151
|
Uchihashi T, Scheuring S. Applications of high-speed atomic force microscopy to real-time visualization of dynamic biomolecular processes. Biochim Biophys Acta Gen Subj 2018; 1862:229-240. [DOI: 10.1016/j.bbagen.2017.07.010] [Citation(s) in RCA: 33] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/04/2017] [Accepted: 07/13/2017] [Indexed: 12/12/2022]
|
152
|
Structure and dynamics of rotary V 1 motor. Cell Mol Life Sci 2018; 75:1789-1802. [PMID: 29387903 PMCID: PMC5910484 DOI: 10.1007/s00018-018-2758-3] [Citation(s) in RCA: 12] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/03/2017] [Revised: 12/25/2017] [Accepted: 01/18/2018] [Indexed: 12/14/2022]
Abstract
Rotary ATPases are unique rotary molecular motors that function as energy conversion machines. Among all known rotary ATPases, F1-ATPase is the best characterized rotary molecular motor. There are many high-resolution crystal structures and the rotation dynamics have been investigated in detail by extensive single-molecule studies. In contrast, knowledge on the structure and rotation dynamics of V1-ATPase, another rotary ATPase, has been limited. However, recent high-resolution structural studies and single-molecule studies on V1-ATPase have provided new insights on how the catalytic sites in this molecular motor change its conformation during rotation driven by ATP hydrolysis. In this review, we summarize recent information on the structural features and rotary dynamics of V1-ATPase revealed from structural and single-molecule approaches and discuss the possible chemomechanical coupling scheme of V1-ATPase with a focus on differences between rotary molecular motors.
Collapse
|
153
|
Optimum Substrates for Imaging Biological Molecules with High-Speed Atomic Force Microscopy. Methods Mol Biol 2018; 1814:159-179. [PMID: 29956232 DOI: 10.1007/978-1-4939-8591-3_10] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/26/2022]
Abstract
Recent progresses in high-speed atomic force microscopy (HS-AFM) have enabled us to directly visualize dynamic processes of various proteins in liquid conditions. One of the key factors leading to successful HS-AFM observations is the selection of an appropriate substrate depending on molecules to be observed. For the HS-AFM imaging, a target molecule must be absorbed on a substrate by controlling its orientation without impairing the dynamics or physiological function of the molecule. In this chapter, we describe protocols for preparation of substrates that have been used for HS-AFM and then introduce observation examples on dynamic processes of biological molecules.
Collapse
|
154
|
Li J, He G, Hiroshi U, Liu W, Noji H, Qi C, Guo X. Direct Measurement of Single-Molecule Adenosine Triphosphatase Hydrolysis Dynamics. ACS NANO 2017; 11:12789-12795. [PMID: 29215860 DOI: 10.1021/acsnano.7b07639] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/07/2023]
Abstract
F1-ATPase (F1) is a bidirectional molecular motor that hydrolyzes nearly all ATPs to fuel the cellular processes. Optical observation of labeled F1 rotation against the α3β3 hexamer ring revealed the sequential mechanical rotation steps corresponding to ATP binding/ADP release and ATP hydrolysis/Pi release. These substeps originate from the F1 rotation but with heavy load on the γ shaft due to fluorescent labeling and the photophysical limitation of an optical microscope, which hampers better understanding of the intrinsic kinetic behavior of ATP hydrolysis. In this work, we present a method capable of electrically monitoring ATP hydrolysis of a single label-free F1 in real time by using a high-gain silicon nanowire-based field-effect transistor circuit. We reproducibly observe the regular current signal fluctuations with two distinct levels, which are induced by the binding dwell and the catalytic dwell, respectively, in both concentration- and temperature-dependent experiments. In comparison with labeled F1, the hydrolysis rate of nonlabeled F1 used in this study is 1 order of magnitude faster (1.69 × 108 M-1 s-1 at 20 °C), and the differences between two sequential catalytic rates are clearer, demonstrating the ability of nanowire nanocircuits to directly probe the intrinsic dynamic processes of the biological activities with single-molecule/single-event sensitivity. This approach is complementary to traditional optical methods, offering endless opportunities to unravel molecular mechanisms of a variety of dynamic biosystems under realistic physiological conditions.
Collapse
Affiliation(s)
- Jie Li
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University , Beijing 100875, P. R. China
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University , Beijing 100871, P. R. China
| | - Gen He
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University , Beijing 100875, P. R. China
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University , Beijing 100871, P. R. China
| | - Ueno Hiroshi
- Department of Applied Chemistry, School of Engineering, The University of Tokyo , Tokyo 113-8654, Japan
| | - Wenzhe Liu
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University , Beijing 100871, P. R. China
| | - Hiroyuki Noji
- Department of Applied Chemistry, School of Engineering, The University of Tokyo , Tokyo 113-8654, Japan
| | - Chuanmin Qi
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University , Beijing 100875, P. R. China
| | - Xuefeng Guo
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University , Beijing 100871, P. R. China
- Department of Materials Science and Engineering, College of Engineering, Peking University , Beijing 100871, P. R. China
| |
Collapse
|
155
|
Ando T. High-speed atomic force microscopy and its future prospects. Biophys Rev 2017; 10:285-292. [PMID: 29256119 DOI: 10.1007/s12551-017-0356-5] [Citation(s) in RCA: 98] [Impact Index Per Article: 14.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/03/2017] [Accepted: 11/16/2017] [Indexed: 10/18/2022] Open
Abstract
Various techniques have been developed and used to investigate how proteins produce complex biological architectures and phenomena. Among these techniques, high-speed atomic force microscopy (HS-AFM) holds a unique position. It is only HS-AFM that allows the simultaneous assessment of structure and dynamics of single protein molecules in action. This new microscopy tool has been successfully applied to a variety of proteins, from motor proteins to membrane proteins, antibodies, enzymes, and even to intrinsically disordered proteins. And yet there still remain many biomolecular phenomena that cannot be addressed by HS-AFM in its current form. Here, I present a brief history of HS-AFM development, describe the current state of HS-AFM, and then discuss which new biological scanning probe microscopy techniques will be coming up next.
Collapse
Affiliation(s)
- Toshio Ando
- Nano-Life Science Institute, Kanazawa University, Kakuma-machi, Kanazawa, 920-1192, Japan. .,Core Research for Evolutionary Science and Technology (CREST), Japan Science and Technology Agency (JST), Tokyo, 102-0075, Japan.
| |
Collapse
|
156
|
Ogawa T, Hirokawa N. Multiple analyses of protein dynamics in solution. Biophys Rev 2017; 10:299-306. [PMID: 29204883 DOI: 10.1007/s12551-017-0354-7] [Citation(s) in RCA: 7] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/03/2017] [Accepted: 11/15/2017] [Indexed: 12/22/2022] Open
Abstract
The need for accurate description of protein behavior in solution has gained importance in various fields, including biophysics, biochemistry, structural biology, drug discovery, and antibody drugs. To achieve the desired accuracy, multiple precise analyses should be performed on the target molecule, compared, and effectively combined. This review focuses on the combination of multiple analyses in solution: size-exclusion chromatography (SEC), multi-angle light scattering (MALS), small-angle X-ray scattering (SAXS), analytical ultracentrifugation (AUC), and their complementary methods, such as atomic force microscopy (AFM) and mass spectrometry (MS). We also discuss the comparison between the determined molar mass value of not only the standard proteins, but of a target molecule tubulin and its depolymerizing protein, KIF2, as an example. The comparison of the estimated molar mass value from the different methods provides additional information about the target molecule, because the value reflects the dynamically changing states of the target molecule in solution. The combination and integration of multiple methods will permit a deeper understanding of protein dynamics in solution.
Collapse
Affiliation(s)
- Tadayuki Ogawa
- Department of Cell Biology and Anatomy, Graduate School of Medicine, University of Tokyo, 7-3-1 Hongo, Bunkyo-ku, Tokyo, 113-0033, Japan
| | - Nobutaka Hirokawa
- Department of Cell Biology and Anatomy, Graduate School of Medicine, University of Tokyo, 7-3-1 Hongo, Bunkyo-ku, Tokyo, 113-0033, Japan. .,Center of Excellence in Genome Medicine Research, King Abdulaziz University, Jeddah, Saudi Arabia.
| |
Collapse
|
157
|
Dai L, Flechsig H, Yu J. Deciphering Intrinsic Inter-subunit Couplings that Lead to Sequential Hydrolysis of F 1-ATPase Ring. Biophys J 2017; 113:1440-1453. [PMID: 28978438 PMCID: PMC5627347 DOI: 10.1016/j.bpj.2017.08.015] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/02/2017] [Revised: 07/31/2017] [Accepted: 08/04/2017] [Indexed: 11/05/2022] Open
Abstract
Rotary sequential hydrolysis of the metabolic machine F1-ATPase is a prominent manifestation of high coordination among multiple chemical sites in ring-shaped molecular machines, and it is also functionally essential for F1 to tightly couple chemical reactions and central γ-shaft rotation. High-speed AFM experiments have identified that sequential hydrolysis is maintained in the F1 stator ring even in the absence of the γ-rotor. To explore the origins of intrinsic sequential performance, we computationally investigated essential inter-subunit couplings on the hexameric ring of mitochondrial and bacterial F1. We first reproduced in stochastic Monte Carlo simulations the experimentally determined sequential hydrolysis schemes by kinetically imposing inter-subunit couplings and following subsequent tri-site ATP hydrolysis cycles on the F1 ring. We found that the key couplings to support the sequential hydrolysis are those that accelerate neighbor-site ADP and Pi release upon a certain ATP binding or hydrolysis reaction. The kinetically identified couplings were then examined in atomistic molecular dynamics simulations at a coarse-grained level to reveal the underlying structural mechanisms. To do that, we enforced targeted conformational changes of ATP binding or hydrolysis to one chemical site on the F1 ring and monitored the ensuing conformational responses of the neighboring sites using structure-based simulations. Notably, we found asymmetrical neighbor-site opening that facilitates ADP release upon enforced ATP binding. We also captured a complete charge-hopping process of the Pi release subsequent to enforced ATP hydrolysis in the neighbor site, confirming recent single-molecule analyses with regard to the role of ATP hydrolysis in F1. Our studies therefore elucidate both the coordinated chemical kinetics and structural dynamics mechanisms underpinning the sequential operation of the F1 ring.
Collapse
Affiliation(s)
- Liqiang Dai
- Complex System Research Division, Beijing Computational Science Research Center, Beijing, China
| | - Holger Flechsig
- Department of Mathematical and Life Sciences, Graduate School of Science, Hiroshima University, Hiroshima, Japan
| | - Jin Yu
- Complex System Research Division, Beijing Computational Science Research Center, Beijing, China.
| |
Collapse
|
158
|
Dukic M, Todorov V, Andany S, Nievergelt AP, Yang C, Hosseini N, Fantner GE. Digitally controlled analog proportional-integral-derivative (PID) controller for high-speed scanning probe microscopy. THE REVIEW OF SCIENTIFIC INSTRUMENTS 2017; 88:123712. [PMID: 29289234 DOI: 10.1063/1.5010181] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/07/2023]
Abstract
Nearly all scanning probe microscopes (SPMs) contain a feedback controller, which is used to move the scanner in the direction of the z-axis in order to maintain a constant setpoint based on the tip-sample interaction. The most frequently used feedback controller in SPMs is the proportional-integral (PI) controller. The bandwidth of the PI controller presents one of the speed limiting factors in high-speed SPMs, where higher bandwidths enable faster scanning speeds and higher imaging resolution. Most SPM systems use digital signal processor-based PI feedback controllers, which require analog-to-digital and digital-to-analog converters. These converters introduce additional feedback delays which limit the achievable imaging speed and resolution. In this paper, we present a digitally controlled analog proportional-integral-derivative (PID) controller. The controller implementation allows tunability of the PID gains over a large amplification and frequency range, while also providing precise control of the system and reproducibility of the gain parameters. By using the analog PID controller, we were able to perform successful atomic force microscopy imaging of a standard silicon calibration grating at line rates up to several kHz.
