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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Cell. Author manuscript; available in PMC Jan 9, 2010.
Published in final edited form as:
PMCID: PMC2768392
The Mechanism of Kinesin Regulation by Ca++ for Control of Mitochondrial Motility
Xinnan Wang and Thomas L. Schwarz*
F. M. Kirby Neurobiology Center, Children’s Hospital Boston, and Department of Neurobiology, Harvard Medical School, Boston, MA 02115, USA.
Cells regulate mitochondrial movement in order to distribute mitochondria properly and thereby meet the changing energy needs of each region of the cell. Ca++ signaling, which halts both anterograde and retrograde mitochondrial motion, is one such regulation. We show that the EF-hands of Miro mediate this arrest and elucidate the regulatory mechanism of the motor kinesin-1. Kinesin-1 remains on mitochondria whether they are stationary, moving anterograde, or moving retrograde and the protein complex that couples kinesin-1 to mitochondria is not dissociated by elevated Ca++. Instead, Ca++-binding to Miro permits Miro to interact directly with the motor domain, thereby preventing motor/microtubule interactions. This switching mechanism allows Ca++ to regulate mitochondrial motility via two kinesin states: an active state in which kinesin is bound to mitochondria via its tail and milton, and an inactive state in which the motor domain binds directly Miro. Disrupting this regulation diminishes neuronal resistance to excitotoxicity.
Molecular motors are responsible for distributing proteins and organelles within the cell. To achieve the correct spatial distribution of these cargos, and to change that distribution in response to changing conditions, these motors need to be precisely regulated. Although great progress has been made in identifying molecular motors and studying the biophysical mechanisms of their movement, much less is known about how these motors are regulated (Gross et al., 2007). The dynamic regulation of motors is especially important for mitochondria, which are frequently in motion. Particularly in neurons, whose highly extended processes are highly dependent on organelle transport, regulation of motors permits mitochondria to redistribute themselves to balance the changing energy needs of each portion of the cell (Hollenbeck and Saxton, 2005).
All cells depend on mitochondria for local ATP supply and Ca++ buffering. In neuronal axons and dendrites these requirements need to be addressed locally and not by diffusion from distant cell bodies. Consequently, defects in mitochondrial distribution can underlie neurodegenerative disease (Chen and Chan, 2006; Petrozzi et al., 2007). Moreover, because the demand for energy and the need for Ca++ buffering differ from one neuron to another and indeed from one part of the neuron to another part, the density of mitochondria differs between neurons and within a single neuron. The task of distributing mitochondria properly in a neuron to balance changing energy needs may therefore require particularly dynamic regulation.
Reflecting the dynamic nature of these organelles, many axonal mitochondria are in motion, traveling both long and short distances and starting and stopping often (Chang et al., 2006; Hollenbeck and Saxton, 2005; Overly et al., 1996). The majority of these movements are microtubule-based, either anterograde, toward the (+)-ends of the microtubules in the periphery, or retrograde, toward the (-)-ends in the cell bodies. The behavior of mitochondria is therefore primarily governed by the interplay of (+)-end directed kinesin motors, the (-)-end directed dynein motor, and tethering proteins that may hold mitochondria in place (Chada and Hollenbeck, 2003, 2004; Hollenbeck and Saxton, 2005; Kang et al., 2008; Morris and Hollenbeck, 1995). How multiple motors on an organelle are coordinated is not yet understood.
Kinesin-1, the conventional kinesin whose motor domain resides in kinesin heavy chain (KHC), appears to be the primary anterograde motor for mitochondria (Glater et al., 2006; Hurd and Saxton, 1996; Pilling et al., 2006; Tanaka et al., 1998). We previously demonstrated the existence of a motor/adaptor complex containing KHC and two proteins, milton and Miro, that are also essential for the axonal transport of mitochondria (Figure 1A) (Glater et al., 2006; Stowers et al., 2002). KHC is recruited to mitochondria by binding to milton, which in turn binds to the cytoplasmic surface of the mitochondrion by interacting with Miro, a transmembrane protein of the outer-mitochondrial membrane (Fransson et al., 2003; Fransson et al., 2006; Glater et al., 2006; Guo et al., 2005). This complex is conserved from flies to mammals (Beck et al., 2002; Brickley et al., 2005; Fransson et al., 2003; Glater et al., 2006; Stowers et al., 2002) and is likely to govern aspects of mitochondrial distribution in many cell types, including neurons (Glater et al., 2006; Guo et al., 2005; Stowers et al., 2002), oocytes (Cox and Spradling, 2006) and muscle (Guo et al., 2005). In yeast, a homolog of Miro (GEM1p) also influences mitochondrial distribution (Frederick et al., 2004). A regulatory role is indicated for Miro by its Ca++-binding sites and Rho-like GTPase domains and for milton by its post-translational modifications and splicing variants.
