S2 domain gives myosin filaments some flexibility

JGP microscopy study supports the idea that the region linking myosin head and tail domains can be peeled away from filament backbone to prevent actin-attached heads from impeding filament movement.

Myosin II motors move along actin filaments by coupling cycles of ATP binding and hydrolysis to a repetitive process in which the myosin head domains attach to actin, undergo a conformational shift/powerstroke, and then detach. In muscle cells, myosin II molecules assemble into thick filaments containing hundreds of head domains, and any heads that remain attached to actin after completing their power stroke may impede the ability of other heads to move the filament and drive muscle contraction. In this issue of JGP, Brizendine et al. provide direct evidence that this potential drag on filament movement is limited by the flexibility of myosin II’s S2 subdomain (1).(Left to right) Richard Brizendine, Christine Cremo, and Murali Anuganti provide direct evidence that the S2 domain of myosin II is a flexible structure, which would allow it to prevent actin-attached heads from impeding the movement of myosin filaments. Quantum dots labeling a head domain (black) and the filament backbone (red) mostly follow the same trajectory as a filament moves in vitro. But, in rare instances (insets), an actin-attached head briefly lags the backbone’s trajectory before catching up, an event facilitated by the flexibility of the S2 region that connects the motor protein’s head and tail domains.For the past few years, Christine Cremo and colleagues at the University of Nevada, Reno, have been studying the kinetics of filament movement using fluorescently labeled myosin and actin filaments in vitro (2). Based on their data, Cremo’s team, in collaboration with Josh Baker, developed a mixed kinetic model that predicted a key mechanical function for the S2 subdomain of myosin II, which links the motor protein’s head domains to the C-terminal light meromyosin (LMM) domains that mediate filament assembly (3,4). According to the model, the flexibility of the S2 subdomain, and its ability to be peeled away from the filament backbone, provides some slack to actin-attached heads as the filament moves forward, giving them more time to detach before they impede the filament’s progress.“So now we wanted to see if we could directly observe this flexibility,” Cremo explains. To do this, two postdocs in Cremo’s laboratory, Richard Brizendine and Murali Anuganti, assembled smooth muscle myosin filaments labeled with two differently colored quantum dots, one attached to the LMM domain and the other attached to the head domain. Most of the time, these two labels should follow the same trajectory along actin filaments in vitro. If the S2 domain is flexible, however, it should be possible to occasionally observe an actin-attached head remain in place while the LMM domain continues moving forward. This brief “dwell” should then be followed by a “jump” as the head domain detaches from actin and catches up with the trajectory of the filament backbone.“We were looking for rare events in a sea of noise,” Cremo says, yet the researchers were able to identify dwells and jumps in the quantum dot trajectories consistent with the predicted flexibility of the S2 domain. The frequency and duration of these events fit the known kinetics of actomyosin motility.Based on their data, Brizendine et al. (1) estimate that, in smooth muscle, a myosin filament can move up to ∼52 nm without being impeded by an actin-attached head, a figure close to that predicted by the mixed kinetic model. To provide this flexibility, the researchers calculate that as much as 26 nm of the S2 domain can be unzipped from the filament backbone. Intriguingly, this matches the maximum length that S2 can be seen to project from thick filaments in tomograms of Drosophila flight muscle (5), and the forces generated by working myosin heads should be more than sufficient to achieve this unzipping.Many cardiomyopathy-associated mutations are located in the S2 region of myosin II. However, the mixed kinetic model predicts that, compared with smooth muscle, myosin filaments in cardiac and skeletal muscle cannot move quite as far without being impeded by actin-attached heads. “What leads to these differences?” Cremo wonders. “Are there differences in the biophysical behavior of the S2 domain in different muscle types?”     