Collapse
Affiliation(s)
- Maja Dukic
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| | | | - Santiago Andany
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| | - Adrian P Nievergelt
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| | - Chen Yang
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| | - Nahid Hosseini
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| | - Georg E Fantner
- Laboratory for Bio- and Nano-Instrumentation, School of Engineering, Ecole Polytechnique Federale de Lausanne, Lausanne 1015, Switzerland
| |
Collapse
|
159
|
Benning FMC, Sakiyama Y, Mazur A, Bukhari HST, Lim RYH, Maier T. High-Speed Atomic Force Microscopy Visualization of the Dynamics of the Multienzyme Fatty Acid Synthase. ACS NANO 2017; 11:10852-10859. [PMID: 29023094 DOI: 10.1021/acsnano.7b04216] [Citation(s) in RCA: 13] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/09/2023]
Abstract
Multienzymes, such as the protein metazoan fatty acid synthase (FAS), are giant and highly dynamic molecular machines for critical biosynthetic processes. The molecular architecture of FAS was elucidated by static high-resolution crystallographic analysis, while electron microscopy revealed large-scale conformational variability in FAS with some correlation to functional states in catalysis. However, little is known about time scales of conformational dynamics, the trajectory of motions in individual FAS molecules, and the extent of coupling between catalysis and structural changes. Here, we present an experimental single-molecule approach to film immobilized or selectively tethered FAS in solution at different viewing angles and high spatiotemporal resolution using high-speed atomic force microscopy. Mobility of individual regions of the multienzyme is recognized in video sequences, and correlation of shape features implies a convergence of temporal resolution and velocity of FAS dynamics. Conformational variety can be identified and grouped by reference-free 2D class averaging, enabling the tracking of conformational transitions in movies. The approach presented here is suited for comprehensive studies of the dynamics of FAS and other multienzymes in aqueous solution at the single-molecule level.
Collapse
Affiliation(s)
- Friederike M C Benning
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Yusuke Sakiyama
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Adam Mazur
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Habib S T Bukhari
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Roderick Y H Lim
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Timm Maier
- Biozentrum, ‡Swiss Nanoscience Institute, and §Research IT, Biozentrum, University of Basel , Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| |
Collapse
|
160
|
Li M, Dang D, Xi N, Wang Y, Liu L. Nanoscale imaging and force probing of biomolecular systems using atomic force microscopy: from single molecules to living cells. NANOSCALE 2017; 9:17643-17666. [PMID: 29135007 DOI: 10.1039/c7nr07023c] [Citation(s) in RCA: 25] [Impact Index Per Article: 3.6] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/07/2023]
Abstract
Due to the lack of adequate tools for observation, native molecular behaviors at the nanoscale have been poorly understood. The advent of atomic force microscopy (AFM) provides an exciting instrument for investigating physiological processes on individual living cells with molecular resolution, which attracts the attention of worldwide researchers. In the past few decades, AFM has been widely utilized to investigate molecular activities on diverse biological interfaces, and the performances and functions of AFM have also been continuously improved, greatly improving our understanding of the behaviors of single molecules in action and demonstrating the important role of AFM in addressing biological issues with unprecedented spatiotemporal resolution. In this article, we review the related techniques and recent progress about applying AFM to characterize biomolecular systems in situ from single molecules to living cells. The challenges and future directions are also discussed.
Collapse
Affiliation(s)
- Mi Li
- State Key Laboratory of Robotics, Shenyang Institute of Automation, Chinese Academy of Sciences, Shenyang 110016, China.
| | | | | | | | | |
Collapse
|
161
|
Kozai T, Sekiguchi T, Satoh T, Yagi H, Kato K, Uchihashi T. Two-step process for disassembly mechanism of proteasome α7 homo-tetradecamer by α6 revealed by high-speed atomic force microscopy. Sci Rep 2017; 7:15373. [PMID: 29133893 PMCID: PMC5684232 DOI: 10.1038/s41598-017-15708-8] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/26/2017] [Accepted: 10/31/2017] [Indexed: 01/06/2023] Open
Abstract
The 20S proteasome is a core particle of the eukaryotic proteasome responsible for proteolysis and is composed of layered α and β hetero-heptameric rings. The α7 subunit, which is one of components of the α ring, is known to self-assemble into a double-ringed homo-tetradecamer composed of two layers of the α7 heptameric ring. The α7 tetradecamer is known to disassemble upon the addition of α6 subunit, producing a 1:7 hetero-octameric α6-α7 complex. However, the detailed disassembly mechanism remains unclear. Here, we applied high-speed atomic force microscopy (HS-AFM) to dissect the disassembly process of the α7 double ring caused by interaction with the α6. HS-AFM movies clearly demonstrated two different modes of interaction in which the α6 monomer initially cracks at the interface between the stacked two α7 single rings and the subsequent intercalation of the α6 monomer in the open pore of the α7 single ring blocks the re-association of the single rings into the double ring. This result provides a mechanistic insight about the disassembly process of non-native homo-oligomers formed by proteasome components which is crucial for the initial process for assembly of 20S proteasome.
Collapse
Affiliation(s)
- Toshiya Kozai
- College of Science and Engineering, Kanazawa University, Kakuma, Kanazawa, Ishikawa, 920-1192, Japan
| | - Taichiro Sekiguchi
- Faculty and Graduate School of Pharmaceutical Sciences, Nagoya City University, 3-1 Tanabe-dori, Mizuho-ku, Nagoya, Aichi, 467-8603, Japan
| | - Tadashi Satoh
- Faculty and Graduate School of Pharmaceutical Sciences, Nagoya City University, 3-1 Tanabe-dori, Mizuho-ku, Nagoya, Aichi, 467-8603, Japan
| | - Hirokazu Yagi
- Faculty and Graduate School of Pharmaceutical Sciences, Nagoya City University, 3-1 Tanabe-dori, Mizuho-ku, Nagoya, Aichi, 467-8603, Japan
| | - Koichi Kato
- Faculty and Graduate School of Pharmaceutical Sciences, Nagoya City University, 3-1 Tanabe-dori, Mizuho-ku, Nagoya, Aichi, 467-8603, Japan. .,Okazaki Institute for Integrative Bioscience and Institute for Molecular Science, National Institutes of Natural Sciences, 5-1 Higashiyama, Myodaiji, Okazaki, Aichi, 444-8787, Japan.
| | - Takayuki Uchihashi
- Department of Physics, Nagoya University, Furo-cho, Chikusa-ku, Nagoya, Aichi, 464-8602, Japan. .,CREST, JST (Japan Science and Technology), Kawaguchi, Saitama, 332-0012, Japan.
| |
Collapse
|
162
|
Shibata M, Nishimasu H, Kodera N, Hirano S, Ando T, Uchihashi T, Nureki O. Real-space and real-time dynamics of CRISPR-Cas9 visualized by high-speed atomic force microscopy. Nat Commun 2017; 8:1430. [PMID: 29127285 PMCID: PMC5681550 DOI: 10.1038/s41467-017-01466-8] [Citation(s) in RCA: 125] [Impact Index Per Article: 17.9] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/13/2017] [Accepted: 09/18/2017] [Indexed: 12/26/2022] Open
Abstract
The CRISPR-associated endonuclease Cas9 binds to a guide RNA and cleaves double-stranded DNA with a sequence complementary to the RNA guide. The Cas9-RNA system has been harnessed for numerous applications, such as genome editing. Here we use high-speed atomic force microscopy (HS-AFM) to visualize the real-space and real-time dynamics of CRISPR-Cas9 in action. HS-AFM movies indicate that, whereas apo-Cas9 adopts unexpected flexible conformations, Cas9-RNA forms a stable bilobed structure and interrogates target sites on the DNA by three-dimensional diffusion. These movies also provide real-time visualization of the Cas9-mediated DNA cleavage process. Notably, the Cas9 HNH nuclease domain fluctuates upon DNA binding, and subsequently adopts an active conformation, where the HNH active site is docked at the cleavage site in the target DNA. Collectively, our HS-AFM data extend our understanding of the action mechanism of CRISPR-Cas9.
Collapse
Affiliation(s)
- Mikihiro Shibata
- High-speed AFM for Biological Application Unit, Institute for Frontier Science Initiative, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan. .,Bio-AFM Frontier Research Center, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan.
| | - Hiroshi Nishimasu
- Department of Biological Sciences, Graduate School of Science, The University of Tokyo, 2-11-16 Yayoi, Bunkyo-ku, Tokyo, 113-0032, Japan. .,JST, PRESTO, 4-1-8 Honcho, Kawaguchi, Saitama, 332-0012, Japan.
| | - Noriyuki Kodera
- Bio-AFM Frontier Research Center, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan.,JST, PRESTO, 4-1-8 Honcho, Kawaguchi, Saitama, 332-0012, Japan
| | - Seiichi Hirano
- Department of Biological Sciences, Graduate School of Science, The University of Tokyo, 2-11-16 Yayoi, Bunkyo-ku, Tokyo, 113-0032, Japan
| | - Toshio Ando
- Bio-AFM Frontier Research Center, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan.,CREST/JST, 4-1-8 Honcho, Kawaguchi, Saitama, 332-0012, Japan
| | - Takayuki Uchihashi
- Bio-AFM Frontier Research Center, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan.,CREST/JST, 4-1-8 Honcho, Kawaguchi, Saitama, 332-0012, Japan.,Department of Physics, Kanazawa University, Kakuma, Kanazawa, 920-1192, Japan.,Department of Physics, Nagoya University, Furo-cho, Chikusa-ku, Nagoya, 464-8602, Japan
| | - Osamu Nureki
- Department of Biological Sciences, Graduate School of Science, The University of Tokyo, 2-11-16 Yayoi, Bunkyo-ku, Tokyo, 113-0032, Japan.
| |
Collapse
|
163
|
Terahara N, Kodera N, Uchihashi T, Ando T, Namba K, Minamino T. Na +-induced structural transition of MotPS for stator assembly of the Bacillus flagellar motor. SCIENCE ADVANCES 2017; 3:eaao4119. [PMID: 29109979 PMCID: PMC5665596 DOI: 10.1126/sciadv.aao4119] [Citation(s) in RCA: 34] [Impact Index Per Article: 4.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 07/17/2017] [Accepted: 10/06/2017] [Indexed: 05/03/2023]
Abstract
The bacterial flagellar motor consists of a rotor and a dozen stator units and regulates the number of active stator units around the rotor in response to changes in the environment. The MotPS complex is a Na+-type stator unit in the Bacillus subtilis flagellar motor and binds to the peptidoglycan layer through the peptidoglycan-binding (PGB) domain of MotS to act as the stator. The MotPS complex is activated in response to an increase in the Na+ concentration in the environment, but the mechanism of this activation has remained unknown. We report that activation occurs by a Na+-induced folding and dimer formation of the PGB domain of MotS, as revealed in real-time imaging by high-speed atomic force microscopy. The MotPS complex showed two distinct ellipsoid domains connected by a flexible linker. A smaller domain, corresponding to the PGB domain, became structured and unstructured in the presence and absence of 150 mM NaCl, respectively. When the amino-terminal portion of the PGB domain adopted a partially stretched conformation in the presence of NaCl, the center-to-center distance between these two domains increased by up to 5 nm, allowing the PGB domain to reach and bind to the peptidoglycan layer. We propose that assembly of the MotPS complex into a motor proceeds by means of Na+-induced structural transitions of its PGB domain.