Figure 1
Figure 1
Milton Recruits KHC to Neuronal Mitochondria
Several intracellular signals have been shown to control the movement of mitochondria and thereby influence mitochondrial distribution (Boldogh and Pon, 2007; Chada and Hollenbeck, 2003, 2004; Kang et al., 2008). The most widely studied of these is intracellular Ca++ which, when elevated, arrests microtubule-based mitochondrial movement in many cell types (Chang et al., 2006; Hollenbeck and Saxton, 2005; Rintoul et al., 2003; Szabadkai et al., 2006; Yi et al., 2004), although the bulk of fast axonal transport persists in the presence of Ca++ (Brady et al., 1984). Ca++ influx occurs in regions of high metabolic demand, such as nerve terminals and postsynaptic specializations where the extrusion of ions is energetically expensive and where mitochondria are concentrated. In addition, sustained elevated cytosolic Ca++ may be a symptom of insufficient local ATP to power Ca++ export across the plasma membrane, or impaired buffering capacity of mitochondria due to decreased activity of the electron transport chain. Thus a tendency for mitochondria to arrest where Ca++ is elevated will cause them to be retained where energy requirements are high and supplies are low and will thereby balance ATP production to local need. How Ca++ halts mitochondrial motility is presently unknown.
Because Miro contains a pair of EF-hand Ca++-binding motifs, we hypothesized that the KHC/milton/Miro complex would mediate the Ca++-dependent regulation of mitochondrial motility. By examining mitochondrial movement in transfected neurons, we here show that the EF-hands are essential for this regulation and elucidate the mechanism of kinesin inhibition.
Milton Recruits KHC to Neuronal Mitochondria
Previous work from this lab and others has established that milton, Miro, and KHC, whether from Drosophila or mammals, coprecipitate when expressed in cell lines (Beck et al., 2002; Brickley et al., 2005; Fransson et al., 2003; Glater et al., 2006; Stowers et al., 2002). Endogenous mammalian KHC, milton and Miro also coprecipitated as a complex from HEK293T cells (Figure 1B). Furthermore, in transfected COS cells, overexpressed KHC will be recruited onto mitochondria only if milton is co-expressed and that milton binding to mitochondria is mediated by Miro (Glater et al., 2006), supporting the model in Figure 1A. Because milton and Miro mutations prevent anterograde transport of mitochondria in Drosophila axons and because milton and KHC co-precipitate from Drosophila head extracts, we have presumed that the same complex mediated the mitochondrial association of KHC in neurons. To test this hypothesis, we have transfected rat hippocampal neurons with a fluorescently tagged KHC (KHC-mCit), Miro-Myc, and an RFP tagged mitochondrial-import sequence (RFP-mito) (Colwill et al., 2006; Fransson et al., 2006; Cai et al., 2007), in the presence or absence of co-transfected milton. The specificity of RFP-mito as a mitochondrial marker in these cultures was ascertained by costaining with a mitochondrial dye and antibodies to the mitochondrial protein Miro (Figure S1). We found that KHC-mCit was diffusely distributed in neuronal processes unless milton was also present, in which case it became highly concentrated on mitochondria (Figure 1C). Thus, milton in neurons can also serve as an adaptor protein for the recruitment of KHC to mitochondria. In the absence of milton, Miro is inadequate to recruit KHC to the mitochondria in either neurons (Figure 1C) or COS cells (Figure S2). This model implies that there is no direct interaction between KHC and Miro. We confirmed this model by immunoprecipitation of tagged KHC and Miro from transfected HEK cells. Immunoprecipitation of KHC efficiently precipitated Miro only if milton was co-expressed (Figure 1D). On longer exposures, low levels of Miro-KHC association were sometimes seen without milton coexpression; these low levels of association were probably mediated by endogenous milton. Thus milton appears to be essential for connecting KHC to Miro on the mitochondrial surface.
Cytosolic Ca++ Regulates Mitochondrial Motility in Hippocampal Axons
In order to study the regulation of mitochondrial motility by Ca++ and the KHC/milton/Miro complex, mitochondrial movements were examined in cultured rat hippocampal neurons sparsely transfected with RFP-mito. Because axons have a largely uniform microtubule polarity with (+)- ends located distally, we restricted our analysis to axons and identified them by cotransfection with the axonally restricted synaptic vesicle marker, synaptophysin (SYP)-YFP (Chang et al., 2006) (Figure 2A). Axons could also be distinguished from dendrites by their greater length, thin and uniform diameter, sparse branching, and prominent growth cones (Chang et al., 2006). The polarity of an axon was determined by tracing it back to its cell body or forward to its growth cone. Neither significant bleaching nor damage to the mitochondria was observed during 2 hours of imaging. The average velocities of moving mitochondria were: anterograde 0.12±0.01μm/s (n=32 mitochondria), retrograde 0.12±0.01μm/s (n=40). The mitochondria were in anterograde motion 14±2.6% of the time and retrograde 15±2.4% (n=152). The average mitochondrial length was 1.6±0.1μm (n=111) (see Experimental Procedures for analytic methods). These parameters are comparable to previously published values in cultured hippocampal neurons (Overly et al., 1996).