A model to account for the elastic element in muscle crossbridges in terms of a bending myosin rod

We advance a structural model to account for the rapid elastic element seen in mechanical transient experiments on vertebrate skeletal muscle (A.F. Huxley & Simmons 1971 Nature, Lond. 233, 533-538). In contrast to other crossbridge models, ours does not envisage a myosin rod made up of two rigid portions connected by a hinge, but rather a gradually bending rod portion connecting the heads to the thick filament shaft. We propose that, in relaxed muscle, the subfragment 2 (S2) portion of the myosin rod is bound to the thick filament shaft by ionic interactions analogous to those between the light meromyosin (LMM) portions of the rod that constitute the body of the shaft. These interactions probably involve the alternating zones of positive and negative charge seen in myosin rod amino acid sequences. As the crossbridge cycle that generates tension begins, we propose that part of S2 detaches from the thick filament shaft and bends to enable the myosin head to attach to actin. When tension develops in the crossbridge, the S2 is straightened and more of it becomes detached from the shaft so that the junction between S2 and the myosin heads moves 3-4 nm axially. As tension declines at the end of the crossbridge stroke, we propose that S2 rebinds to the thick filament shaft and that this provides the restoring force to return the junction of the heads and S2 to its original axial position. Thus this movement would have the characteristics of an elastic element; detailed calculations indicate that it would have properties similar to those observed experimentally. Furthermore, this model can account for the radial attractive force seen in rigor and in contracting muscle, the decrease in stiffness when interfilament spacing is increased in skinned muscle, and the increased rate of proteolysis observed at the S2-LMM junction in contracting muscle.     

Structural changes accompanying phosphorylation of tarantula muscle myosin filaments

Electron microscopy has been used to study the structural changes that occur in the myosin filaments of tarantula striated muscle when they are phosphorylated. Myosin filaments in muscle homogenates maintained in relaxing conditions (ATP, EGTA) are found to have nonphosphorylated regulatory light chains as shown by urea/glycerol gel electrophoresis and [32P]phosphate autoradiography. Negative staining reveals an ordered, helical arrangement of crossbridges in these filaments, in which the heads from axially neighboring myosin molecules appear to interact with each other. When the free Ca2+ concentration in a homogenate is raised to 10(-4) M, or when a Ca2+-insensitive myosin light chain kinase is added at low Ca2+ (10(-8) M), the regulatory light chains of myosin become rapidly phosphorylated. Phosphorylation is accompanied by potentiation of the actin activation of the myosin Mg-ATPase activity and by loss of order of the helical crossbridge arrangement characteristic of the relaxed filament. We suggest that in the relaxed state, when the regulatory light chains are not phosphorylated, the myosin heads are held down on the filament backbone by head-head interactions or by interactions of the heads with the filament backbone. Phosphorylation of the light chains may alter these interactions so that the crossbridges become more loosely associated with the filament backbone giving rise to the observed changes and facilitating crossbridge interaction with actin.     

Myosin S2 Origins Track Evolution of Strong Binding on Actin by Azimuthal Rolling of Motor Domain

Myosin crystal structures have given rise to the swinging lever arm hypothesis, which predicts a large axial tilt of the lever arm domain during the actin-attached working stroke. Previous work imaging the working stroke in actively contracting, fast-frozen Lethocerus muscle confirmed the axial tilt; but strongly bound myosin heads also showed an unexpected azimuthal slew of the lever arm around the thin filament axis, which was not predicted from known crystal structures. We hypothesized that an azimuthal reorientation of the myosin motor domain on actin during the weak-binding to strong-binding transition could explain the lever arm slew provided that myosin’s α-helical coiled-coil subfragment 2 (S2) domain emerged from the thick filament backbone at a particular location. However, previous studies did not adequately resolve the S2 domain. Here we used electron tomography of rigor muscle swollen by low ionic strength to pull S2 clear of the thick filament backbone, thereby revealing the azimuth of its point of origin. The results show that the azimuth of S2 origins of those rigor myosin heads, bound to the actin target zone of actively contracting muscle, originate from a restricted region of the thick filament. This requires an azimuthal reorientation of the motor domain on actin during the weak to strong transition.     