Collapse
Affiliation(s)
- Naoya Terahara
- Graduate School of Frontier Biosciences, Osaka University, 1-3 Yamadaoka, Suita, Osaka 565-0871, Japan
| | - Noriyuki Kodera
- Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa 920-1192, Japan
| | - Takayuki Uchihashi
- Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa 920-1192, Japan
- Department of Physics, Kanazawa University, Kanazawa 920-1192, Japan
- Department of Physics, Nagoya University, Chikusa-ku, Nagoya 464-8602, Japan
| | - Toshio Ando
- Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa 920-1192, Japan
- Core Research for Evolutional Science and Technology, Japan Science and Technology Agency, Goban-cho, Chiyoda-ku, Tokyo 102-0076, Japan
| | - Keiichi Namba
- Graduate School of Frontier Biosciences, Osaka University, 1-3 Yamadaoka, Suita, Osaka 565-0871, Japan
- Quantitative Biology Center, RIKEN, 1-3 Yamadaoka, Suita, Osaka 565-0871, Japan
- Corresponding author. (T.M.); (K.N.)
| | - Tohru Minamino
- Graduate School of Frontier Biosciences, Osaka University, 1-3 Yamadaoka, Suita, Osaka 565-0871, Japan
- Corresponding author. (T.M.); (K.N.)
| |
Collapse
|
164
|
Wang D, Russell TP. Advances in Atomic Force Microscopy for Probing Polymer Structure and Properties. Macromolecules 2017. [DOI: 10.1021/acs.macromol.7b01459] [Citation(s) in RCA: 95] [Impact Index Per Article: 13.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/04/2023]
Affiliation(s)
| | - Thomas P. Russell
- Polymer
Science and Engineering Department, University of Massachusetts Amherst, Amherst, Massachusetts 01003, United States
- Materials
Sciences Division, Lawrence Berkeley National Laboratory, 1 Cyclotron Road, Berkeley, California 94720, United States
| |
Collapse
|
165
|
Zhang S, Geryak R, Geldmeier J, Kim S, Tsukruk VV. Synthesis, Assembly, and Applications of Hybrid Nanostructures for Biosensing. Chem Rev 2017; 117:12942-13038. [DOI: 10.1021/acs.chemrev.7b00088] [Citation(s) in RCA: 206] [Impact Index Per Article: 29.4] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/18/2022]
Affiliation(s)
- Shuaidi Zhang
- School of Materials Science
and Engineering, Georgia Institute of Technology, Atlanta, Georgia 30332-0245, United States
| | - Ren Geryak
- School of Materials Science
and Engineering, Georgia Institute of Technology, Atlanta, Georgia 30332-0245, United States
| | - Jeffrey Geldmeier
- School of Materials Science
and Engineering, Georgia Institute of Technology, Atlanta, Georgia 30332-0245, United States
| | - Sunghan Kim
- School of Materials Science
and Engineering, Georgia Institute of Technology, Atlanta, Georgia 30332-0245, United States
| | - Vladimir V. Tsukruk
- School of Materials Science
and Engineering, Georgia Institute of Technology, Atlanta, Georgia 30332-0245, United States
| |
Collapse
|
166
|
In Situ Atomic Force Microscopy Studies on Nucleation and Self-Assembly of Biogenic and Bio-Inspired Materials. MINERALS 2017. [DOI: 10.3390/min7090158] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 12/12/2022]
|
167
|
Shibata M, Watanabe H, Uchihashi T, Ando T, Yasuda R. High-speed atomic force microscopy imaging of live mammalian cells. Biophys Physicobiol 2017; 14:127-135. [PMID: 28900590 PMCID: PMC5590786 DOI: 10.2142/biophysico.14.0_127] [Citation(s) in RCA: 19] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/29/2017] [Accepted: 07/26/2017] [Indexed: 01/17/2023] Open
Abstract
Direct imaging of morphological dynamics of live mammalian cells with nanometer resolution under physiological conditions is highly expected, but yet challenging. High-speed atomic force microscopy (HS-AFM) is a unique technique for capturing biomolecules at work under near physiological conditions. However, application of HS-AFM for imaging of live mammalian cells was hard to be accomplished because of collision between a huge mammalian cell and a cantilever during AFM scanning. Here, we review our recent improvements of HS-AFM for imaging of activities of live mammalian cells without significant damage to the cell. The improvement of an extremely long (~3 μm) AFM tip attached to a cantilever enables us to reduce severe damage to soft mammalian cells. In addition, a combination of HS-AFM with simple fluorescence microscopy allows us to quickly locate the cell in the AFM scanning area. After these improvements, we demonstrate that developed HS-AFM for live mammalian cells is possible to image morphogenesis of filopodia, membrane ruffles, pits open-close formations, and endocytosis in COS-7, HeLa cells as well as hippocampal neurons.
Collapse
Affiliation(s)
- Mikihiro Shibata
- High-speed AFM for Biological Application Unit, Institute for Frontier Science Initiative, Kanazawa University, Kanazawa, Ishikawa 920-1192, Japan.,Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa, Ishikawa 920-1192, Japan
| | - Hiroki Watanabe
- Research Institute of Biomolecule Metrology Co., Ltd., Tsukuba, Ibaraki 305-0853, Japan
| | - Takayuki Uchihashi
- Department of Physics and Structural Biology Research Center, Graduate School of Science, Nagoya University, Nagoya, Aichi 464-8602, Japan
| | - Toshio Ando
- Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa, Ishikawa 920-1192, Japan
| | - Ryohei Yasuda
- Max Planck Florida Institute for Neuroscience, Jupiter, Florida 33458, USA
| |
Collapse
|
168
|
Iino R, Iida T, Nakamura A, Saita EI, You H, Sako Y. Single-molecule imaging and manipulation of biomolecular machines and systems. Biochim Biophys Acta Gen Subj 2017; 1862:241-252. [PMID: 28789884 DOI: 10.1016/j.bbagen.2017.08.008] [Citation(s) in RCA: 9] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/16/2017] [Revised: 07/23/2017] [Accepted: 08/03/2017] [Indexed: 02/08/2023]
Abstract
BACKGROUND Biological molecular machines support various activities and behaviors of cells, such as energy production, signal transduction, growth, differentiation, and migration. SCOPE OF REVIEW We provide an overview of single-molecule imaging methods involving both small and large probes used to monitor the dynamic motions of molecular machines in vitro (purified proteins) and in living cells, and single-molecule manipulation methods used to measure the forces, mechanical properties and responses of biomolecules. We also introduce several examples of single-molecule analysis, focusing primarily on motor proteins and signal transduction systems. MAJOR CONCLUSIONS Single-molecule analysis is a powerful approach to unveil the operational mechanisms both of individual molecular machines and of systems consisting of many molecular machines. GENERAL SIGNIFICANCE Quantitative, high-resolution single-molecule analyses of biomolecular systems at the various hierarchies of life will help to answer our fundamental question: "What is life?" This article is part of a Special Issue entitled "Biophysical Exploration of Dynamical Ordering of Biomolecular Systems" edited by Dr. Koichi Kato.
Collapse
Affiliation(s)
- Ryota Iino
- Okazaki Institute for Integrative Bioscience, Institute for Molecular Science, National Institutes of Natural Sciences, Japan; Department of Functional Molecular Science, School of Physical Sciences, The Graduate University for Advanced Studies (SOKENDAI), Japan.
| | - Tatsuya Iida
- Okazaki Institute for Integrative Bioscience, Institute for Molecular Science, National Institutes of Natural Sciences, Japan; Department of Functional Molecular Science, School of Physical Sciences, The Graduate University for Advanced Studies (SOKENDAI), Japan
| | - Akihiko Nakamura
- Okazaki Institute for Integrative Bioscience, Institute for Molecular Science, National Institutes of Natural Sciences, Japan; Department of Functional Molecular Science, School of Physical Sciences, The Graduate University for Advanced Studies (SOKENDAI), Japan
| | - Ei-Ichiro Saita
- Information Processing Biology Unit, Okinawa Institute of Science and Technology Graduate University, Japan
| | - Huijuan You
- School of Pharmacy, Tongji Medical College, Huazhong University of Science and Technology, China.
| | | |
Collapse
|
169
|
Harada H, Onoda A, Uchihashi T, Watanabe H, Sunagawa N, Samejima M, Igarashi K, Hayashi T. Interdomain flip-flop motion visualized in flavocytochrome cellobiose dehydrogenase using high-speed atomic force microscopy during catalysis. Chem Sci 2017; 8:6561-6565. [PMID: 28989682 PMCID: PMC5627353 DOI: 10.1039/c7sc01672g] [Citation(s) in RCA: 21] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/14/2017] [Accepted: 07/15/2017] [Indexed: 12/02/2022] Open
Abstract
To visualize the dynamic domain motion of class-I CDH from Phanerochaete chrysosporium (PcCDH) during catalysis using high-speed atomic force microscopy, the apo-form of PcCDH was anchored to a heme-immobilized flat gold surface that can fix the orientation of the CYT domain.
Cellobiose dehydrogenase (CDH) is a dual domain flavocytochrome, which consists of a dehydrogenase (DH) domain containing a flavin adenine dinucleotide and a cytochrome (CYT) domain containing b-type heme. To directly visualize the dynamic domain motion of class-I CDH from Phanerochaete chrysosporium (PcCDH) during catalysis using high-speed atomic force microscopy, the apo-form of PcCDH was anchored to a heme-immobilized flat gold surface that can specifically fix the orientation of the CYT domain. The two domains of CDH are found to be immobile in the absence of cellobiose, whereas the addition of cellobiose triggers an interdomain flip-flop motion involving domain–domain association and dissociation. Our results indicate that dynamic motion of a dual domain enzyme during catalysis induces efficient electron transfer to an external electron acceptor.
Collapse
Affiliation(s)
- Hirofumi Harada
- Department of Applied Chemistry , Graduate School of Engineering , Osaka University , 2-1 Yamadaoka , Suita , Osaka 565-0871 , Japan . ;
| | - Akira Onoda
- Department of Applied Chemistry , Graduate School of Engineering , Osaka University , 2-1 Yamadaoka , Suita , Osaka 565-0871 , Japan . ;
| | - Takayuki Uchihashi
- Department of Physics , Nagoya University , Furo-cho, Chikusa-ku , Nagoya , 464-8602 , Japan .
| | - Hiroki Watanabe
- Faculty of Natural Science and Technology , Kanazawa University , Kakuma , Kanazawa , 920-1192 , Japan
| | - Naoki Sunagawa
- Department of Biomaterials Sciences , Graduate School of Agricultural and Life Sciences , The University of Tokyo , Bunkyo-ku , 113-8657 , Japan .
| | - Masahiro Samejima
- Department of Biomaterials Sciences , Graduate School of Agricultural and Life Sciences , The University of Tokyo , Bunkyo-ku , 113-8657 , Japan .
| | - Kiyohiko Igarashi
- Department of Biomaterials Sciences , Graduate School of Agricultural and Life Sciences , The University of Tokyo , Bunkyo-ku , 113-8657 , Japan . .,VTT Technical Research Centre of Finland , P.O. Box 1000, Tietotie 2 , Espoo FI-02044 VTT , Finland
| | - Takashi Hayashi
- Department of Applied Chemistry , Graduate School of Engineering , Osaka University , 2-1 Yamadaoka , Suita , Osaka 565-0871 , Japan . ;
| |
Collapse
|
170
|
Ando T. Directly watching biomolecules in action by high-speed atomic force microscopy. Biophys Rev 2017; 9:421-429. [PMID: 28762198 DOI: 10.1007/s12551-017-0281-7] [Citation(s) in RCA: 32] [Impact Index Per Article: 4.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/03/2017] [Accepted: 07/14/2017] [Indexed: 12/17/2022] Open
Abstract
Proteins are dynamic in nature and work at the single molecule level. Therefore, directly watching protein molecules in dynamic action at high spatiotemporal resolution must be the most straightforward approach to understanding how they function. To make this observation possible, high-speed atomic force microscopy (HS-AFM) has been developed. Its current performance allows us to film biological molecules at 10-16 frames/s, without disturbing their function. In fact, dynamic structures and processes of various proteins have been successfully visualized, including bacteriorhodopsin responding to light, myosin V walking on actin filaments, and even intrinsically disordered proteins undergoing order/disorder transitions. The molecular movies have provided insights that could not have been reached in other ways. Moreover, the cantilever tip can be used to manipulate molecules during successive imaging. This capability allows us to observe changes in molecules resulting from dissection or perturbation. This mode of imaging has been successfully applied to myosin V, peroxiredoxin and doublet microtubules, leading to new discoveries. Since HS-AFM can be combined with other techniques, such as super-resolution optical microscopy and optical tweezers, the usefulness of HS-AFM will be further expanded in the near future.
