 142 (3), 768-776 (1980).
- Abrahams, J. P., Leslie, A. G., Lutter, R., Walker, J. E. Structure at 2.8 Å resolution of F1ATPase from bovine heart mitochondria. Nature. 370 (6491), 621-628 (1994).
- Lutter, R., et al. Crystallization of F1-ATPase from bovine heart mitochondria. Journal of Molecular Biology. 229 (3), 787-790 (1993).
- Kabaleeswaran, V., Puri, N., Walker, J. E., Leslie, A. G., Mueller, D. M. Novel features of the rotary catalytic mechanism revealed in the structure of yeast F1-ATPase. The EMBO Journal. 25 (22), 5433-5442 (2006).
- Shirakihara, Y., et al. Structure of a thermophilic F1-ATPase inhibited by an epsilon-subunit: deeper insight into the epsilon-inhibition mechanism. The FEBS Journal. 282 (15), 2895-2913 (2015).
- Stocker, A., Keis, S., Cook, G. M., Dimroth, P. Purification, crystallization, and properties of F1-ATPase complexes from the thermoalkaliphilic Bacillus sp. strain TA2.A1. Journal of Structural Biology. 152 (2), 140-145 (2005).
- Ferguson, S. A., Cook, G. M., Montgomery, M. G., Leslie, A. G., Walker, J. E. Regulation of the thermoalkaliphilic F1-ATPase from Caldalkalibacillus thermarum. Proceedings of the National Academy of Sciences of the United States of America. 113 (39), 10860-10865 (2016).
- Cataldi de Flombaum, M. A., Frasch, A. C. C., Stoppani, A. O. M. Adenosine triphosphatase from Trypanosoma cruzi: purification and properties. Comparative Biochemistry and Physiology Part B: Comparative Biochemistry. 65 (1), 103-109 (1980).
- Williams, N., Frank, P. H. The mitochondrial ATP synthase of Trypanosoma brucei: isolation and characterization of the intact F1 moiety. Molecular and Biochemical Parasitology. 43 (1), 125-132 (1990).
- Higa, A. I., Cazzulo, J. J. Mg2+-activated adenosine triphosphatase from Crithidia fasciculata: purification and inhibition by suramin and efrapeptin. Molecular and Biochemical Parasitology. 3 (6), 357-367 (1981).
- Walker, J. E., et al. Primary structure and subunit stoichiometry of F1-ATPase from bovine mitochondria. Journal of Molecular Biology. 184 (4), 677-701 (1985).
- Mueller, D. M., et al. Ni-chelate-affinity purification and crystallization of the yeast mitochondrial F1-ATPase. Protein Expression and Purification. 37 (2), 479-485 (2004).
- Gahura, O., et al. The F1-ATPase from Trypanosoma brucei is elaborated by three copies of an additional p18-subunit. The FEBS Journal. 285 (3), 614-628 (2018).
- Montgomery, M. G., Gahura, O., Leslie, A. G. W., Zikova, A., Walker, J. E. ATP synthase from Trypanosoma brucei has an elaborated canonical F1-domain and conventional catalytic sites. Proceedings of the National Academy of Sciences of the United States of America. 115 (9), 2102-2107 (2018).
- Schneider, A., Charriere, F., Pusnik, M., Horn, E. K. Isolation of mitochondria from procyclic Trypanosoma brucei. Methods in Molecular Biology. 372, 67-80 (2007).
- Smith, P. K., et al. Measurement of protein using bicinchoninic acid. Analytical Biochemistry. 150 (1), 76-85 (1985).
- Wirtz, E., Leal, S., Ochatt, C., Cross, G. A. A tightly regulated inducible expression system for conditional gene knock-outs and dominant-negative genetics in Trypanosoma brucei. Molecular and Biochemical Parasitology. 99 (1), 89-101 (1999).
- Speijer, D., et al. Characterization of the respiratory chain from cultured Crithidia fasciculata. Molecular and Biochemical Parasitology. 85 (2), 171-186 (1997).
- Nelson, R. E., Aphasizheva, I., Falick, A. M., Nebohacova, M., Simpson, L. The I-complex in Leishmania tarentolae is an uniquely-structured F1-ATPase. Molecular and Biochemical Parasitology. 135 (2), 221-224 (2004).
- Carbajo, R. J., et al. How the N-terminal domain of the OSCP subunit of bovine F1Fo-ATP synthase interacts with the N-terminal region of an alpha subunit. Journal of Molecular Biology. 368 (2), 310-318 (2007).
- Bowler, M. W., Montgomery, M. G., Leslie, A. G., Walker, J. E. Ground state structure of F1-ATPase from bovine heart mitochondria at 1.9 Å resolution. The Journal of Biological Chemistry. 282 (19), 14238-14242 (2007).