Three-dimensional reconstruction of tarantula myosin filaments suggests how phosphorylation may regulate myosin activity

Muscle contraction involves the interaction of the myosin heads of the thick filaments with actin subunits of the thin filaments. Relaxation occurs when this interaction is blocked by molecular switches on these filaments. In many muscles, myosin-linked regulation involves phosphorylation of the myosin regulatory light chains (RLCs). Electron microscopy of vertebrate smooth muscle myosin molecules (regulated by phosphorylation) has provided insight into the relaxed structure, revealing that myosin is switched off by intramolecular interactions between its two heads, the free head and the blocked head. Three-dimensional reconstruction of frozen-hydrated specimens revealed that this asymmetric head interaction is also present in native thick filaments of tarantula striated muscle. Our goal in this study was to elucidate the structural features of the tarantula filament involved in phosphorylation-based regulation. A new reconstruction revealed intra- and intermolecular myosin interactions in addition to those seen previously. To help interpret the interactions, we sequenced the tarantula RLC and fitted an atomic model of the myosin head that included the predicted RLC atomic structure and an S2 (subfragment 2) crystal structure to the reconstruction. The fitting suggests one intramolecular interaction, between the cardiomyopathy loop of the free head and its own S2, and two intermolecular interactions, between the cardiac loop of the free head and the essential light chain of the blocked head and between the Leu305-Gln327 interaction loop of the free head and the N-terminal fragment of the RLC of the blocked head. These interactions, added to those previously described, would help switch off the thick filament. Molecular dynamics simulations suggest how phosphorylation could increase the helical content of the RLC N-terminus, weakening these interactions, thus releasing both heads and activating the thick filament.     

Probing Muscle Myosin Motor Action: X-Ray (M3 and M6) Interference Measurements Report Motor Domain Not Lever Arm Movement

The key question in understanding how force and movement are produced in muscle concerns the nature of the cyclic interaction of myosin molecules with actin filaments. The lever arm of the globular head of each myosin molecule is thought in some way to swing axially on the actin-attached motor domain, thus propelling the actin filament past the myosin filament. Recent X-ray diffraction studies of vertebrate muscle, especially those involving the analysis of interference effects between myosin head arrays in the two halves of the thick filaments, have been claimed to prove that the lever arm moves at the same time as the sliding of actin and myosin filaments in response to muscle length or force steps. It was suggested that the sliding of myosin and actin filaments, the level of force produced and the lever arm angle are all directly coupled and that other models of lever arm movement will not fit the X-ray data. Here, we show that, in addition to interference across the A-band, which must be occurring, the observed meridional M3 and M6 X-ray intensity changes can all be explained very well by the changing diffraction effects during filament sliding caused by heads stereospecifically attached to actin moving axially relative to a population of detached or non-stereospecifically attached heads that remain fixed in position relative to the myosin filament backbone. Crucially, and contrary to previous interpretations, the X-ray interference results provide little direct information about the position of the myosin head lever arm; they are, in fact, reporting relative motor domain movements. The implications of the new interpretation are briefly assessed.     

Calcium regulates scallop muscle by changing myosin flexibility

Muscle myosins are molecular motors that convert the chemical free energy available from ATP hydrolysis into mechanical displacement of actin filaments, bringing about muscle contraction. Myosin cross-bridges exert force on actin filaments during a cycle of attached and detached states that are coupled to each round of ATP hydrolysis. Contraction and ATPase activity of the striated adductor muscle of scallop is controlled by calcium ion binding to myosin. This mechanism of the so-called “thick filament regulation” is quite different to vertebrate striated muscle which is switched on and off via “thin filament regulation” whereby calcium ions bind to regulatory proteins associated with the actin filaments. We have used an optically based single molecule technique to measure the angular disposition adopted by the two myosin heads whilst bound to actin in the presence and absence of calcium ions. This has allowed us to directly observe the movement of individual myosin heads in aqueous solution at room temperature in real time. We address the issue of how scallop striated muscle myosin might be regulated by calcium and have interpreted our results in terms of the structures of smooth muscle myosin that also exhibit thick filament regulation. This paper is not being submitted elsewhere and the authors have no competing financial interests     

The tail of myosin reduces actin filament velocity in the in vitro motility assay

