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International Journal of Alzheimer's Disease
Volume 2012 (2012), Article ID 172837, 16 pages
Accumulation of Vesicle-Associated Human Tau in Distal Dendrites Drives Degeneration and Tau Secretion in an In Situ Cellular Tauopathy Model
Department of Biological Sciences, Center for Cellular Neuroscience and Neurodegeneration Research, University of Massachusetts Lowell, Lowell, MA 01854, USA
Received 15 June 2011; Accepted 15 September 2011
Academic Editor: Vincenzo Solfrizzi
Copyright © 2012 Sangmook Lee et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
We used a nontransgenic cellular tauopathy model in which individual giant neurons in the lamprey CNS (ABCs) overexpress human tau isoforms cell autonomously to characterize the still poorly understood consequences of disease-associated tau processing in situ. In this model, tau colocalizes with endogenous microtubules and is nontoxic when expressed at low levels, but is misprocessed by a toxicity-associated alternative pathway when expressed above levels that saturate dendritic microtubules, causing abnormally phosphorylated, vesicle-associated tau to accumulate in ABC distal dendrites. This causes localized microtubule loss and eventually dendritic degeneration, which is preceded by tau secretion to the extracellular space. This sequence is reiterated at successively more proximal dendritic locations over time, suggesting that tau-induced dendritic degeneration is driven by distal dendritic accumulation of hyperphosphorylated, vesicle-associated tau perpetuated by localized microtubule loss. The implications for the diagnosis and treatment of human disease are discussed.
Alterations of the microtubule-associated protein (MAP) tau that affect tau:tau and tau:tubulin interactions are a key factor in the cytopathogenesis of neurodegenerative syndromes involving tau (tauopathies) [1–3] reviewed in [4, 5]. Phosphorylation at proline-directed sites flanking the microtubule binding repeat (MTBR) domain is inhibitory to MT binding, and ultimately causes the formation of tau aggregates  and progressive loss of MTs and neurodegeneration in tauopathy models [7–12]. The extent to which this occurs is likely a key determinant of whether tau is playing a normal or pathological role [4, 13]. Exonic tau mutations responsible for familial tauopathies cause hyperphosphorylation, a reduction in MT binding, and an increased tendency to aggregate [14–17], suggesting that a causal link exists between these features and toxicity. Although mutant tau isoforms are more toxic than wild-type (WT) isoforms when expressed in situ , the patterns of degeneration produced by WT and mutant tau species are very similar, even in disease models using identified neurons , suggesting that the cytoplasmic accumulation of hyperphosphorylated, non-MT-bound tau is a common feature that drives toxicity.
Since the tau MTBR forms the core of the neurofibrillary aggregates characteristic of tauopathies and is the site of most exonic mutations that drive familial tauopathies [6, 19, 20], the modulation of tau:MT and tau:tau interactions via tau phosphorylation [1, 3, 13, 21] or cleavage [22–25] to form toxic oligomers or aggregates  has become the central research focus in studies of tau-induced toxicity and tauopathy cytopathogenesis. However, very little is known about how tau aggregates are produced and distributed in the somata and dendrites of neurons in situ, making it difficult to establish the sequence and causality of cellular events that lead to neurodegeneration. The role of aggregation is further obscured by findings that cleavage fragments of the amino terminal “projection” domain of tau [27–30] can also mediate tau toxicity via a separate pathway [30, 31]. This pathway involves caspase  and calpain  activation and can mediate toxicity caused by extracellular agents, such as beta amyloid · We now know that tau misprocessing also involves the interaction of tau with lipid raft-associated proteins at the plasma membrane via the tau N-terminal domain [35, 36], which becomes phosphorylated at tyrosine 18 (Y18) . Abnormal tau-actin interactions  and the misrouting of tau to the Golgi  in tauopathy suggest that an abnormal association with the plasma membrane and/or “trafficking” vesicles derived from it may also play a role in tau-mediated toxicity. Recent findings that tau is secreted to [40, 41] and taken up from  the extracellular space and that it can be transported transneuronally in situ [40, 43] make it necessary to distinguish cell autonomous from interneuronal effects of tau misprocessing. In this study, we used the unique advantages of the lamprey ABC tauopathy model, in which tau is expressed cell autonomously in identified neurons (ABCs), to characterize tau misprocessing at the cellular level in neurodegeneration in situ.