Collapse
Affiliation(s)
- Toshio Ando
- Bio-AFM Frontier Research Center, Institute of Science and Engineering, Kanazawa University, Kakuma-machi, Kanazawa, 920-1192, Japan. .,CREST, Japan Science and Technology Agency, Tokyo, 102-0075, Japan.
| |
Collapse
|
171
|
Yamada Y, Konno H, Shimabukuro K. Demonstration of correlative atomic force and transmission electron microscopy using actin cytoskeleton. Biophys Physicobiol 2017; 14:111-117. [PMID: 28828286 PMCID: PMC5551270 DOI: 10.2142/biophysico.14.0_111] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/14/2016] [Accepted: 06/29/2017] [Indexed: 12/01/2022] Open
Abstract
In this study, we present a new technique called correlative atomic force and transmission electron microscopy (correlative AFM/TEM) in which a targeted region of a sample can be observed under AFM and TEM. The ultimate goal of developing this new technique is to provide a technical platform to expand the fields of AFM application to complex biological systems such as cell extracts. Recent advances in the time resolution of AFM have enabled detailed observation of the dynamic nature of biomolecules. However, specifying molecular species, by AFM alone, remains a challenge. Here, we demonstrate correlative AFM/TEM, using actin filaments as a test sample, and further show that immuno-electron microscopy (immuno-EM), to specify molecules, can be integrated into this technique. Therefore, it is now possible to specify molecules, captured under AFM, by subsequent observation using immuno-EM. In conclusion, correlative AFM/TEM can be a versatile method to investigate complex biological systems at the molecular level.
Collapse
Affiliation(s)
- Yutaro Yamada
- Department of Chemical and Biological Engineering, National College of Technology, Ube College, Ube, Yamaguchi 755-8555, Japan
| | - Hiroki Konno
- Bio-AFM Frontier Research Center, Kanazawa University, Kanazawa, Ishikawa 920-1192, Japan
| | - Katsuya Shimabukuro
- Department of Chemical and Biological Engineering, National College of Technology, Ube College, Ube, Yamaguchi 755-8555, Japan
| |
Collapse
|
172
|
Tirion MM. A comparison of the innate flexibilities of six chains in F1-ATPase with identical secondary and tertiary folds; 3 active enzymes and 3 structural proteins. Struct Dyn 2017; 4:044001. [PMID: 27872875 PMCID: PMC5097049 DOI: 10.1063/1.4967226] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/11/2016] [Accepted: 10/21/2016] [Indexed: 11/23/2022] Open
Abstract
The α and β subunits comprising the hexameric assembly of F1-ATPase share a high degree of structural identity, though low primary identity. Each subunit binds nucleotide in similar pockets, yet only β subunits are catalytically active. Why? We re-examine their internal symmetry axes and observe interesting differences. Dividing each chain into an N-terminal head region, a C-terminal foot region, and a central torso, we observe (1) that while the foot and head regions in all chains obtain high and similar mobility, the torsos obtain different mobility profiles, with the β subunits exhibiting a higher motility compared to the α subunits, a trend supported by the crystallographic B-factors. The β subunits have greater torso mobility by having fewer distributed, nonlocal packing interactions providing a spacious and soft connectivity and offsetting the resultant softness with local stiffness elements, including an additional β sheet. (2) A loop near the nucleotide binding-domain of the β subunits, absent in the α subunits, swings to create a large variation in the occlusion of the nucleotide binding region. (3) A combination of the softest three eigenmodes significantly reduces the root mean square difference between the open and closed conformations of the β subunits. (4) Comparisons of computed and observed crystallographic B-factors suggest a suppression of a particular symmetry axis in an α subunit. (5) Unexpectedly, the soft intra-monomer oscillations pertain to distortions that do not create inter-monomer steric clashes in the assembly, suggesting that structural optimization of the assembly evolved at all levels of complexity.
Collapse
Affiliation(s)
- Monique M. Tirion
- Physics Department, Clarkson University, Potsdam, New York 13699-5820, USA
| |
Collapse
|
173
|
Zhang Y, Yoshida A, Sakai N, Uekusa Y, Kumeta M, Yoshimura SH. In vivo dynamics of the cortical actin network revealed by fast-scanning atomic force microscopy. Microscopy (Oxf) 2017; 66:272-282. [DOI: 10.1093/jmicro/dfx015] [Citation(s) in RCA: 18] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/07/2017] [Accepted: 04/29/2017] [Indexed: 11/13/2022] Open
Affiliation(s)
- Yanshu Zhang
- Graduate School of Biostudies, Kyoto University, Yoshida-konoe, Sakyo-ku, Kyoto 606-8501, Japan
| | - Aiko Yoshida
- Graduate School of Biostudies, Kyoto University, Yoshida-konoe, Sakyo-ku, Kyoto 606-8501, Japan
| | | | | | - Masahiro Kumeta
- Graduate School of Biostudies, Kyoto University, Yoshida-konoe, Sakyo-ku, Kyoto 606-8501, Japan
| | - Shige H. Yoshimura
- Graduate School of Biostudies, Kyoto University, Yoshida-konoe, Sakyo-ku, Kyoto 606-8501, Japan
| |
Collapse
|
174
|
Maegawa KI, Watanabe S, Noi K, Okumura M, Amagai Y, Inoue M, Ushioda R, Nagata K, Ogura T, Inaba K. The Highly Dynamic Nature of ERdj5 Is Key to Efficient Elimination of Aberrant Protein Oligomers through ER-Associated Degradation. Structure 2017; 25:846-857.e4. [PMID: 28479060 DOI: 10.1016/j.str.2017.04.001] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 11/14/2016] [Revised: 03/08/2017] [Accepted: 04/10/2017] [Indexed: 12/12/2022]
Abstract
ERdj5, composed of an N-terminal J domain followed by six thioredoxin-like domains, is the largest protein disulfide isomerase family member and functions as an ER-localized disulfide reductase that enhances ER-associated degradation (ERAD). Our previous studies indicated that ERdj5 comprises two regions, the N- and C-terminal clusters, separated by a linker loop and with distinct functional roles in ERAD. We here present a new crystal structure of ERdj5 with a largely different cluster arrangement relative to that in the original crystal structure. Single-molecule observation by high-speed atomic force microscopy visualized rapid cluster movement around the flexible linker loop, indicating the highly dynamic nature of ERdj5 in solution. ERdj5 mutants with a fixed-cluster orientation compromised the ERAD enhancement activity, likely because of less-efficient reduction of aberrantly formed disulfide bonds and prevented substrate transfer in the ERdj5-mediated ERAD pathway. We propose a significant role of ERdj5 conformational dynamics in ERAD of disulfide-linked oligomers.
Collapse
Affiliation(s)
- Ken-Ichi Maegawa
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan; CREST, JST, Japan
| | - Satoshi Watanabe
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan; CREST, JST, Japan
| | - Kentaro Noi
- Institute of Molecular Embryology and Genetics, Kumamoto University, Kumamoto 860-0811, Japan; CREST, JST, Japan
| | - Masaki Okumura
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan
| | - Yuta Amagai
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan
| | - Michio Inoue
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan; CREST, JST, Japan
| | - Ryo Ushioda
- Department of Molecular Biosciences, Kyoto Sangyo University, Kyoto 603-8455, Japan; CREST, JST, Japan
| | - Kazuhiro Nagata
- Department of Molecular Biosciences, Kyoto Sangyo University, Kyoto 603-8455, Japan; CREST, JST, Japan
| | - Teru Ogura
- Institute of Molecular Embryology and Genetics, Kumamoto University, Kumamoto 860-0811, Japan; CREST, JST, Japan
| | - Kenji Inaba
- Institute of Multidisciplinary Research for Advanced Materials, Tohoku University, Katahira 2-1-1, Aoba-ku, Sendai 980-8577, Japan; CREST, JST, Japan.
| |
Collapse
|
175
|
Dufrêne YF, Ando T, Garcia R, Alsteens D, Martinez-Martin D, Engel A, Gerber C, Müller DJ. Imaging modes of atomic force microscopy for application in molecular and cell biology. NATURE NANOTECHNOLOGY 2017; 12:295-307. [PMID: 28383040 DOI: 10.1038/nnano.2017.45] [Citation(s) in RCA: 482] [Impact Index Per Article: 68.9] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/10/2016] [Accepted: 02/23/2017] [Indexed: 05/22/2023]
Abstract
Atomic force microscopy (AFM) is a powerful, multifunctional imaging platform that allows biological samples, from single molecules to living cells, to be visualized and manipulated. Soon after the instrument was invented, it was recognized that in order to maximize the opportunities of AFM imaging in biology, various technological developments would be required to address certain limitations of the method. This has led to the creation of a range of new imaging modes, which continue to push the capabilities of the technique today. Here, we review the basic principles, advantages and limitations of the most common AFM bioimaging modes, including the popular contact and dynamic modes, as well as recently developed modes such as multiparametric, molecular recognition, multifrequency and high-speed imaging. For each of these modes, we discuss recent experiments that highlight their unique capabilities.
Collapse
Affiliation(s)
- Yves F Dufrêne
- Institute of Life Sciences and Walloon Excellence in Life Sciences and Biotechnology (WELBIO), Université catholique de Louvain, Croix du Sud 4-5, bte L7.07.06., B-1348 Louvain-la-Neuve, Belgium
| | - Toshio Ando
- Department of Physics, Kanazawa University, Kanazawa 920-1192, Japan
| | - Ricardo Garcia
- Instituto de Ciencia de Materiales de Madrid, CSIC, Sor Juana Inés de la Cruz 3, 28049 Madrid, Spain
| | - David Alsteens
- Institute of Life Sciences and Walloon Excellence in Life Sciences and Biotechnology (WELBIO), Université catholique de Louvain, Croix du Sud 4-5, bte L7.07.06., B-1348 Louvain-la-Neuve, Belgium
| | - David Martinez-Martin
- Department of Biosystems Science and Engineering, Eidgenössische Technische Hochschule (ETH) Zürich, Mattenstrasse 28, 4056 Basel, Switzerland
| | - Andreas Engel
- Department of BioNanoscience, Delft University of Technology, Van der Maasweg 9, 2629 HZ Delft, The Netherlands
| | - Christoph Gerber
- Swiss Nanoscience Institute, University of Basel, Klingelbergstrasse 80, 4057 Basel, Switzerland
| | - Daniel J Müller
- Department of Biosystems Science and Engineering, Eidgenössische Technische Hochschule (ETH) Zürich, Mattenstrasse 28, 4056 Basel, Switzerland
| |
Collapse
|
176
|
Noji H, Ueno H, McMillan DGG. Catalytic robustness and torque generation of the F 1-ATPase. Biophys Rev 2017; 9:103-118. [PMID: 28424741 PMCID: PMC5380711 DOI: 10.1007/s12551-017-0262-x] [Citation(s) in RCA: 40] [Impact Index Per Article: 5.7] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/30/2017] [Accepted: 03/13/2017] [Indexed: 12/28/2022] Open
Abstract
The F1-ATPase is the catalytic portion of the FoF1 ATP synthase and acts as a rotary molecular motor when it hydrolyzes ATP. Two decades have passed since the single-molecule rotation assay of F1-ATPase was established. Although several fundamental issues remain elusive, basic properties of F-type ATPases as motor proteins have been well characterized, and a large part of the reaction scheme has been revealed by the combination of extensive structural, biochemical, biophysical, and theoretical studies. This review is intended to provide a concise summary of the fundamental features of F1-ATPases, by use of the well-described model F1 from the thermophilic Bacillus PS3 (TF1). In the last part of this review, we focus on the robustness of the rotary catalysis of F1-ATPase to provide a perspective on the re-designing of novel molecular machines.