It has been observed that heavy meromyosin (HMM) propels actin filaments to higher velocities than native myosin in the in vitro motility assay, yet the reason for this difference has remained unexplained. Since the major difference between these two proteins is the presence of the tail in native myosin, we tested the hypothesis that unknown interactions between actin and the tail (LMM) slow motility in native myosin. Chymotryptic HMM and LMM were mixed in a range of molar ratios (0-5 LMM/HMM) and compared to native rat skeletal myosin in the in vitro motility assay at 30 degrees C. Increasing proportions of LMM to HMM slowed actin filament velocities, becoming equivalent to native myosin at a ratio of 3 LMM/HMM. NH4+ -ATPase assays demonstrated that HMM concentrations on the surface were constant and independent of LMM concentration, arguing against a simple displacement mechanism. Relationships between velocity and the number of available heads suggested that the duty cycle of HMM was not altered by the presence of LMM. HMM prepared with a lower chymotrypsin concentration and with very short digestion times moved actin at the same high velocity. The difference between velocities of actin filament propelled by HMM and HMM/LMM decreased with increasing ionic strength, suggesting that ionic bonds between myosin tail and actin filaments may play a role in slowing filament velocity. These data suggest the high velocities of actin filaments over HMM result from the absence of drag generated by the myosin tail, and not from proteolytic nicking of the motor domain.     

Dynamic modulation of the regulatory domain of myosin heads by pH, ionic strength, and RLC phosphorylation in synthetic myosin filaments

The position of the myosin head with respect to the filament backbone is thought to be a function of pH, ionic strength (micro) and the extent of regulatory light chain (RLC) phosphorylation [Harrington (1979) Proc. Natl. Acad. Sci. U.S.A. 76, 5066-5070]. The object of this study is to examine the dynamics of the proximal part of the myosin head (regulatory domain) which accompany the changes in head disposition. The essential light chain was labeled at Cys177 with the indanedione spin-label followed by the exchange of the labeled proteins into myosin. The mobility of the labeled domain was investigated with saturation transfer electron paramagnetic resonance in reconstituted, synthetic myosin filaments. We have found that the release of the heads from the myosin filament surface by reduction of electrostatic charge is accompanied by a 2-fold increase in the mobility of the regulatory domain. Phosphorylation of the RLC by myosin light chain kinase resulted in a smaller 1. 5-fold increase of motion, establishing that the head disordering observed by electron microscopy [Levine et al. (1996) Biophys. J. 71, 898-907] is due to increased mobility of the heads. This result indirectly supports the hypothesis that the RLC phosphorylation effect on potentiation of force arises from a release of heads from the filament surface and a shift of the heads toward actin.     

Inhibition of smooth muscle myosin's activity and assembly by an anti-rod monoclonal antibody.

Monoclonal antibodies specific for the rod region can affect smooth muscle myosin's motor properties. Actin movement by phosphorylated myosin was inhibited by an antibody (LMM.4) which binds to the COOH-terminal end of the coiled-coil rod, a region thought to be involved in filament assembly. The actin-activated ATPase activity of the myosin-antibody LMM.4 complex was also reduced 10-fold at actin concentrations that gave maximal turnover rates with filamentous myosin. Metal-shadowing of the phosphorylated myosin-antibody complex at low ionic strength showed small bundles of parallel extended molecules, instead of filaments. Five other anti-rod antibodies had little or no effect on myosin's ability to act as a motor. This is the first demonstration that a muscle myosin's activity is affected by its state of assembly. A common theme that emerges from the studies on both muscle and non-muscle myosins is that assembly into a filamentous structure stimulates the activity of the individual myosin molecules.     

High flexibility of the actomyosin crossbridge resides in skeletal muscle myosin subfragment-2 as demonstrated by a new single molecule assay

Popular views of force generation in muscle indicate that a lever arm in the myosin head initiates displacement of the thin filament. However, this lever arm is attached to the thick filament backbone by a flexible combination of coiled coils and hinges in the myosin subfragment-2 (S2); therefore, efficient force generation depends on tension development in this linking structure. Herein, a single molecule assay is developed to examine the flexibility of the intact S2 relative to that of the myosin head. Fluorescently labeled myosin rod is polymerized onto a single myosin molecule that is bound to actin, and the resulting Brownian motion of the rod is analyzed at video rates by digital image processing. Complete rotations of the rod suggest significant amounts of random coil in the linking structure. The close similarity of twist rates for double-headed and single-headed myosin indicates that most of the flexibility originates at or beyond the first pitch of coiled coil in S2 and most likely at the hinge connecting S2 and the light meromyosin. The myosin head has a smaller but still detectable impact on this flexibility, since the addition of ADP to the rigor crossbridge produces differential effects on the torsional characteristics of double-headed versus single-headed myosin.     