Figure 2
Figure 2
Ca++ Influx Inhibits Axonal Transport of Hippocampal Mitochondria
Increasing cytosolic Ca++ can reduce mitochondrial movements in many cell types (Chang et al., 2006; Yi et al., 2004), a phenomenon that is independent of mitochondrial membrane potential (Yi et al., 2004). To determine if hippocampal mitochondria were similarly regulated, we increased global intracellular Ca++ by applying the calcium ionophore calcimycin (10 μM) in a saline containing 1.8 mM Ca++. Within 5 minutes of calcimycin addition to the cultures, an obvious decrease of mitochondrial motility (Figure 2B, Movie S1, Table S1), but not synaptic vesicular motility (visualized with SYP-YFP, Figure S3, Table S2), could be observed.
Disruption of the EF Hands in Miro Prevents the Ca++-induced Arrest of Axonal Mitochondria
To determine whether the EF-hands in this motor/adaptor complex mediate the Ca++-dependent regulation of mitochondrial transport, we compared wildtype Miro to a mutated version (MiroKK) in which the EF-hands have been disrupted by changing essential glutamates in the Ca++-binding sequence to lysines (Fransson et al., 2006). Each construct was cotransfected with RFP-mito in rat hippocampal neurons and the axonal transport of mitochondria was examined. The location and morphology of axonal mitochondria were grossly normal in both cases when compared to control cultures only expressing RFP-mito (compare Figures Figures22 and and3).3). In this regard, neuronal expression differed from what we and others have observed in COS cells where overexpression of either Miro construct caused perinuclear accumulations of mitochondria (Fransson et al., 2006; data not shown). The fraction of time axonal mitochondria were in motion was not significantly different for either construct when compared to cells without transfected Miro, for either anterograde (12±2.4% Miro, n=145 and 17±2.8% MiroKK, n=156) or retrograde (14±2.6% Miro, n=145 and 13±2.6% MiroKK, n=156) movements. Similarly, their average velocities, lengths, and frequencies of stopping or reversing directions were unaltered by the expression of either wildtype Miro or MiroKK (Table S1, Figure S4).
Figure 3
Figure 3
EF-hand Mutations in Miro Prevent the Inhibition by Ca++ of Mitochondrial Axonal Transport
Addition of calcimycin to raise cytosolic Ca++ reduced bidirectional axonal transport of mitochondria in Miro-overexpressing cells, but mitochondria remained highly motile in MiroKK-expressing cells (Figure 3, Movies S2, S3). Notably, movement persisted in both the anterograde (presumably kinesin-mediated) and retrograde (presumably dynein-mediated) directions (see Discussion). We analyzed the movement parameters before and after the increase of Ca++, comparing control neurons to those expressing either wildtype Miro or MiroKK. We did not observe any significant change in the length of mitochondria upon the addition of calcimycin within the time window for which mitochondrial movements were analyzed (Figure S4A, Table S1), suggesting that the mitochondria we analyzed were morphologically healthy and had not undergone swelling or abnormal fission-and-fusion. The velocities of mitochondria moving in either direction were not significantly different between Miro and MiroKK-overexpressing axons, neither before nor after the increase of cytosolic Ca++ (Figure S4B, Table S1). However, the percent of time mitochondria move was significantly decreased in axons expressing Miro but not MiroKK after the increase of cytosolic Ca++ (Figure 3C, Table S1). Thus, although the basic characteristics of mitochondrial dynamics were unaltered by those mutations, the Ca++-dependent regulation of that motility was prevented by disrupting the EF-hands of Miro.