We use confocal microscopy and the high spatiotemporal resolution offered by the ABC tauopathy model to make a detailed correlation between the expression level, intracellular distribution, phosphorylation state, and secretion of human tau isoforms relative to the distribution and stability of MTs. We previously used this model to show that tau phosphorylated at Y18 (9G3+ tau) becomes associated with vesicle-like particles and accumulates in ABC dendritic tips [18, 41], where it causes distension and ultimately degeneration [8, 9, 18, 41]. In this study, we address the role(s) played by (a) tau-MT binding (and the phosphorylation of sites known to affect tau:MT binding) and (b) the effects of tau expression level and somatodendritic distribution in producing the toxic effects caused by tau expression on the neuronal cytoskeleton in situ. We show that exogenous tau expression above the level needed to saturate dendritic MTs results in the redistribution of specific phosphotau species (9G3/12E8 tau) distally to dendritic tips, dendritic MT loss in the vicinity of tau accumulation, and tau secretion from tau accumulation sites with ongoing or recent MT loss. In addition, we characterized the morphology of exocytosing vesicles involved in tau secretion and identified proteins that colocalize with tau as it is secreted. We propose that non-MT-associated tau accumulation activates an alternative tau processing pathway involving abnormal endosome formation, centrifugal dendritic transport, and secretion of vesicle-associated tau and suggest that this may play a key role in the cellular and intercellular pathogenesis of human tauopathies.
2.1. Tau Expression
We used the pEn123c and pEn1234c plasmids encoding green fluorescent protein-(GFP-) tagged wild-type human tau 3R0N and 4R0N isoforms (resp.) for most of these experiments. We also used P301L tauopathy mutant of 4R0N and a double pseudophosphorylation mutant at S262D and S356D in the MTBR of 3R0N that were derived from the corresponding parent WT plasmids [18, 41]. Plasmids encoding lamprey neurofilament (NF180)  or GFP  served as expression controls. All plasmids used the CMV promoter to drive exogenous protein expression. Microinjection of plasmids was performed as described , using 1 mg/mL of plasmid mixed in microtubule stabilizing buffer.
Immunohistochemical analysis of transverse sections through ABC somata, dendrites, and axons (Figure 1) was performed using standard enzyme-linked and immunofluorescence protocols [8, 18, 41, 47, 48]. After 10 days following plasmid injection, brains were reexposed under fluorescence to identify ABCs expressing GFP-tagged exogenous proteins and then fixed with FAA (10% formalin, 10% glacial acetic acid, and 80% ethanol), dehydrated, embedded in paraffin, and sectioned at 10 μm. Rabbit polyclonal anti-GFP (1 : 200, Invitrogen) were used to detect the expression of GFP-tagged tau or NF-180. HRP-linked staining with diaminobenzidine (Sigma) was used on every 7th section to reveal immunopositive ABCs, with the remaining sections used for immunofluorescence. Sections were deparaffinized, rehydrated, quenched with H2O2, boiled for 10 min in pH 9 and 10 mM Tris-EDTA buffer to unmask antigen, and incubated in primary antibody overnight at 4°C. For immunofluorescence staining, sections were quenched 10 minutes in 1% sodium borohydride/TBS.