3D structure of relaxed fish muscle myosin filaments by single particle analysis

To understand the structural changes involved in the force-producing myosin cross-bridge cycle in vertebrate muscle it is necessary to know the arrangement and conformation of the myosin heads at the start of the cycle (i.e. the relaxed state). Myosin filaments isolated from goldfish muscle under relaxing conditions and viewed in negative stain by electron microscopy (EM) were divided into segments and subjected to three-dimensional (3D) single particle analysis without imposing helical symmetry. This allowed the known systematic departure from helicity characteristic of vertebrate striated muscle myosin filaments to be preserved and visualised. The resulting 3D reconstruction reveals details to about 55 A resolution of the myosin head density distribution in the three non-equivalent head 'crowns' in the 429 A myosin filament repeat. The analysis maintained the well-documented axial perturbations of the myosin head crowns and revealed substantial azimuthal perturbations between crowns with relatively little radial perturbation. Azimuthal rotations between crowns were approximately 60 degrees , 60 degrees and 0 degrees , rather than the regular 40 degrees characteristic of an unperturbed helix. The new density map correlates quite well with the head conformations analysed in other EM studies and in the relaxed fish muscle myosin filament structure modelled from X-ray fibre diffraction data. The reconstruction provides information on the polarity of the myosin head array in the A-band, important in understanding the geometry of the myosin head interaction with actin during the cross-bridge cycle, and supports a number of conclusions previously inferred by other methods. The observed azimuthal head perturbations are consistent with the X-ray modelling results from intact muscle, indicating that the observed perturbations are an intrinsic property of the myosin filaments and are not induced by the proximity of actin filaments in the muscle A-band lattice. Comparison of the axial density profile derived in this study with the axial density profile of the X-ray model of the fish myosin filaments which was restricted to contributions from the myosin heads allows the identification of a non-myosin density peak associated with the azimuthally perturbed head crown which can be interpreted as a possible location for C-protein or X-protein (MyBP-C or -X). This position for C-protein is also consistent with the C-zone interference function deduced from previous analysis of the meridional X-ray pattern from frog muscle. It appears that, along with other functions, C-(X-) protein may have the role of slewing the heads of one crown so that they do not clash with the neighbouring actin filaments, but are readily available to interact with actin when the muscle is activated.     

3D Structure of fish muscle myosin filaments

Myosin filaments isolated from goldfish (Carassius auratus) muscle under relaxing conditions and viewed in negative stain by electron microscopy have been subjected to 3D helical reconstruction to provide details of the myosin head arrangement in relaxed muscle. Previous X-ray diffraction studies of fish muscle (plaice) myosin filaments have suggested that the heads project a long way from the filament surface rather than lying down flat and that heads in a single myosin molecule tend to interact with each other rather than with heads from adjacent molecules. Evidence has also been presented that the head tilt is away from the M-band. Here we seek to confirm these conclusions using a totally independent method. By using 3D helical reconstruction of isolated myosin filaments the known perturbation of the head array in vertebrate muscles was inevitably averaged out. The 3D reconstruction was therefore compared with the X-ray model after it too had been helically averaged. The resulting images showed the same characteristic features: heads projecting out from the filament backbone to high radius and the motor domains at higher radius and further away from the M-band than the light-chain-binding neck domains (lever arms) of the heads.     