Ca++ Does Not Disrupt the Association of KHC with the milton/Miro Complex or Mitochondria
Because anterograde, microtubule-based motility of mitochondria depends on their attachment to KHC via the adaptor complex containing milton and Miro, we hypothesized that Ca++-binding to Miro might arrest movement by dissociating the complex and thereby releasing mitochondria from their motor. To test this hypothesis, we co-transfected neurons with mCit-tagged KHC and milton, in addition to Miro or MiroKK. KHC-mCit was localized to mitochondria both before and after calcimycin addition, in both Miro/milton/KHC and MiroKK/milton/KHC transfected axons (Figure 4A, B). The fluorescent intensities of KHC-mCit on mitochondria were not significantly changed after calcimycin addition (Figure 4C). Thus there was no indication that increased cytosolic Ca++ released KHC from the mitochondria. We compared the movement of KHC-mCit and RFP-mito, both before and after calcimycin addition and found that KHC-mCit puncta always moved together with RFP-mito regardless of the direction of movement and was also colocalized with stationary mitochondria. They remained associated with mitochondria before and after calcimycin addition and in both wildtype and mutated Miro (Figures 4D-F, S4A-B, Table S1, Movies S4, S5). The invariant association of KHC with mitochondria indicates that neither the Ca++-dependency of movement nor the choice of anterograde vs. retrograde movement is governed by the association and dissociation of this motor. These physiological observations were also supported by a biochemical analysis of the KHC/milton/Miro complex. High Ca++ did not prevent the three components (milton, Miro and KHC) from coprecipitating when coexpressed in HEK cells (Figure 4G). In a further test of the Ca++-dependence of KHC association with mitochondria, we prepared a mitochondrial fraction from rat hippocampal neurons and determined the level of KHC present after washing with either 0 or 2mM Ca++. High Ca++ did not dissociate KHC from the mitochondria (Figure 4H).
Figure 4
Figure 4
All Axonal Mitochondria Have KHC
Ca++ Binding to Miro Interferes with KHC Binding to Microtubules
Because the motor/adaptor complex was not disrupted by elevated Ca++ and KHC remained associated with mitochondria, we hypothesized that the Ca++ might instead regulate via Miro the ability of KHC to interact with microtubules. To test this hypothesis, we performed microtubule cosedimentation experiments. HEK cells transfected with KHC alone, or cotransfected with milton and Miro, were lysed and incubated with polymerized microtubules in either 0 or 2 mM Ca++ buffer. The microtubules and any bound proteins were pelleted through a sucrose cushion. When KHC was present without cotransfected milton and Miro, it was exclusively found in the microtubule pellet, whether or not Ca++ was present (Figure 5). When KHC was coexpressed with milton and Miro, however, Ca++ caused a substantial shift of KHC, together with its adaptor proteins milton and Miro, to the soluble fraction. This shift was observed only when wildtype Miro was expressed; when KHC was coexpressed with the EF-hand-disrupted MiroKK mutant, KHC remained in the microtubule pellet, even in 2 mM Ca++. Thus Ca++, via the EF-hands of Miro, can cause KHC to dissociate from microtubules.
Figure 5
Figure 5
Ca++, via Miro, Releases KHC from Microtubules
Ca++-dependent Binding of Miro to the N-terminal Motor Domain of KHC
Heretofore, the only interaction observed between Miro and KHC was mediated by milton, which binds to the C-terminus of KHC (Figure 1A) (Glater et al., 2006), whereas the N-terminus of KHC interacts with microtubules. How then do the EF hands of Miro regulate the interaction of KHC with microtubules? We investigated the possibility that Ca++ induced a direct interaction of Miro and KHC, and found that Miro and KHC would indeed co-precipitate in elevated Ca++ even in the absence of cotransfected milton (Figure 6A-C), although in Ca++-free conditions milton was required. This Ca++-dependent interaction was mediated by the EF hands of Miro; MiroKK did not substantially coprecipitate with KHC in either the presence or absence of Ca++ unless milton was present (Figure 6A-C).
Figure 6
Figure 6
Binding of the Kinesin Motor Domain to Microtubules is Inhibited by Ca++-dependent Interactions with Miro
To test if the Ca++-dependent coprecipitation of Miro and KHC was a direct interaction or mediated by endogenous milton, and to map the region of interaction, we used truncated KHC (Figure 6D-F). KHC(1-682) lacks the milton-binding site (810-891 of the KHC tail (Glater et al., 2006)). MiroΔTM deletes mitochondrial anchoring the domain (TM, transmembrane domain) of Miro (Glater et al., 2006). The truncated KHC bound MiroΔTM in a Ca++-dependent way, and these interactions were prevented by mutation of the EF hands (Figure 6D-F). These data indicate that the association of KHC and Miro is not dependent on the milton-binding domain of KHC or on a mitochondrial localization for Miro. Indeed, when a construct encoding only the N-terminal motor domain of KHC was coexpressed with Miro they exhibited Ca++-dependent coprecipitation (Figure 6G-H). Thus, Miro interacts with KHC in two ways: the tail of KHC is linked to Miro by milton in a Ca++-independent manner and the motor domain can interact directly with Miro in the presence of Ca++.