Collapse
Affiliation(s)
- Hiroyuki Noji
- Department of Applied Chemistry, Graduate School of Engineering, The University of Tokyo, Tokyo, 113-8656 Japan
| | - Hiroshi Ueno
- Department of Applied Chemistry, Graduate School of Engineering, The University of Tokyo, Tokyo, 113-8656 Japan
| | - Duncan G. G. McMillan
- Department of Applied Chemistry, Graduate School of Engineering, The University of Tokyo, Tokyo, 113-8656 Japan
| |
Collapse
|
177
|
Karner A, Nimmervoll B, Plochberger B, Klotzsch E, Horner A, Knyazev DG, Kuttner R, Winkler K, Winter L, Siligan C, Ollinger N, Pohl P, Preiner J. Tuning membrane protein mobility by confinement into nanodomains. NATURE NANOTECHNOLOGY 2017; 12:260-266. [PMID: 27842062 PMCID: PMC5734611 DOI: 10.1038/nnano.2016.236] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.4] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 08/07/2015] [Accepted: 09/30/2016] [Indexed: 05/04/2023]
Abstract
High-speed atomic force microscopy (HS-AFM) can be used to visualize function-related conformational changes of single soluble proteins. Similar studies of single membrane proteins are, however, hampered by a lack of suitable flat, non-interacting membrane supports and by high protein mobility. Here we show that streptavidin crystals grown on mica-supported lipid bilayers can be used as porous supports for membranes containing biotinylated lipids. Using SecYEG (protein translocation channel) and GlpF (aquaglyceroporin), we demonstrate that the platform can be used to tune the lateral mobility of transmembrane proteins to any value within the dynamic range accessible to HS-AFM imaging through glutaraldehyde-cross-linking of the streptavidin. This allows HS-AFM to study the conformation or docking of spatially confined proteins, which we illustrate by imaging GlpF at sub-molecular resolution and by observing the motor protein SecA binding to SecYEG.
Collapse
Affiliation(s)
- Andreas Karner
- Center for Advanced Bioanalysis GmbH, Gruberstr. 40-42, 4020 Linz, Austria
| | | | - Birgit Plochberger
- Upper Austria University of Applied Sciences, Campus Linz, Garnisonstrasse 21, 4020 Linz, Austria
| | - Enrico Klotzsch
- EMBL Australia Node in Single Molecule Science and ARC Centre of Excellence in Advanced Molecular Imaging, University of New South Wales, Sydney, Australia
| | - Andreas Horner
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Denis G. Knyazev
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Roland Kuttner
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Klemens Winkler
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Lukas Winter
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Christine Siligan
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Nicole Ollinger
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Peter Pohl
- Institute of Biophysics, Johannes Kepler University Linz, Gruberstr. 40, 4020 Linz, Austria
| | - Johannes Preiner
- Center for Advanced Bioanalysis GmbH, Gruberstr. 40-42, 4020 Linz, Austria
| |
Collapse
|
178
|
Sysoeva TA. Assessing heterogeneity in oligomeric AAA+ machines. Cell Mol Life Sci 2017; 74:1001-1018. [PMID: 27669691 PMCID: PMC11107579 DOI: 10.1007/s00018-016-2374-z] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/14/2016] [Revised: 09/13/2016] [Accepted: 09/19/2016] [Indexed: 10/20/2022]
Abstract
ATPases Associated with various cellular Activities (AAA+ ATPases) are molecular motors that use the energy of ATP binding and hydrolysis to remodel their target macromolecules. The majority of these ATPases form ring-shaped hexamers in which the active sites are located at the interfaces between neighboring subunits. Structural changes initiate in an active site and propagate to distant motor parts that interface and reshape the target macromolecules, thereby performing mechanical work. During the functioning cycle, the AAA+ motor transits through multiple distinct states. Ring architecture and placement of the catalytic sites at the intersubunit interfaces allow for a unique level of coordination among subunits of the motor. This in turn results in conformational differences among subunits and overall asymmetry of the motor ring as it functions. To date, a large amount of structural information has been gathered for different AAA+ motors, but even for the most characterized of them only a few structural states are known and the full mechanistic cycle cannot be yet reconstructed. Therefore, the first part of this work will provide a broad overview of what arrangements of AAA+ subunits have been structurally observed focusing on diversity of ATPase oligomeric ensembles and heterogeneity within the ensembles. The second part of this review will concentrate on methods that assess structural and functional heterogeneity among subunits of AAA+ motors, thus bringing us closer to understanding the mechanism of these fascinating molecular motors.
Collapse
Affiliation(s)
- Tatyana A Sysoeva
- Department of Biomedical Engineering, Duke University, Durham, NC, 27708, USA.
| |
Collapse
|
179
|
Lu X, Ovchinnikov V, Demapan D, Roston D, Cui Q. Regulation and Plasticity of Catalysis in Enzymes: Insights from Analysis of Mechanochemical Coupling in Myosin. Biochemistry 2017; 56:1482-1497. [PMID: 28225609 DOI: 10.1021/acs.biochem.7b00016] [Citation(s) in RCA: 27] [Impact Index Per Article: 3.9] [Reference Citation Analysis] [Abstract] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/08/2023]
Abstract
The mechanism of ATP hydrolysis in the myosin motor domain is analyzed using a combination of DFTB3/CHARMM simulations and enhanced sampling techniques. The motor domain is modeled in the pre-powerstroke state, in the post-rigor state, and as a hybrid based on the post-rigor state with a closed nucleotide-binding pocket. The ATP hydrolysis activity is found to depend on the positioning of nearby water molecules, and a network of polar residues facilitates proton transfer and charge redistribution during hydrolysis. Comparison of the observed hydrolysis pathways and the corresponding free energy profiles leads to detailed models for the mechanism of ATP hydrolysis in the pre-powerstroke state and proposes factors that regulate the hydrolysis activity in different conformational states. In the pre-powerstroke state, the scissile Pγ-O3β bond breaks early in the reaction. Proton transfer from the lytic water to the γ-phosphate through active site residues is an important part of the kinetic bottleneck; several hydrolysis pathways that feature distinct proton transfer routes are found to have similar free energy barriers, suggesting a significant degree of plasticity in the hydrolysis mechanism. Comparison of hydrolysis in the pre-powerstroke state and the closed post-rigor model suggests that optimization of residues beyond the active site for electrostatic stabilization and preorganization is likely important to enzyme design.
Collapse
Affiliation(s)
- Xiya Lu
- Department of Chemistry and Theoretical Chemistry Institute, University of Wisconsin-Madison , 1101 University Avenue, Madison, Wisconsin 53706, United States
| | - Victor Ovchinnikov
- Department of Chemistry and Chemical Biology, Harvard University , 12 Oxford Street, Boston, Massachusetts 02138, United States
| | - Darren Demapan
- Department of Chemistry and Theoretical Chemistry Institute, University of Wisconsin-Madison , 1101 University Avenue, Madison, Wisconsin 53706, United States
| | - Daniel Roston
- Department of Chemistry and Theoretical Chemistry Institute, University of Wisconsin-Madison , 1101 University Avenue, Madison, Wisconsin 53706, United States
| | - Qiang Cui
- Department of Chemistry and Theoretical Chemistry Institute, University of Wisconsin-Madison , 1101 University Avenue, Madison, Wisconsin 53706, United States
| |
Collapse
|
180
|
Imaging and Force Recognition of Single Molecular Behaviors Using Atomic Force Microscopy. SENSORS 2017; 17:s17010200. [PMID: 28117741 PMCID: PMC5298773 DOI: 10.3390/s17010200] [Citation(s) in RCA: 22] [Impact Index Per Article: 3.1] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 12/28/2016] [Revised: 01/12/2017] [Accepted: 01/16/2017] [Indexed: 12/23/2022]
Abstract
The advent of atomic force microscopy (AFM) has provided a powerful tool for investigating the behaviors of single native biological molecules under physiological conditions. AFM can not only image the conformational changes of single biological molecules at work with sub-nanometer resolution, but also sense the specific interactions of individual molecular pair with piconewton force sensitivity. In the past decade, the performance of AFM has been greatly improved, which makes it widely used in biology to address diverse biomedical issues. Characterizing the behaviors of single molecules by AFM provides considerable novel insights into the underlying mechanisms guiding life activities, contributing much to cell and molecular biology. In this article, we review the recent developments of AFM studies in single-molecule assay. The related techniques involved in AFM single-molecule assay were firstly presented, and then the progress in several aspects (including molecular imaging, molecular mechanics, molecular recognition, and molecular activities on cell surface) was summarized. The challenges and future directions were also discussed.
Collapse
|
181
|
In situ structure of trypanosomal ATP synthase dimer reveals a unique arrangement of catalytic subunits. Proc Natl Acad Sci U S A 2017; 114:992-997. [PMID: 28096380 DOI: 10.1073/pnas.1612386114] [Citation(s) in RCA: 38] [Impact Index Per Article: 5.4] [Reference Citation Analysis] [Abstract] [Key Words] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/05/2023] Open
Abstract
We used electron cryotomography and subtomogram averaging to determine the in situ structures of mitochondrial ATP synthase dimers from two organisms belonging to the phylum euglenozoa: Trypanosoma brucei, a lethal human parasite, and Euglena gracilis, a photosynthetic protist. At a resolution of 32.5 Å and 27.5 Å, respectively, the two structures clearly exhibit a noncanonical F1 head, in which the catalytic (αβ)3 assembly forms a triangular pyramid rather than the pseudo-sixfold ring arrangement typical of all other ATP synthases investigated so far. Fitting of known X-ray structures reveals that this unusual geometry results from a phylum-specific cleavage of the α subunit, in which the C-terminal αC fragments are displaced by ∼20 Å and rotated by ∼30° from their expected positions. In this location, the αC fragment is unable to form the conserved catalytic interface that was thought to be essential for ATP synthesis, and cannot convert γ-subunit rotation into the conformational changes implicit in rotary catalysis. The new arrangement of catalytic subunits suggests that the mechanism of ATP generation by rotary ATPases is less strictly conserved than has been generally assumed. The ATP synthases of these organisms present a unique model system for discerning the individual contributions of the α and β subunits to the fundamental process of ATP synthesis.