Does the S2 rod of myosin II uncoil upon two-headed binding to actin? A leucine-zippered HMM study

Myosin II, like many molecular motors, is a two-headed dimer held together by a coiled-coil rod. The stability of the (S2) rod has implications for head-head interactions, force generation, and possibly regulation. Whether S2 uncoils has been controversial. To test the stability of S2, we constructed a series of "zippered" dimeric smooth muscle myosin II compounds, containing a high-melting temperature 32-amino acid GCN4 leucine zipper in the S2 rod beginning 0, 1, 2, or 15 heptads from the head-rod junction. We then assessed the ability of these and wild-type myosin to bind strongly via two heads to an actin filament by measuring the fluorescence quenching of pyrene-labeled actin induced by myosin binding. Such two-headed binding is expected to exert a large strain that tends to uncoil S2, and hence provide a robust test of S2 stability. We find that wild-type and zippered heavy meromyosin (HMM) are able to bind by both heads to actin under both nucleotide-free and saturating ADP conditions. In addition, we compared the actin affinity and rates for the 0- and 15-zippered HMMs in the phosphorylated "on" state and found them to be very similar. These results strongly suggest that S2 uncoiling is not necessary for two-headed binding of myosin to actin, presumably due to a compliant point in the myosin head(s). We conclude that S2 likely remains intact during the catalytic cycle.     

Human platelet myosin. II. In vitro assembly and structure of myosin filaments

We have used electron microscopy and solubility measurements to investigate the assembly and structure of purified human platelet myosin and myosin rod into filaments. In buffers with ionic strengths of less than 0.3 M, platelet myosin forms filaments which are remarkable for their small size, being only 320 nm long and 10-11 nm wide in the center of the bare zone. The dimensions of these filaments are not affected greatly by variation of the pH between 7 and 8, variation of the ionic strength between 0.05 and 0.2 M, the presence or absence of 1 mM Mg++ or ATP, or variation of the myosin concentration between 0.05 and 0.7 mg/ml. In 1 mM Ca++ and at pH 6.5 the filaments grow slightly larger. More than 90% of purified platelet myosin molecules assemble into filaments in 0.1 M KC1 at pH 7. Purified preparations of the tail fragment of platelet myosin also form filaments. These filaments are slightly larger than myosin filaments formed under the same conditions, indicating that the size of the myosin filaments may be influenced by some interaction between the head and tail portions of myosin molecules. Calculations based on the size and shape of the myosin filaments, the dimensions of the myosin molecule and analysis of the bare zone reveal that the synthetic platelet myosin filaments consists of 28 myosin molecules arranged in a bipolar array with the heads of two myosin molecules projecting from the backbone of the filament at 14-15 nm intervals. The heads appear to be loosely attached to the backbone by a flexible portion of the myosin tail. Given the concentration of myosin in platelets and the number of myosin molecules per filament, very few of these thin myosin filaments should be present in a thin section of a platelet, even if all of the myosin molecules are aggregated into filaments.     

Millisecond time-resolved changes occurring in Ca2+-regulated myosin filaments upon relaxation

Contraction of many muscles is activated in part by the binding of Ca²⁺ to, or phosphorylation of, the myosin heads on the surface of the thick filaments. In relaxed muscle, the myosin heads are helically ordered and undergo minimal interaction with actin. On Ca²⁺ binding or phosphorylation, the head array becomes disordered, reflecting breakage of the head-head and other interactions that underlie the ordered structure. Loosening of the heads from the filament surface enables them to interact with actin filaments, bringing about contraction. On relaxation, the heads return to their ordered positions on the filament backbone. In scallop striated adductor muscle, the disordering that takes place on Ca²⁺ binding occurs on the millisecond time scale, suggesting that it is a key element of muscle activation. Here we have studied the reverse process. Using time-resolved negative staining electron microscopy, we show that the rate of reordering on removal of Ca²⁺ also occurs on the same physiological time scale. Direct observation of images together with analysis of their Fourier transforms shows that activated heads regain their axial ordering within 20 ms and become ordered in their final helical positions within 50 ms. This rapid reordering suggests that reformation of the ordered structure, and the head-head and other interactions that underlie it, is a critical element of the relaxation process.     