The KHC Motor Domain Bound to Miro Does Not Bind to Microtubules
The ability of Miro to bind the motor domain in the presence of Ca++ suggested that a direct competition between Miro and microtubules might explain the regulation of anterograde transport by Ca++: the interaction of Miro with the motor domain could cause that domain to dissociate from microtubules. We transfected a truncated KHC containing only the motor domain into HEK cells, together with Miro or MiroKK, and performed microtubule cosedimentation experiments as above. Consistently, using Miro-transfected cell lysates, high Ca++ shifted the motor domain from the microtubule pellet to the supernatant. This shift was not observed with MiroKK-transfected cell lysates (Figure 6I, J). Thus, in a manner mediated by the EF-hands, Ca++-induced binding of Miro to the KHC motor domain, prevents the motor domain from binding to microtubules.
The Switching of the KHC Motor Between Miro- and Microtubule-bound States is Ca++-Concentration Dependent
We determined the range of Ca++ concentrations over which Miro could influence the microtubule binding of the motor domain. Microtubule cosedimentations, as described above, were conducted in a series of Ca++ concentrations ranging from 0 to 2 mM. The amount of the motor domain bound to microtubules decreased in a concentration-dependent manner, with a 50% reduction in binding occurring in 50 μM free Ca++ (Figure 6K, M). The Ca++-dependent binding of the motor domain to Miro showed a reciprocal concentration-dependence, with 50% of maximal binding also occurring in 50 μM free Ca++ (Figure 6L, M). The similarity of the concentration-dependences is consistent with a model in which Ca++ binding to the EF hands permits Miro to interact with the motor domain and thereby inhibits the binding of KHC to microtubules. This inhibition can account for the Ca++-dependent arrest of anterograde movement of mitochondria, despite the continued association of KHC with the organelle. One prediction of this model is that overexpression of the KHC motor domain alone might compete with endogenous KHC for binding to Miro and thereby interfere with the Ca++-induced arrest of mitochondrial motility. Overexpression of the motor domain had little effect on the properties of mitochondrial movement in axons prior to calcimycin but did indeed prevent Ca++-dependent arrest of mitochondria (Figure S4C, D, Table S3). This observation is consistent with a required interaction of the endogenous motor domain and Miro for disengaging KHC from microtubules.
The EF-hands of Miro Mediate Glutamatergic Regulation of Mitochondrial Motility and are Protective during Excitotoxic Stresses
Glutamatergic synaptic transmission causes Ca++ influx in dendrites and the application of glutamate has been shown to arrest dendritic mitochondria in a Ca++-dependent maner (Chang et al., 2006; Li et al., 2004). Therefore, to determine whether a physiologically relevant response to a Ca++ signal was mediated by the same mechanism as the calcimycin response, we examined the effects of glutamate application to dendrites of MiroKK—expressing neurons. Whereas the percentage of time mitochondria were motion was significantly decreased by glutamate in dendrites expressing Miro, no such inhibition of movement was observed when MiroKK was expressed (Figure 7A-B, Table S4). As observed in axons (Figs, (Figs,33 and and4),4), both anterograde and retrograde movements became Ca++ resistant in the presence of MiroKK.
Figure 7
Figure 7
The EF-hands of Miro Mediate Responses of Dendritic Mitochondria to Glutamate and Protect against Excitotoxicity
In considering the physiological significance of this Ca++ effect, we hypothesized that regulation via Miro permits mitochondria to concentrate in sites of high energy demand, where cytosolic Ca++ is elevated and in regions where mitochondrial buffering of Ca++ is required. This hypothesis predicts that MiroKK-transfected neurons would be more susceptible to glutamate excitotoxicity because they would not redistribute mitochondria appropriately. To test this hypothesis, we applied the glutamate-receptor agonist and excitotoxin, NMDA (N-methyl-D-aspartic acid) to Miro or MiroKK-transfected neurons for 5 minutes. Transfected neurons were identified by coexpression of GFP and the concentration/sensitivity of the survival of GFP-expressing neurons was examined 24 h after NMDA incubation. In the absence of NMDA, counts of GFP-alone, GFP/Miro, and GFP/MiroKK-transfected neurons were similar at 24 h and GFP/MiroKK cultures remained healthy for several weeks. Exposure to 3, 10, or 30 μM NMDA reduced the numbers of surviving neurons in all conditions, but survival of GFP/MiroKK neurons was significantly worse than those expressing GFP alone or GFP and Miro. At 30μM NMDA application, approximately 40% of GFP-alone and GFP/Miro-transfected neurons survived, but only 20% of GFP/MiroKK-transfected neurons (Figure 7 C-D). Thus, the ability of the EF-hands of Miro to respond to Ca++ protects neurons during excitotoxic challenge.