Collapse
|
182
|
Singharoy A, Chipot C, Moradi M, Schulten K. Chemomechanical Coupling in Hexameric Protein-Protein Interfaces Harnesses Energy within V-Type ATPases. J Am Chem Soc 2017; 139:293-310. [PMID: 27936329 PMCID: PMC5518570 DOI: 10.1021/jacs.6b10744] [Citation(s) in RCA: 37] [Impact Index Per Article: 5.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/28/2022]
Abstract
ATP synthase is the most prominent bioenergetic macromolecular motor in all life forms, utilizing the proton gradient across the cell membrane to fuel the synthesis of ATP. Notwithstanding the wealth of available biochemical and structural information inferred from years of experiments, the precise molecular mechanism whereby vacuolar (V-type) ATP synthase fulfills its biological function remains largely fragmentary. Recently, crystallographers provided the first high-resolution view of ATP activity in Enterococcus hirae V1-ATPase. Employing a combination of transition-path sampling and high-performance free-energy methods, the sequence of conformational transitions involved in a functional cycle accompanying ATP hydrolysis has been investigated in unprecedented detail over an aggregate simulation time of 65 μs. Our simulated pathways reveal that the chemical energy produced by ATP hydrolysis is harnessed via the concerted motion of the protein-protein interfaces in the V1-ring, and is nearly entirely consumed in the rotation of the central stalk. Surprisingly, in an ATPase devoid of a central stalk, the interfaces of this ring are perfectly designed for inducing ATP hydrolysis. However, in a complete V1-ATPase, the mechanical property of the central stalk is a key determinant of the rate of ATP turnover. The simulations further unveil a sequence of events, whereby unbinding of the hydrolysis product (ADP + Pi) is followed by ATP uptake, which, in turn, leads to the torque generation step and rotation of the center stalk. Molecular trajectories also bring to light multiple intermediates, two of which have been isolated in independent crystallography experiments.
Collapse
Affiliation(s)
- Abhishek Singharoy
- Theoretical and Computational Biophysics Group, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign , 405 North Mathews Avenue, Urbana, Illinois 61801, United States
| | - Christophe Chipot
- Theoretical and Computational Biophysics Group, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign , 405 North Mathews Avenue, Urbana, Illinois 61801, United States
- Laboratoire International Associé Centre National de la Recherche Scientifique et University of Illinois at Urbana-Champaign, Unité Mixte de Recherche n°7565, Université de Lorraine , B.P. 70239, 54506 Vandœuvre-lès-Nancy Cedex, France
- Department of Physics, University of Illinois at Urbana-Champaign , 1110 West Green Street, Urbana, Illinois 61801, United States
| | - Mahmoud Moradi
- Department of Chemistry and Biochemistry, University of Arkansas , Fayetteville, Arkansas 72701, United States
| | - Klaus Schulten
- Theoretical and Computational Biophysics Group, Beckman Institute for Advanced Science and Technology, University of Illinois at Urbana-Champaign , 405 North Mathews Avenue, Urbana, Illinois 61801, United States
- Department of Physics, University of Illinois at Urbana-Champaign , 1110 West Green Street, Urbana, Illinois 61801, United States
| |
Collapse
|
183
|
Ruppert MG, Harcombe DM, Ragazzon MRP, Moheimani SOR, Fleming AJ. A review of demodulation techniques for amplitude-modulation atomic force microscopy. BEILSTEIN JOURNAL OF NANOTECHNOLOGY 2017; 8:1407-1426. [PMID: 28900596 PMCID: PMC5530615 DOI: 10.3762/bjnano.8.142] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/23/2016] [Accepted: 06/07/2017] [Indexed: 05/09/2023]
Abstract
In this review paper, traditional and novel demodulation methods applicable to amplitude-modulation atomic force microscopy are implemented on a widely used digital processing system. As a crucial bandwidth-limiting component in the z-axis feedback loop of an atomic force microscope, the purpose of the demodulator is to obtain estimates of amplitude and phase of the cantilever deflection signal in the presence of sensor noise or additional distinct frequency components. Specifically for modern multifrequency techniques, where higher harmonic and/or higher eigenmode contributions are present in the oscillation signal, the fidelity of the estimates obtained from some demodulation techniques is not guaranteed. To enable a rigorous comparison, the performance metrics tracking bandwidth, implementation complexity and sensitivity to other frequency components are experimentally evaluated for each method. Finally, the significance of an adequate demodulator bandwidth is highlighted during high-speed tapping-mode atomic force microscopy experiments in constant-height mode.
Collapse
Affiliation(s)
- Michael G Ruppert
- School of Electrical Engineering and Computing, The University of Newcastle, Callaghan, NSW, 2308, Australia
| | - David M Harcombe
- School of Electrical Engineering and Computing, The University of Newcastle, Callaghan, NSW, 2308, Australia
| | - Michael R P Ragazzon
- Department of Engineering Cybernetics, NTNU, Norwegian University of Science and Technology, Trondheim, Norway
| | - S O Reza Moheimani
- Department of Mechanical Engineering, The University of Texas at Dallas, Richardson, TX, USA
| | - Andrew J Fleming
- School of Electrical Engineering and Computing, The University of Newcastle, Callaghan, NSW, 2308, Australia
| |
Collapse
|
184
|
Guzman HV. Scaling law to determine peak forces in tapping-mode AFM experiments on finite elastic soft matter systems. BEILSTEIN JOURNAL OF NANOTECHNOLOGY 2017; 8:968-974. [PMID: 28546891 PMCID: PMC5433196 DOI: 10.3762/bjnano.8.98] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/24/2016] [Accepted: 03/26/2017] [Indexed: 05/07/2023]
Abstract
Analytical equations to estimate the peak force will facilitate the interpretation and the planning of amplitude-modulation force microscopy (tapping mode) experiments. A closed-form analytical equation to estimate the tip-sample peak forces while imaging soft materials in liquid environment and within an elastic deformation regime has been deduced. We have combined a multivariate regression method with input from the virial-dissipation equations and Tatara's bidimensional deformation contact mechanics model. The equation enables to estimate the peak force based on the tapping mode observables, probe characteristics and the material properties of the sample. The accuracy of the equation has been verified by comparing it to numerical simulations for the archetypical operating conditions to image soft matter with high spatial resolution in tapping-mode AFM.
Collapse
Affiliation(s)
- Horacio V Guzman
- Max Planck Institute for Polymer Research, Ackermannweg 10, 55128 Mainz, Germany
| |
Collapse
|
185
|
Direct-write nanoscale printing of nanogranular tunnelling strain sensors for sub-micrometre cantilevers. Nat Commun 2016; 7:12487. [PMID: 27666316 PMCID: PMC5052671 DOI: 10.1038/ncomms12487] [Citation(s) in RCA: 32] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/04/2015] [Accepted: 07/07/2016] [Indexed: 01/07/2023] Open
Abstract
The sensitivity and detection speed of cantilever-based mechanical sensors increases drastically through size reduction. The need for such increased performance for high-speed nanocharacterization and bio-sensing, drives their sub-micrometre miniaturization in a variety of research fields. However, existing detection methods of the cantilever motion do not scale down easily, prohibiting further increase in the sensitivity and detection speed. Here we report a nanomechanical sensor readout based on electron co-tunnelling through a nanogranular metal. The sensors can be deposited with lateral dimensions down to tens of nm, allowing the readout of nanoscale cantilevers without constraints on their size, geometry or material. By modifying the inter-granular tunnel-coupling strength, the sensors' conductivity can be tuned by up to four orders of magnitude, to optimize their performance. We show that the nanoscale printed sensors are functional on 500 nm wide cantilevers and that their sensitivity is suited even for demanding applications such as atomic force microscopy. Reducing the size of cantilever-based sensors increases the sensitivity and detection speed of techniques such as atomic force microscopy. Here, the authors demonstrate a nanomechanical readout method that can be easily scaled down in size by using electron co-tunnelling through a nanogranular metal.
Collapse
|
186
|
Rangl M, Miyagi A, Kowal J, Stahlberg H, Nimigean CM, Scheuring S. Real-time visualization of conformational changes within single MloK1 cyclic nucleotide-modulated channels. Nat Commun 2016; 7:12789. [PMID: 27647260 PMCID: PMC5034309 DOI: 10.1038/ncomms12789] [Citation(s) in RCA: 24] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/11/2016] [Accepted: 08/01/2016] [Indexed: 01/11/2023] Open
Abstract
Eukaryotic cyclic nucleotide-modulated (CNM) ion channels perform various physiological roles by opening in response to cyclic nucleotides binding to a specialized cyclic nucleotide-binding domain. Despite progress in structure-function analysis, the conformational rearrangements underlying the gating of these channels are still unknown. Here, we image ligand-induced conformational changes in single CNM channels from Mesorhizobium loti (MloK1) in real-time, using high-speed atomic force microscopy. In the presence of cAMP, most channels are in a stable conformation, but a few molecules dynamically switch back and forth (blink) between at least two conformations with different heights. Upon cAMP depletion, more channels start blinking, with blinking heights increasing over time, suggestive of slow, progressive loss of ligands from the tetramer. We propose that during gating, MloK1 transitions from a set of mobile conformations in the absence to a stable conformation in the presence of ligand and that these conformations are central for gating the pore.
Collapse
Affiliation(s)
- Martina Rangl
- INSERM U1006, Aix-Marseille Université, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, Marseille 13009, France
| | - Atsushi Miyagi
- INSERM U1006, Aix-Marseille Université, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, Marseille 13009, France
| | - Julia Kowal
- Center for Cellular Imaging and NanoAnalytics, Biozentrum, University of Basel, Mattenstrasse 26, Basel CH-4058, Switzerland
| | - Henning Stahlberg
- Center for Cellular Imaging and NanoAnalytics, Biozentrum, University of Basel, Mattenstrasse 26, Basel CH-4058, Switzerland
| | - Crina M Nimigean
- INSERM U1006, Aix-Marseille Université, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, Marseille 13009, France.,Departments of Anesthesiology, Physiology and Biophysics, and Biochemistry, Weill Cornell Medical College, 1300 York Avenue, New York, New York 10065, USA
| | - Simon Scheuring
- INSERM U1006, Aix-Marseille Université, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, Marseille 13009, France
| |
Collapse
|
187
|
Abstract
F1- and V1-ATPase are rotary molecular motors that convert chemical energy released upon ATP hydrolysis into torque to rotate a central rotor axle against the surrounding catalytic stator cylinder with high efficiency. How conformational change occurring in the stator is coupled to the rotary motion of the axle is the key unknown in the mechanism of rotary motors. Here, we generated chimeric motor proteins by inserting an exogenous rod protein, FliJ, into the stator ring of F1 or of V1 and tested the rotation properties of these chimeric motors. Both motors showed unidirectional and continuous rotation, despite no obvious homology in amino acid sequence between FliJ and the intrinsic rotor subunit of F1 or V1 These results showed that any residue-specific interactions between the stator and rotor are not a prerequisite for unidirectional rotation of both F1 and V1 The torque of chimeric motors estimated from viscous friction of the rotation probe against medium revealed that whereas the F1-FliJ chimera generates only 10% of WT F1, the V1-FliJ chimera generates torque comparable to that of V1 with the native axle protein that is structurally more similar to FliJ than the native rotor of F1 This suggests that the gross structural mismatch hinders smooth rotation of FliJ accompanied with the stator ring of F1.
Collapse
|
188
|
Li J, He G, Ueno H, Jia C, Noji H, Qi C, Guo X. Direct real-time detection of single proteins using silicon nanowire-based electrical circuits. NANOSCALE 2016; 8:16172-16176. [PMID: 27714062 DOI: 10.1039/c6nr04103e] [Citation(s) in RCA: 26] [Impact Index Per Article: 3.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/06/2023]
Abstract
We present an efficient strategy through surface functionalization to build a single silicon nanowire field-effect transistor-based biosensor that is capable of directly detecting protein adsorption/desorption at the single-event level. The step-wise signals in real-time detection of His-tag F1-ATPases demonstrate a promising electrical biosensing approach with single-molecule sensitivity, thus opening up new opportunities for studying single-molecule biophysics in broad biological systems.