We used the following primary antibodies: PHF1 (1 : 200), Tau1 (1 : 400), Tau5 (1 : 400), Tau7 (1 : 400), Tau12 (1 : 400), Tau46 (1 : 100, Sigma), 9G3 (1 : 30), AT180 (1 : 200, Pierce), DM1A (1 : 500, Sigma), TUB1 (1 : 500, Sigma), and 611B (1 : 500, Sigma). Tau1, Tau5, Tau7, and Tau12 antibodies were kindly provided by Dr. Lester Binder (Department of Cell and Molecular Biology, Northwestern University Medical School, Chicago, IL, USA). PHF1 was a generous gift from Dr. Peter Davies (Department of Pathology, Albert Einstein of College of Medicine, Bronx, NY, USA). 9G3 was provided by Dr. Gloria Lee (University of Iowa, Iowa City, IA). Polyclonal Abs against human fyn (1 : 50, Santa Cruz), LC3 (1 : 30, Abgent), and COX1 (1 : 200, MitoScience) were used to label the highly conserved eponymous lamprey homologues of fyn (92% identity), LC3 (73% identity), and COX1 (64% identity).
2.4. Data Analysis
Immunofluorescence intensity was measured in multiply immunolabeled sections containing somatodendritic profiles of tau-expressing ABCs. Confocal images were analyzed using either ImageJ or Volocity (ImproVision) to generate image stacks. In some cases, densitometric analysis of nonconfocal images of DAB-revealed adjacent sections from the same brain was performed. For quantitative assessment of exogenous tau immunolabel intensity or for comparisons between different phosphotau epitopes, the immunolabel density at the point of dendritic degeneration (POD) was normalized to 100%, with localization along dendrites defined in terms of distances from the POD (distal = plus). For the calculation of tau:tubulin intensity ratios and for comparing “absolute” levels of tau expression (e.g., to assign ABCs to “low” and “high” tau expression categories), we compared tau (GFP tag) versus tubulin (DM1A) immunolabel intensities in confocal stacks of multiply immunostained sections, which were scored relative to DM1A neuropil immunolabel in that location of the section using the same PMT settings. Intensity of tubulin (DMIA, TUB1, 611b) immunolabel was scored relative to the neuropil surrounding ABC axonal, dendritic, and somatic profiles. The cellular elements of “neuropil” consist mainly of small axon cross/longitudinal profiles that stain relatively uniformly for the probes shown in Figure 2 and are unaffected by exogenous protein expression in ABCs. All comparisons of immunolabel intensity were done using a two-sample t-test or one-way ANOVA as appropriate; such data are expressed as mean ± SEM, and significance was expressed at values as noted. Quantitative analyses that required the categorization of data sets according to defined criteria, such as “high” versus “low” tau expression (as defined in the Results section), were analyzed using the chi-square test. Ratios of phosphotau to total tau was calculated using the “sync windows” and “sync measure” 3D plug ins of ImageJ. Quantitative comparisons of axonal versus dendritic tau immunolabel intensity were made using the “Measure RGB” plugin. This was only done in “low” tau expressing ABCs and was restricted to sections where both axonal and dendritic profiles were unambiguously present. Unbiased comparison of tau label intensity between axon profiles (which invariably extended through the entire section) with dendritic profiles which occupied varying proportions of the axis was accomplished by normalizing tau to tubulin levels in each sample. Quantitation of DAB product for tubulin versus tau immunolabel ratios in the axons of tau-expressing ABCs and adjacent axonal profiles of similar size was performed on 10 sets of 4 adjacent sections in the obex. Ratios between tau versus tubulin immunostaining intensity were performed by comparing the intensity of label between the red and green color channels on a per voxel basis using the ratio channel function of Volocity 4.3.
2.5. Colocalization Analyses
Semiquantitative comparisons of the degree of colocalization to MTs between (a) dendritic GFP-tau label in low- and high-expressing ABCs (Figure 4) and (b) markers of high- (tau1, tau5) and low- (9G3) MT-affinity tau species (Figures 6 and 7) was performed on stacks using ImageJ “colocalization highlighter” at a common threshold value. Images in which only the colocalized voxels are shown (such as was done with the phalloidin label in some of the images in Figure 7) were obtained by substituting the “colocalized points” 8-bit file generated by colocalization highlighter for the original channel in the final image, which was produced using the ImageJ plugin “3D Viewer”.