Kinesin motors drive the movements of chromosomes during mitosis and of proteins and organelles in postmitotic cells To accomplish these tasks, their activities must be carefully regulated and recent work has begun to reveal the diversity of mechanisms that orchestrate the kinesins, either through regulation of motor activity or cargo association (Adio et al., 2006; Cai et al., 2007). In addressing how Ca++ regulates kinesin-1 in the context of mitochondrial motility, we have determined 1) that the EF-hands of Miro are essential for the Ca++-dependent arrest of axonal mitochondria, whether induced by calcimycin or glutamate, but did not noticeably alter any other aspect of their movements; 2) that kinesin heavy chain remains on mitochondria regardless of whether they are moving or stationary, whether they are moving to (+) or (-) ends, or whether Ca++ is at resting or elevated levels; 3) that Ca++, via interaction with Miro, causes the kinesin heavy chain to lose its association with microtubules; 4) that this dissociation arises from the Ca++-dependent binding of the motor domain to Miro; 5) that the EF-hands of Miro mediate the arrest of retrograde as well as anterograde movement of mitochondria; and 6) that this effect enhances neuronal survival under conditions of excitotoxic stress.
The regulation of mitochondrial kinesin-1 can be viewed as a switch between two states of the motor adaptor complex (Figure 7E). In the “on” state, KHC is bound to the mitochondrion by the interaction of its C-terminal tail with milton, which is in turn bound to Miro on the mitochondrial surface. This conformation leaves the N-terminal motor domain of KHC free to interact with microtubules and accomplish anterograde movement. In the “off” state, an additional, direct interaction occurs between the motor domain of KHC and Miro that prevents interactions with microtubules. In other EF-hand proteins, Ca++ binding induces a major conformational change (Nelson and Chazin, 1998), and we presume that a similar change in the structure of Miro drives the switch between the “on” and “off” states of the complex. The interaction of the KHC motor domain with Miro may inhibit microtubule binding either by steric interference with the microtubule binding site or by an allosteric change in the structure of the motor domain.
This regulatory mechanism is distinct from those that have previously been described for kinesin-1 in other contexts. The binding of kinesin light chains to the tail domain, for example, can induce a closed, inactive state and cargo-binding can relieve that inhibition (Cai et al., 2007; Reed et al., 2006). However, at least in Drosophila, mitochondrial transport in axons is independent of the light chain and the light chain is not present in the KHC/milton/Miro complex (Glater et al., 2006). Moreover, we found no evidence for a change in cargo association: mitochondria retained KHC under all the conditions studied (Figures (Figures4,4, ,6).6). Although the kinesin regulation reported here is unlike any previously described for a kinesin-1 or indeed any animal kinesin, it may bear some resemblance to the interactions of the Kinesin-like Calmodulin Binding Protein (KCBP) of plants, an unusual minus-end directed motor. The motor region of KCBP can bind either calmodulin or a related protein, KIC, via their EF hands and in a Ca++-dependent manner (Vinogradova et al., 2004). This binding reaction releases the motor from the microtubule pellet to the supernatant in microtubule-binding assays (Deavours et al., 1998). The EF hands of Miro may similarly bind directly to the motor domain of KHC and interfere with microtubule binding by a comparable mechanism. In a broader sense, the regulation of KHC by Miro also resembles myosin V regulation by calmodulin (Homma et al., 2000).
The complex regulation of mitochondrial distribution is likely to reflect the diverse functions of mitochondria in signaling and energy supply. Ca++-dependent arrest of mitochondrial motility is observed in many cell types, and likely represents a means to two distinct ends: the positioning of mitochondria where they are most needed for Ca++-buffering and the recruitment of mitochondria to cellular regions with insufficient ATP supply. Where ATP is low, Ca++-transport mechanisms are compromised and cytosolic Ca++ increases (Yang and Steele, 2000). If randomly moving mitochondria stop where Ca++ is elevated, they will be recruited to regions of insufficient ATP and retained there until ATP levels are restored. This mechanism may therefore assist in balancing the distribution of mitochondria throughout the cell. Failure of this mechanism may account for the increased excitotoxicity of NMDA to MiroKK-expressing neurons.
An unanticipated finding in the present study was that the EF hands of Miro mediate Ca++-dependent arrest of retrograde motion as well as anterograde (Figures (Figures3,3, ,4).4). Retrograde motion of axonal mitochondria is dependent on dynein rather than kinesin (Hollenbeck and Saxton, 2005; Pilling et al., 2006). This raises the likelihood that Miro has interactions with the dynein complex in addition to its known interactions with kinesin. At present, little is known about how kinesin and dynein motors interact and whether, or how, they are coordinated (Gross et al., 2007). Estimates of the motor molecules per mitochondrion vary from 2 to 200 (Gross et al., 2007), and it is unknown whether these motors are activated and inactivated in concert. With fluorescent tags on both KHC and mitochondria we have shown that KHC remains associated with mitochondria even when they are moving in the retrograde direction (Figure 4). These kinesin molecules must either be switched off or actively oppose the retrograde movement (Gross et al., 2007). The possibility of a shared association with Miro, therefore, may provide an entry to understanding how opposing motors may be coordinately regulated.