Collapse
Affiliation(s)
- Jie Li
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University, Beijing 100875, P. R. China. and Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University, Beijing 100871, P. R. China.
| | - Gen He
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University, Beijing 100875, P. R. China. and Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University, Beijing 100871, P. R. China.
| | - Hiroshi Ueno
- Department of Applied Chemistry, School of Engineering, The University of Tokyo, Tokyo 113-8654, Japan.
| | - Chuancheng Jia
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University, Beijing 100871, P. R. China.
| | - Hiroyuki Noji
- Department of Applied Chemistry, School of Engineering, The University of Tokyo, Tokyo 113-8654, Japan.
| | - Chuanmin Qi
- Key Laboratory of Radiopharmaceuticals, Ministry of Education, College of Chemistry, Beijing Normal University, Beijing 100875, P. R. China.
| | - Xuefeng Guo
- Beijing National Laboratory for Molecular Sciences, State Key Laboratory for Structural Chemistry of Unstable and Stable Species, College of Chemistry and Molecular Engineering, Peking University, Beijing 100871, P. R. China. and Department of Materials Science and Engineering, College of Engineering, Peking University, Beijing 100871, P. R. China
| |
Collapse
|
189
|
Torque, chemistry and efficiency in molecular motors: a study of the rotary-chemical coupling in F1-ATPase. Q Rev Biophys 2016; 48:395-403. [PMID: 26537397 PMCID: PMC4873004 DOI: 10.1017/s0033583515000050] [Citation(s) in RCA: 21] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Abstract] [Key Words] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/24/2022]
Abstract
Detailed understanding of the action of biological molecular machines must overcome the challenge of gaining a clear knowledge of the corresponding free-energy landscape. An example for this is the elucidation of the nature of converting chemical energy to torque and work in the rotary molecular motor of F1-ATPase. A major part of the challenge involves understanding the rotary–chemical coupling from a non-phenomenological structure/energy description. Here we focused on using a coarse-grained model of F1-ATPase to generate a structure-based free-energy landscape of the rotary–chemical process of the whole system. In particular, we concentrated on exploring the possible impact of the position of the catalytic dwell on the efficiency and torque generation of the molecular machine. It was found that the experimentally observed torque can be reproduced with landscapes that have different positions for the catalytic dwell on the rotary–chemical surface. Thus, although the catalysis is undeniably required for torque generation, the experimentally observed position of the catalytic dwell at 80° might not have a clear advantage for the force generation by F1-ATPase. This further implies that the rotary–chemical couplings in these biological motors are quite robust and their efficiencies do not depend explicitly on the position of the catalytic dwells. Rather, the specific positioning of the dwells with respect to the rotational angle is a characteristic arising due to the structural construct of the molecular machine and might not bear any clear connection to the thermodynamic efficiency for the system.
Collapse
|
190
|
Zhang Y, Kersell H, Stefak R, Echeverria J, Iancu V, Perera UGE, Li Y, Deshpande A, Braun KF, Joachim C, Rapenne G, Hla SW. Simultaneous and coordinated rotational switching of all molecular rotors in a network. NATURE NANOTECHNOLOGY 2016; 11:706-712. [PMID: 27159740 DOI: 10.1038/nnano.2016.69] [Citation(s) in RCA: 59] [Impact Index Per Article: 7.4] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/14/2014] [Accepted: 03/31/2016] [Indexed: 06/05/2023]
Abstract
A range of artificial molecular systems has been created that can exhibit controlled linear and rotational motion. In the further development of such systems, a key step is the addition of communication between molecules in a network. Here, we show that a two-dimensional array of dipolar molecular rotors can undergo simultaneous rotational switching when applying an electric field from the tip of a scanning tunnelling microscope. Several hundred rotors made from porphyrin-based double-decker complexes can be simultaneously rotated when in a hexagonal rotor network on a Cu(111) surface by applying biases above 1 V at 80 K. The phenomenon is observed only in a hexagonal rotor network due to the degeneracy of the ground-state dipole rotational energy barrier of the system. Defects are essential to increase electric torque on the rotor network and to stabilize the switched rotor domains. At low biases and low initial rotator angles, slight reorientations of individual rotors can occur, resulting in the rotator arms pointing in different directions. Analysis reveals that the rotator arm directions are not random, but are coordinated to minimize energy via crosstalk among the rotors through dipolar interactions.
Collapse
Affiliation(s)
- Y Zhang
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - H Kersell
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - R Stefak
- CEMES, CNRS, 29 rue J. Marvig, 31055 Toulouse, France
| | - J Echeverria
- CEMES, CNRS, 29 rue J. Marvig, 31055 Toulouse, France
| | - V Iancu
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - U G E Perera
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - Y Li
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - A Deshpande
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - K-F Braun
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
| | - C Joachim
- CEMES, CNRS, 29 rue J. Marvig, 31055 Toulouse, France
| | - G Rapenne
- CEMES, CNRS, 29 rue J. Marvig, 31055 Toulouse, France
- Universite' de Toulouse, UPS, 118 route de Narbonne, 31062 Toulouse, France
| | - S-W Hla
- Physics and Astronomy Department, Nanoscale and Quantum Phenomena Institute, Ohio University, Athens, Ohio 45701, USA
- Center for Nanoscale Materials, Nanoscience and Technology Division, Argonne National Laboratory, Illinois 60439, USA
| |
Collapse
|
191
|
Sakiyama Y, Mazur A, Kapinos LE, Lim RYH. Spatiotemporal dynamics of the nuclear pore complex transport barrier resolved by high-speed atomic force microscopy. NATURE NANOTECHNOLOGY 2016; 11:719-23. [PMID: 27136131 DOI: 10.1038/nnano.2016.62] [Citation(s) in RCA: 110] [Impact Index Per Article: 13.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/21/2015] [Accepted: 03/15/2016] [Indexed: 05/27/2023]
Abstract
Nuclear pore complexes (NPCs) are biological nanomachines that mediate the bidirectional traffic of macromolecules between the cytoplasm and nucleus in eukaryotic cells. This process involves numerous intrinsically disordered, barrier-forming proteins known as phenylalanine-glycine nucleoporins (FG Nups) that are tethered inside each pore. The selective barrier mechanism has so far remained unresolved because the FG Nups have eluded direct structural analysis within NPCs. Here, high-speed atomic force microscopy is used to visualize the nanoscopic spatiotemporal dynamics of FG Nups inside Xenopus laevis oocyte NPCs at timescales of ∼100 ms. Our results show that the cytoplasmic orifice is circumscribed by highly flexible, dynamically fluctuating FG Nups that rapidly elongate and retract, consistent with the diffusive motion of tethered polypeptide chains. On this basis, intermingling FG Nups exhibit transient entanglements in the central channel, but do not cohere into a tightly crosslinked meshwork. Therefore, the basic functional form of the NPC barrier is comprised of highly dynamic FG Nups that manifest as a central plug or transporter when averaged in space and time.
Collapse
Affiliation(s)
- Yusuke Sakiyama
- Biozentrum and the Swiss Nanoscience Institute, University of Basel, Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Adam Mazur
- Research IT, Biozentrum, University of Basel, CH-4056 Basel, Switzerland
| | - Larisa E Kapinos
- Biozentrum and the Swiss Nanoscience Institute, University of Basel, Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| | - Roderick Y H Lim
- Biozentrum and the Swiss Nanoscience Institute, University of Basel, Klingelbergstrasse 70, CH-4056 Basel, Switzerland
| |
Collapse
|
192
|
Chaperonin GroEL–GroES Functions as both Alternating and Non-Alternating Engines. J Mol Biol 2016; 428:3090-101. [DOI: 10.1016/j.jmb.2016.06.017] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/09/2016] [Revised: 06/23/2016] [Accepted: 06/27/2016] [Indexed: 11/21/2022]
|
193
|
Kulish O, Wright AD, Terentjev EM. F1 rotary motor of ATP synthase is driven by the torsionally-asymmetric drive shaft. Sci Rep 2016; 6:28180. [PMID: 27321713 PMCID: PMC4913325 DOI: 10.1038/srep28180] [Citation(s) in RCA: 15] [Impact Index Per Article: 1.9] [Reference Citation Analysis] [Abstract] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/02/2016] [Accepted: 05/31/2016] [Indexed: 11/26/2022] Open
Abstract
F1F0 ATP synthase (ATPase) either facilitates the synthesis of ATP in a process driven by the proton moving force (pmf), or uses the energy from ATP hydrolysis to pump protons against the concentration gradient across the membrane. ATPase is composed of two rotary motors, F0 and F1, which compete for control of their shared γ -shaft. We present a self-consistent physical model of F1 motor as a simplified two-state Brownian ratchet using the asymmetry of torsional elastic energy of the coiled-coil γ -shaft. This stochastic model unifies the physical concepts of linear and rotary motors, and explains the stepped unidirectional rotary motion. Substituting the model parameters, all independently known from recent experiments, our model quantitatively reproduces the ATPase operation, e.g. the ‘no-load’ angular velocity is ca. 400 rad/s anticlockwise at 4 mM ATP. Increasing the pmf torque exerted by F0 can slow, stop and overcome the torque generated by F1, switching from ATP hydrolysis to synthesis at a very low value of ‘stall torque’. We discuss the motor efficiency, which is very low if calculated from the useful mechanical work it produces - but is quite high when the ‘useful outcome’ is measured in the number of H+ pushed against the chemical gradient.
Collapse
Affiliation(s)
- O Kulish
- Cavendish Laboratory, University of Cambridge, Cambridge CB3 0HE, UK
| | - A D Wright
- Cavendish Laboratory, University of Cambridge, Cambridge CB3 0HE, UK
| | - E M Terentjev
- Cavendish Laboratory, University of Cambridge, Cambridge CB3 0HE, UK
| |
Collapse
|
194
|
Dong C, Hu X, Dinu CZ. Current status and perspectives in atomic force microscopy-based identification of cellular transformation. Int J Nanomedicine 2016; 11:2107-18. [PMID: 27274238 PMCID: PMC4876801 DOI: 10.2147/ijn.s103501] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/16/2022] Open
Abstract
Understanding the complex interplay between cells and their biomechanics and how the interplay is influenced by the extracellular microenvironment, as well as how the transforming potential of a tissue from a benign to a cancerous one is related to the dynamics of both the cell and its surroundings, holds promise for the development of targeted translational therapies. This review provides a comprehensive overview of atomic force microscopy-based technology and its applications for identification of cellular progression to a cancerous phenotype. The review also offers insights into the advancements that are required for the next user-controlled tool to allow for the identification of early cell transformation and thus potentially lead to improved therapeutic outcomes.