3.1. ABC Cytoskeleton
The composition of the somatodendritic and axonal cytoskeleton in lamprey ABCs is typical of large projection neurons in vertebrate central nervous systems [8, 47, 48]. Somatodendritic MTs consist of both stably polymerized and dynamic tubulin in ABCs, especially in large proximal dendrites (5+ microns diameter). Total and tyrosinated (i.e., recently polymerized) alpha-tubulin levels are highest in such dendrites and both are clearly above neuropil levels in all but the smallest dendrites. Levels of acetylated (stably polymerized) tubulin are comparatively lower, with the largest dendrites staining near neuropil levels and the smaller ABC dendrites staining below. Tubulin immunolabel intensity in ABC axons is generally similar to those seen in the soma and typically were not as strong as those of dendritic tubulin. NF immunolabel intensity (LCM3 ) is above neuropil levels in large proximal dendrites, declining distally to below neuropil in the smallest dendrites (Figure 2). NF staining was stronger in axons than in somata and dendrites [43, 44], and axonal NF label was stronger than that of tubulin. This is to be expected given that NF to MT frequency in large axons such as those of ABCs is as high as 20 : 1, and up to 3x higher than that of small axon profiles [46, 49, 50]. Cross reaction of mAbs T46 and Tau7 (not shown) to the relatively well-conserved tau C terminus  identified an axonally targeted endogenous lamprey MAP (lamprey tau). Lamprey tau is concentrated in small axons, is relatively low in ABC axons, and is virtually absent from ABC somata and dendrites (Figure 2) and so was not considered to be a significant factor in the distribution and MT-binding of exogenous tau species (see below).
3.2. Expression of Exogenous Proteins in ABCs
Previous comparisons of the effects of expressing human tau via plasmid microinjection [8, 9, 45, 52] versus a control proteins (lamprey neurofilament NF180) showed that toxicity due to overexpression is tau specific. Here we used NF180 and GFP to control for nonspecific overexpression effects on MT integrity and other cytoskeletal changes, especially in the proximal dendrites and axon. Expression of GFP alone resulted in a relatively even distribution of anti-GFP immunolabel, while the distribution of exogenous NF180 resembled that of endogenous NF180 (Figure 3).
3.3. Distribution of Exogenous Tau between the Axon and Dendrites Is Modulated by Tau Expression Levels in ABCs
We used the distribution of total exogenous human tau (GFP tag) relative to that of endogenous tubulin (DM1A) immunolabel in proximal dendrites to sort ABCs into “low-expressing” and “high-expressing” groups (Figures 3 and 5). In “low-tau” ABCs, the axon and proximal dendrites exhibited the strongest staining in a pattern that was similar to that of tubulin (Figure 3). This distribution is consistent with the known function of tau as a MAP and is the expected pattern if tau is primarily binding directly to MTs. There was a slight preferential distribution of tau to the proximal axon relative to proximal dendrites (Figure 3(b)), but this was only seen at low expression levels in comparisons between raw GFP-tau levels in WT T24-expressing ABCs versus GFP alone. The difference between WT and P301L tau distribution disappeared when axon:dendrite tau ratios were normalized to tubulin levels to account for differences in -axis profile dimensions between axons and dendrites. Preferential axonal staining did not appear to involve the ability to bind MTs directly, since it was still present with the S262/356D mutant . By contrast, with “high” tau expression, tau tended to accumulate in perimembranous regions of the soma and in distal dendrites (Figures 3(c) and 4). Moreover, tau in high-expressing ABCs was preferentially localized to dendritic tips and was thus much more distally located than dendritic tubulin staining. The most striking difference between the “low” and “high” distributions of tau was that in the latter case the areas of highest tau accumulation were devoid of MTs, whereas tau and tubulin were colocalized with “low” tau expression (Figure 3(c)).