The regulation of mitochondrial dynamics is likely to be extremely intricate, extending well beyond the Ca++-dependent effects on kinesin activity described here. The atypical GTPase-domains in Miro (Fransson et al., 2003; Fransson et al., 2006) and splicing variants of milton (Cox and Spradling, 2006; Glater et al., 2006; Smith et al., 2006) represent additional likely control points. The potential interplay of the GTPase motifs and EF-hands is not presently understood, but may resemble the influence of Ca++ on Rho-GTPase in controlling actin dynamics (Aspenstrom et al., 2004; Bader et al., 2004). The splice variants of milton differ in their association with KHC (Glater et al., 2006) and may have tissue specific roles (Cox and Spradling, 2006). In addition, the motility of mitochondria is likely to be interrelated with the fission-fusion machinery, as the dynamin-like GTPase, Drp1, influences mitochondrial density in dendrites (Li et al., 2004), and the absence of fission prevents axonal transport of mitochondria (Verstreken et al., 2005). The Miro homolog of yeast, GEM1p, controls mitochondrial distribution in that organism in a kinesin-independent manner (Frederick et al., 2004) and these additional functions of Miro may be present in higher eukaryotic cells as well (Fransson et al., 2006; Guo et al., 2005). One of the most intriguing potential regulations may be mediated by the enzyme O-GlcNAc transferase (OGT). OGT has been shown to bind to milton and glycosylate it in both mammals (Iyer and Hart, 2003) and Drosophila (Glater et al., 2006). Elsewhere, OGT activity has been shown to reflect glucose concentrations and the metabolic state of the cell (Murrey and Hsieh-Wilson, 2008), opening the possibility that the interactions of milton and OGT may permit mitochondrial distribution to be tailored by the availability of substrates for glycolysis and ATP production. Thus the motor/adaptor complex discussed here may be the nexus of multiple control pathways in addition to the Ca++-sensing role of Miro and is likely to transduce information about local energy supply and demand. These converging signaling pathways will likely regulate mitochondrial dynamics to achieve the most efficient supply and use of energy by the cell.
The following constructs were used: pLPS-RFP-mito (Colwill et al., 2006), (No. 11702, Addgene, Cambridge, MA); human Miro, pRK5Myc-Miro1 and pRK5Myc-Miro1E208K,E328K (MiroKK), (Fransson et al., 2006); Drosophila milton, pCMV-milton A (Stowers et al., 2002); rat KHC, KHC-Myc, KHC1-682-Myc, (Verhey et al., 1998),KHC-ECFP and KHC-mCit (Cai et al., 2007); pCMV-GFP (gift of Dr. Z. Wills); Synaptophysin-YFP, PSD95-YFP (Chang et al., 2006); human KIF5C1-335-EYFP (Smith et al., 2006); and Drosophila Miro, pA1T7-DMiroΔTM (Glater et al., 2006). pA1T7-DMiroE234K,E354K,ΔTM(DMiroKKΔTM) was QuickChange (Stratagene, La Jolla, CA) to introduce into Drosophila Miro the mutations equivalent to E208K and E328K in human Miro.
Cell Culture
Rat hippocampal cells were dissected and dissociated from day 18 embryos, cultured for 8-11 days, transfected with Lipofectamine 2000 (Invitrogen), and imaged 2-4 days later. COS and HEK293T cells were transfected with calcium phosphate. Even when four constructs were simultaneously transfected into neurons or HEK cells, the extent of coexpression was greater than 95%, as determined by retrospective immunostaining (Supplementary Data and Figure S5).
Immunostaining and Confocal Microscopy
Immunocytochemistry was performed as previously described (Glater et al., 2006; Stowers et al., 2002) with mouse anti-Myc (9E10, Santa Cruz Biotechnology, Inc., Santa Cruz, CA) at 1:300 and Cy5-conjugated anti-mouse IgG (Jackson ImmunoResearch Laboratories, West Grove, PA) at 1:500. MitoTracker Orange (Invitrogen) was applied at 100 nM for 10 min. Cells were imaged at room temperature (20°C) with a 63×/NA1.4 oil Plan-Apochromat objective on a laser scanning confocal microscope (LSM 510 META/NLO; Carl Zeiss MicroImaging, Inc., Thornwood, NY) with LSM software 3.2 (Carl Zeiss MicroImaging, Inc.). Images were processed with Photoshop 10.0 (Adobe, San Jose, CA) using only linear adjustments of contrast and color, and Illustrator 13.0 (Adobe).