Collapse
Affiliation(s)
- Chenbo Dong
- Department of Chemical and Biomedical Engineering, West Virginia University, Morgantown, WV, USA
| | - Xiao Hu
- Department of Chemical and Biomedical Engineering, West Virginia University, Morgantown, WV, USA
| | - Cerasela Zoica Dinu
- Department of Chemical and Biomedical Engineering, West Virginia University, Morgantown, WV, USA
| |
Collapse
|
195
|
Miyagi A, Scheuring S. Automated force controller for amplitude modulation atomic force microscopy. THE REVIEW OF SCIENTIFIC INSTRUMENTS 2016; 87:053705. [PMID: 27250433 DOI: 10.1063/1.4950777] [Citation(s) in RCA: 11] [Impact Index Per Article: 1.4] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/05/2023]
Abstract
Atomic Force Microscopy (AFM) is widely used in physics, chemistry, and biology to analyze the topography of a sample at nanometer resolution. Controlling precisely the force applied by the AFM tip to the sample is a prerequisite for faithful and reproducible imaging. In amplitude modulation (oscillating) mode AFM, the applied force depends on the free and the setpoint amplitudes of the cantilever oscillation. Therefore, for keeping the applied force constant, not only the setpoint amplitude but also the free amplitude must be kept constant. While the AFM user defines the setpoint amplitude, the free amplitude is typically subject to uncontrollable drift, and hence, unfortunately, the real applied force is permanently drifting during an experiment. This is particularly harmful in biological sciences where increased force destroys the soft biological matter. Here, we have developed a strategy and an electronic circuit that analyzes permanently the free amplitude of oscillation and readjusts the excitation to maintain the free amplitude constant. As a consequence, the real applied force is permanently and automatically controlled with picoNewton precision. With this circuit associated to a high-speed AFM, we illustrate the power of the development through imaging over long-duration and at various forces. The development is applicable for all AFMs and will widen the applicability of AFM to a larger range of samples and to a larger range of (non-specialist) users. Furthermore, from controlled force imaging experiments, the interaction strength between biomolecules can be analyzed.
Collapse
Affiliation(s)
- Atsushi Miyagi
- U1006 INSERM, Université Aix-Marseille, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, 13009 Marseille, France
| | - Simon Scheuring
- U1006 INSERM, Université Aix-Marseille, Parc Scientifique et Technologique de Luminy, 163 Avenue de Luminy, 13009 Marseille, France
| |
Collapse
|
196
|
Hahn-Herrera O, Salcedo G, Barril X, García-Hernández E. Inherent conformational flexibility of F1-ATPase α-subunit. BIOCHIMICA ET BIOPHYSICA ACTA-BIOENERGETICS 2016; 1857:1392-1402. [PMID: 27137408 DOI: 10.1016/j.bbabio.2016.04.283] [Citation(s) in RCA: 7] [Impact Index Per Article: 0.9] [Reference Citation Analysis] [Abstract] [Key Words] [Subscribe] [Scholar Register] [Received: 01/12/2016] [Revised: 04/12/2016] [Accepted: 04/28/2016] [Indexed: 12/30/2022]
Abstract
The core of F1-ATPase consists of three catalytic (β) and three noncatalytic (α) subunits, forming a hexameric ring in alternating positions. A wealth of experimental and theoretical data has provided a detailed picture of the complex role played by catalytic subunits. Although major conformational changes have only been seen in β-subunits, it is clear that α-subunits have to respond to these changes in order to be able to transmit information during the rotary mechanism. However, the conformational behavior of α-subunits has not been explored in detail. Here, we have combined unbiased molecular dynamics (MD) simulations and calorimetrically measured thermodynamic signatures to investigate the conformational flexibility of isolated α-subunits, as a step toward deepening our understanding of its function inside the α3β3 ring. The simulations indicate that the open-to-closed conformational transition of the α-subunit is essentially barrierless, which is ideal to accompany and transmit the movement of the catalytic subunits. Calorimetric measurements of the recombinant α-subunit from Geobacillus kaustophilus indicate that the isolated subunit undergoes no significant conformational changes upon nucleotide binding. Simulations confirm that the nucleotide-free and nucleotide-bound subunits show average conformations similar to that observed in the F1 crystal structure, but they reveal an increased conformational flexibility of the isolated α-subunit upon MgATP binding, which might explain the evolutionary conserved capacity of α-subunits to recognize nucleotides with considerable strength. Furthermore, we elucidate the different dependencies that α- and β-subunits show on Mg(II) for recognizing ATP.
Collapse
Affiliation(s)
- Otto Hahn-Herrera
- Instituto de Química Universidad Nacional Autónoma de México, Circuito Exterior, Ciudad Universitaria, México 04630, D.F., Mexico
| | - Guillermo Salcedo
- Instituto de Química Universidad Nacional Autónoma de México, Circuito Exterior, Ciudad Universitaria, México 04630, D.F., Mexico
| | - Xavier Barril
- Catalan Institution for Research and Advanced Studies (ICREA), Passeig Lluís Companys 23, 08010 Barcelona, Spain; Departament de Fisicoquímica, Facultat de Farmàcia, Universitat de Barcelona, Barcelona, Spain
| | - Enrique García-Hernández
- Instituto de Química Universidad Nacional Autónoma de México, Circuito Exterior, Ciudad Universitaria, México 04630, D.F., Mexico.
| |
Collapse
|
197
|
Perrino AP, Garcia R. How soft is a single protein? The stress-strain curve of antibody pentamers with 5 pN and 50 pm resolutions. NANOSCALE 2016; 8:9151-8. [PMID: 26732032 DOI: 10.1039/c5nr07957h] [Citation(s) in RCA: 28] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/23/2023]
Abstract
Understanding the mechanical functionalities of complex biological systems requires the measurement of the mechanical compliance of their smallest components. Here, we develop a force microscopy method to quantify the softness of a single antibody pentamer by measuring the stress-strain curve with force and deformation resolutions, respectively, of 5 pN and 50 pm. The curve shows three distinctive regions. For ultrasmall compressive forces (5-75 pN), the protein's central region shows that the strain and stress are proportional (elastic regime). This region has an average Young's modulus of 2.5 MPa. For forces between 80 and 220 pN, the stress is roughly proportional to the strain with a Young's modulus of 9 MPa. Higher forces lead to irreversible deformations (plastic regime). Full elastic recovery could reach deformations amounting to 40% of the protein height. The existence of two different elastic regions is explained in terms of the structure of the antibody central region. The stress-strain curve explains the capability of the antibody to sustain multiple collisions without any loss of biological functionality.
Collapse
Affiliation(s)
- Alma P Perrino
- Instituto de Ciencia de Materiales de Madrid (CSIC), c/ Sor Juana Ines de la Cruz 3, 28049 Madrid, Spain.
| | - Ricardo Garcia
- Instituto de Ciencia de Materiales de Madrid (CSIC), c/ Sor Juana Ines de la Cruz 3, 28049 Madrid, Spain.
| |
Collapse
|
198
|
Contera S. Designer cantilevers for even more accurate quantitative measurements of biological systems with multifrequency AFM. NANOTECHNOLOGY 2016; 27:132501. [PMID: 26901640 DOI: 10.1088/0957-4484/27/13/132501] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/05/2023]
Abstract
Multifrequency excitation/monitoring of cantilevers has made it possible both to achieve fast, relatively simple, nanometre-resolution quantitative mapping of mechanical of biological systems in solution using atomic force microscopy (AFM), and single molecule resolution detection by nanomechanical biosensors. A recent paper by Penedo et al [2015 Nanotechnology 26 485706] has made a significant contribution by developing simple methods to improve the signal to noise ratio in liquid environments, by selectively enhancing cantilever modes, which will lead to even more accurate quantitative measurements.
Collapse
Affiliation(s)
- S Contera
- Oxford Martin Programme on Nanotechnology, Clarendon Laboratory, Physics Department, University of Oxford, Parks Road, Oxford, OX1 3PU, UK
| |
Collapse
|
199
|
Suzuki T, Yamaguchi H, Kikusato M, Matsuhashi T, Matsuo A, Sato T, Oba Y, Watanabe S, Minaki D, Saigusa D, Shimbo H, Mori N, Mishima E, Shima H, Akiyama Y, Takeuchi Y, Yuri A, Kikuchi K, Toyohara T, Suzuki C, Kohzuki M, Anzai JI, Mano N, Kure S, Yanagisawa T, Tomioka Y, Toyomizu M, Ito S, Osaka H, Hayashi KI, Abe T. Mitochonic Acid 5 (MA-5), a Derivative of the Plant Hormone Indole-3-Acetic Acid, Improves Survival of Fibroblasts from Patients with Mitochondrial Diseases. TOHOKU J EXP MED 2016; 236:225-32. [PMID: 26118651 DOI: 10.1620/tjem.236.225] [Citation(s) in RCA: 29] [Impact Index Per Article: 3.6] [Reference Citation Analysis] [Abstract] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/18/2022]
Abstract
Mitochondria are key organelles implicated in a variety of processes related to energy and free radical generation, the regulation of apoptosis, and various signaling pathways. Mitochondrial dysfunction increases cellular oxidative stress and depletes ATP in a variety of inherited mitochondrial diseases and also in many other metabolic and neurodegenerative diseases. Mitochondrial diseases are characterized by the dysfunction of the mitochondrial respiratory chain, caused by mutations in the genes encoded by either nuclear DNA or mitochondrial DNA. We have hypothesized that chemicals that increase the cellular ATP levels may ameliorate the mitochondrial dysfunction seen in mitochondrial diseases. To search for the potential drugs for mitochondrial diseases, we screened an in-house chemical library of indole-3-acetic-acid analogs by measuring the cellular ATP levels in Hep3B human hepatocellular carcinoma cells. We have thus identified mitochonic acid 5 (MA-5), 4-(2,4-difluorophenyl)-2-(1H-indol-3-yl)-4-oxobutanoic acid, as a potential drug for enhancing ATP production. MA-5 is a newly synthesized derivative of the plant hormone, indole-3-acetic acid. Importantly, MA-5 improved the survival of fibroblasts established from patients with mitochondrial diseases under the stress-induced condition, including Leigh syndrome, MELAS (myopathy encephalopathy lactic acidosis and stroke-like episodes), Leber's hereditary optic neuropathy, and Kearns-Sayre syndrome. The improved survival was associated with the increased cellular ATP levels. Moreover, MA-5 increased the survival of mitochondrial disease fibroblasts even under the inhibition of the oxidative phosphorylation or the electron transport chain. These data suggest that MA-5 could be a therapeutic drug for mitochondrial diseases that exerts its effect in a manner different from anti-oxidant therapy.
Collapse
Affiliation(s)
- Takehiro Suzuki
- Division of Nephrology, Endocrinology, and Vascular Medicine, Tohoku University Graduate School of Medicine
| | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | | |
Collapse
|
200
|
Yamato I, Kakinuma Y, Murata T. Operating principles of rotary molecular motors: differences between F 1 and V 1 motors. Biophys Physicobiol 2016; 13:37-44. [PMID: 27924256 PMCID: PMC5042177 DOI: 10.2142/biophysico.13.0_37] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/05/2015] [Accepted: 02/11/2016] [Indexed: 12/01/2022] Open
Abstract
Among the many types of bioenergy-transducing machineries, F- and V-ATPases are unique bio- and nano-molecular rotary motors. The rotational catalysis of F1-ATPase has been investigated in detail, and molecular mechanisms have been proposed based on the crystal structures of the complex and on extensive single-molecule rotational observations. Recently, we obtained crystal structures of bacterial V1-ATPase (A3B3 and A3B3DF complexes) in the presence and absence of nucleotides. Based on these new structures, we present a novel model for the rotational catalysis mechanism of V1-ATPase, which is different from that of F1-ATPases.
Collapse
Affiliation(s)
- Ichiro Yamato
- Department of Biological Science and Technology, Tokyo University of Science, Tokyo 125-8585, Japan
| | - Yoshimi Kakinuma
- Laboratory of Molecular Physiology and Genetics, Faculty of Agriculture, Ehime University, Matsuyama, Ehime 790-8566, Japan
| | - Takeshi Murata
- Department of Chemistry, Graduate School of Science, Chiba University, Chiba 263-8522, Japan; Molecular Chirality Research Center, Chiba University, Chiba 263-8522, Japan; JST, PRESTO, Chiba 263-8522, Japan
| |
Collapse
|