3.4. High Tau Expression Causes Redistribution of Somatodendritic NFs and f-Actin in ABCs
In low tau-expressing ABCs, exogenous tau was distinct from that of endogenous NF-180 and filamentous actin (f-actin) in all parts of the soma and dendrites, with tau being colocalized with MTs (Figures 4(a) and 4(b)). High levels of tau expression did not affect this pattern in the proximal dendrites of high-expressing ABCs; we found that colocalization of NF protein and f-actin with tau did occur in the distal dendrites of some high tau-expressing cells. This was most noticeable at the sites with the largest accumulations of non-MT-associated tau, which were typically in the vicinity of the POD or the dendritic tips, depending on the extent of dendritic degeneration. In the case of endogenous NFs, tau-associated NF180 protein was displaced distad of its typical location; this is readily apparent as there are relatively few NFs in the dendrites of non-tau expressing lamprey neurons [46, 48].
3.5. Tau Distribution and Toxicity in ABCs Is Modulated by the Saturation of Tau Binding Sites on Endogenous MTs
Low tau expression is defined as being below or at the level of tau:MT “saturation” (tubulin is 100% colocalized with tau, and tau is at least 80% colocalized with tubulin) with all tau being colocalized with tubulin in ABC proximal dendrites (Figure 5). High expression is defined as tau expression above the level needed to saturate MTs in ABC proximal dendrites. Low-expressing ABCs nearly always (Figure 5(c)) show low-stage (1 or 1.5) tau-induced degeneration. This definition is consistent with the staging scheme of tau-induced degeneration described in an earlier study  in which stage 1 was defined by the filling of dendritic profiles with even tau label, and higher levels of tau expression (stages 2-3) were characterized by the distal to proximal extent of dendritic degeneration. ABCs staged as “high expressing” (i.e., stage 2 and above) by this method were almost perfectly cosegregated with those scored as having proximal dendrites “above saturation” (Figure 5(c)).
3.6. Tau Redistribution with High Expression Is Correlated with Microtubule Loss and Dendritic Degeneration
The most dramatic effect of high tau expression was to induce tau accumulation in distal dendritic tips (Figures 3(c) and 5) [8, 9, 18]. This was accompanied by the loss of tubulin label that was most evident with tyrosinated tubulin in distal dendrites (Figures 5(e) and 6). By contrast, the level of tau expression had little effect on axonal tubulin levels (Figure 5(e)). The distal dendritic tau accumulations seen with high tau expression were always associated with dendritic degeneration (Figure 3(c)), which was confirmed when tau:tubulin ratios were calculated for GFP/DM1A immunolabeled sections using the ratio channel facility in Volocity (Figure 6(a)) and when ratio measurements were taken manually (Figure 6(b)). We found that the majority of sites at the POD (59%) showed tau:tubulin ratios of 8 : 1 or higher, with 24% at 12 : 1 or higher, whereas 82% of sites sampled 20–50 microns away from the POD showed ratios of under 7 : 1. Moreover, 90% of the sites with the highest tubulin intensity readings (i.e., with readings above neuropil immunostaining levels in the distal dendrites) were beyond 25 microns from the POD and had tau:tubulin ratios of 7 : 1 or below, while all of the sites with the highest tau readings were located at or distal to the POD (Figure 6). This was in close agreement with the Volocity ratio results and strongly indicates that some mechanistic connection exists between tau accumulation in the distal dendrites and localized MT loss and degeneration there.
3.7. Distally Transported Tau Is Disproportionately Phosphorylated at the 9G3 and 12E8 Sites
We found that tau phosphorylation state in distal dendritic accumulations is inversely correlated with respect to tubulin immunostaining levels and thus presumably not MT-associated (Figure 8). The tau in such accumulations is enriched in phosphotau species that are either incapable of binding (12E8+ tau [53–55]) or are not currently bound to MTs (9G3—see Figure 7). By contrast, markers identifying poorly phosphorylated tau with high MT affinity (Tau1, Tau5, Tau12) was localized to MT-rich regions (i.e., large dendrites), with mAbs marking proline-directed phosphorylation that reduces but do not abolish tau:MT binding (AT180, PHF-1 and AT8) showing an intermediate pattern (Figure 8). High-MT-affinity tau was largely colocalized with MTs in ABC dendrites and accumulated minimally at the POD, while 9G3+ tau or tau phosphorylated at KXGS sites in the MTBRs (12E8+ tau) was localized to either the POD itself or to a ventrolateral somatic location near the bases of large dendrites. Proline-directed phosphoepitopes (i.e., AT8, AT180, PHF1) were also more concentrated at the POD than was total (GFP+) tau (Figure 5(c)), but this tendency was less pronounced than with 9G3 and 12E8 (Figure 8).