Live Image Acquisition and Quantification
Confocal images (see Supplemental Data) were captured every 5-10 seconds before and after calcimycin treatments. 60-150 μm of axon at least 250 μm away from the cell body was selected for analysis. For glutamate stimulation, 30-110 μm of dendrite was selected for analysis. Kymographs were generated (Metamorph software, MDC, CA), that represented an interval of 100 s taken before the application of calcimycin or glutamate and 5 min after calcimycin or 1 min after glutamate addition. Each kymograph was then imported into a macro written in Labview (NI, TX), and individual RFP-mito or SYP-YFP puncta were traced using a mouse-driven cursor at the center of the RFP-mito or SYP-YFP object. By using Matlab (The MathWorks, MA), we determined the following parameters: 1) the instantaneous velocity of each mitochondrion, 2) the average velocity of those mitochondria that were in motion, 3) the percent of time each mitochondrion was in motion, 4) stop frequency, and 5) turn back frequency. The lengths of mitochondria were also measured 100 s before and after the 5-min calcimycin exposure. A threshold velocity was defined as 0.05μm/s which was equivalent to a displacement of 1 pixel over a time lapse of 1 pixel and exceeded the bias caused by recording drift and mouse-positioning (see Supplemental Data). Velocities less than 0.05μm/s were considered zero.
Coimmunoprecipitation and Microtubule Cosedimentation
HEK cells were lysed in buffer as in Glater et al., 2006, but with EDTA replaced by 5mM EGTA and 0 Ca++, or by 2 mM Ca++, or by a series of low Ca++ conditions (Figure 6K,L) for which the free Ca++ concentration had been calculated (Maxchelator; Coimmunoprecipitations were performed as described in Glater et al., 2006. Lysates were incubated with rabbit anti-GFP (Invitrogen), mouse anti-Myc (9E10, Santa Cruz Biotechnology, Inc.), or rabbit anti-hMiro1 (Fransson et al., 2003), and protein A-Sepharose beads (GE Healthcare, Piscataway, NJ) for 2-3 hours at 4°C. Immunoprecipitates were analyzed by SDS-PAGE and immunoblotted as indicated (See Supplemental Data)
For cosedimentation experiments, polymerized microtubules were prepared by incubating tubulin (Cytoskeleton Inc., CO) with 1mM GTP and 100 μM Taxol (Sigma, MO) at 37 °C 1 hour. Cell lysates were then incubated with 20 mM Taxol and 0.1 mg/ml polymerized microtubules for 30 minutes at room temperature without ATP. The microtubule pellet and bound proteins were collected by centrifugation at 21,000g for 30 minutes through a 10% sucrose cushion. Soluble proteins in the supernatant were TCA precipitated and both supernatant and microtubules pellet were analyzed by SDS-PAGE and immunoblotted as indicated (see Supplemental Data).
For quantitative immunoprobing, blots were probed with anti-GFP (Invitrogen) and Cy5 goat anti-rabbit (GE Healthcare) at 1:5000 and scanned by Typhoon Trio Imaging Scanner (Amersham BioSciences, Piscataway, NJ). Fluorescent intensity of the bands was quantitated by fluorescence detection in the linear range. The intensity of each KIF5C(1-335)-YFP band was normalized to an unrelated control IgG band on the same blot.
Preparation of Mitochondrial Fractions
Mitochondria were prepared from cultured rat hippocampal neurons by differential centrifugation (see Supplemental Data). The mitochondrial pellet was resuspended in either 0 or 2 mM Ca++ isolation buffer, and centrifuged again. The supernatant (wash) and the mitochondrial pellet were collected separately. 3.5% of the non-mitochondrial fraction, 10% of mitochondrial fraction, and 10% of wash were then loaded in SDS-PAGE and analyzed by Western Blotting with mouse anti-KHC (H2) at 1:400, rabbit anti-VDAC at 1:1000 (Bioreagents, Golden, CO), and mouse anti-synaptophysin at 1:200 (gift of Dr. F. Sun).
Statistical Analysis
Throughout the paper, the distribution of data points is expressed as mean ± standard error of the mean. The Mann-Whitney U tests were used for statistical analysis unless otherwise indicated.
Supplementary Material
We thank I. Rappley, Drs. F. Sun, Z. Wills, P. Aspenström, K. J. Verhey, A. M. Craig, T. Pawson, G. W. Hart, and F. A. Stephenson for reagents; S. Vasquez, Drs. Z. Wills, M. Greenberg, and Z. He for assistance with hippocampal cultures, Dr. L. Bu and the Developmental Disorders Research Center Imaging Core and E. Pogoda for technical assistance; Dr. Y. Chu for assistance with Matlab script and a Labview macro. This work was supported by NIH RO1GM069808.
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