The two actin-binding regions on the myosin heads of cardiac muscle

In the presence of myosin S1 or myosin heads, actin filaments tend to form bundles. The biological meaning of the bundling of actin filaments has been unclear. In this study, we found that the cardiac myosin heads can form the bundles of actin filaments more rapidly than can skeletal S1, as monitored by light scattering and electron microscopy. Moreover, the actin bundles formed by cardiac S1 were found to be more stable against mechanical agitation. The distance between actin filaments in the bundles was approximately 20 nm, which is comparable to the length of a myosin head and two actin molecules. This suggests the direct binding of S1 tails to the adjacent actin filament. The "essential" light chain of cardiac myosin could be cross-linked to the actin molecule in the bundle. When monomeric actin molecules were added to the bundle, the bundles could be dispersed into individual filaments. The three-dimensional structure of the dispersed actin filaments was reconstructed from electron cryo-microscopic images of the single actin filaments dispersed by monomer actin. We were able to demonstrate that cardiac myosin heads bind to two actin molecules: one actin molecule at the conventional actin-binding region and the other at the essential light-chain-binding region. This capability of cardiac myosin heads to bind two actin molecules is discussed in view of lower ATPase activity and slower shortening velocity than those of skeletal ones.     

Packing of myosin molecules in muscle thick filaments

The backbone of the myosin filament is an aggregate of alpha-helical coiled coil myosin rods. Its surface forms a three-stranded helix composed of myosin heads. Currently there is no adequate model to describe the organization of the myosin filament. It is proposed here that, in cross-section the light meromyosin (LMM) of 18 myosin molecules form an outer tube, with nine S2 forming the interior core. At the surface of the thick filament, myosin heads are arranged in three rows, giving the filament a periodicity of 14.3 nm per three myosin molecules. Two of these molecules are organized at an angle of 120 degrees to each other on the same level, while the third is shifted 7.2 nm along the filament axis. This packing gives a striation pattern of 7.2 nm by electron microscopy. An alternative model is also possible, in which the heads of the myosin molecules are uniformly spaced at an interval of 14.3 nm along the filament axis. The packing of individual molecules within the myosin filament is based on a regular pattern of charge on the 28 amino-acid repeat in the rod domain.     

Electron microscopic evidence for the myosin head lever arm mechanism in hydrated myosin filaments using the gas environmental chamber

Muscle contraction results from an attachment–detachment cycle between the myosin heads extending from myosin filaments and the sites on actin filaments. The myosin head first attaches to actin together with the products of ATP hydrolysis, performs a power stroke associated with release of hydrolysis products, and detaches from actin upon binding with new ATP. The detached myosin head then hydrolyses ATP, and performs a recovery stroke to restore its initial position. The strokes have been suggested to result from rotation of the lever arm domain around the converter domain, while the catalytic domain remains rigid. To ascertain the validity of the lever arm hypothesis in muscle, we recorded ATP-induced movement at different regions within individual myosin heads in hydrated myosin filaments, using the gas environmental chamber attached to the electron microscope. The myosin head were position-marked with gold particles using three different site-directed antibodies. The amplitude of ATP-induced movement at the actin binding site in the catalytic domain was similar to that at the boundary between the catalytic and converter domains, but was definitely larger than that at the regulatory light chain in the lever arm domain. These results are consistent with the myosin head lever arm mechanism in muscle contraction if some assumptions are made.     

Disorder induced in nonoverlap myosin cross-bridges by loss of adenosine triphosphate.

Adenosine triphosphate-dependent changes in myosin filament structure have been directly observed in whole muscle by electron microscopy of thin sections of rapidly frozen, demembranated frog sartorius specimens. In the presence of ATP the thick filaments show an ordered, helical array of cross-bridges except in the bare zone. In the absence of ATP they show two distinct appearances: in the region of overlap with actin, there is an ordered, rigorlike array of cross-bridges between the thick and thin filaments, whereas in the nonoverlap region (H-zone) the myosin heads move away from the thick filament backbone and lose their helical order. This result suggests that the presence of ATP is necessary for maintenance of the helical array of cross-bridges characteristic of the relaxed state. The primary effect of ATP removal on the myosin heads appears to be weaken their binding to the thick filament backbone; released heads that are close to an actin filament subsequently form a new actin-based, ordered array.