3.8. Tau Phosphorylated at the 9G3 and 12E8 Sites Is Associated with Fyn- and LC3-Containing Vesicles near Secretion Sites in ABC Dendrites
In earlier studies, we showed that distal dendrites of high-expressing ABCs become strongly tau positive  and filled with vesicular inclusions [8, 18]. Some of the tau accumulated at dendritic tips or the POD becomes transiently immunopositive for 9G3 (marking tau phosphorylation at Y18 by srk-family tyrosine kinases) and may undergo secretion to the extracellular space . In this study, we characterized these inclusions in more detail by immunolabeling sections through tau-secreting ABCs with multiple anti-tau antibodies (Figures 7 and 8) together with Abs to specific vesicular markers, as well as the fluorescently labeled f-actin marker phalloidin. We found that tau-positive vesicular profiles at the surfaces of intact dendrites near the POD in ABCs expressing high levels of tau were colocalized with either non-MT-associated tau epitopes (9G3, 12E8) and/or markers of vesicular organelles (Figures 9 and 10). At sites where secretion was ongoing, many but not all 9G3 tau+ vesicles were colocalized with the srk family tyrosine kinase fyn, which can be considered a dendritic endosome marker [56, 57], with 12E8-positive tau being similarly distributed (not shown). When compared to markers of high-MT-affinity tau (Tau5, Tau12), the GFP tag fused to the tau amino terminus also selectively identified exocytotic profiles at sites of focal secretion (Figure 10).
The misprocessing of tau is a key event in neurodegenerative tauopathies and is typically not associated with MTs. However, the details of the toxicity-associated tau misprocessing pathway in the absence of MT binding are still very poorly understood. We employed overexpression as a means of generating non-MT-associated tau in ABCs in order to characterize this pathway and its relationship to tau-induced degeneration in a high-resolution cellular model in situ. We show that the expression of exogenous tau causes a dose-dependent loss of somatodendritic MTs that is spatiotemporally correlated with tau-induced degeneration. We confirm earlier findings in the lamprey system and elsewhere that tau colocalizes with certain vesicular organelles, especially when phosphorylated at Y18 [18, 36]. Our results indicate that the saturation of dendritic MTs by exogenous human tau accounts for the changes in tau distribution and phosphorylation seen between ABCs expressing low and high levels of tau. Tau expression above this threshold is correlated with degeneration patterns that account for all of the characteristics of tau-induced toxicity observed in this model (and others to our knowledge) so far. We also conducted the first detailed morphological characterization of tau secretion from CNS neurons in an in situ tauopathy model and present evidence that tau secretion occurs via an unconventional mechanism with characteristics of microvesicle and exosome-mediated routes. These events are summarized in Figures 9 and 10, and their relevance to and implications for tau pathobiology in human disease are discussed below.
4.1. Distribution of Exogenous Tau in ABCs
The overexpression of both WT and tauopathy mutant tau in ABCs in most cases produces phosphorylated tau accumulation in dendrites, as reported previously [8, 9, 18, 41]. While there did appear to be some preferential distribution of exogenous tau to the axon at relatively low levels of overexpression in ABCs, this effect was slight and was apparently not related to the preferential association of tau with axonal versus dendritic MTs. Moreover, even this slight preference was lost with relatively moderate levels of overexpression, a pattern similar to that seen with early murine transgenic models [58, 59]. This is consistent with reports that active targeting of tau to the axon occurs mainly at the mRNA rather than the protein level [60, 61] and with reports that tau may be slightly overexpressed in non-AD human tauopathies . We, therefore, propose that tau overexpression in ABCs re-creates the circumstances needed for tau toxicity (e.g., tau hyperphosphorylation, tau cleavage) simply by exceeding the tau-binding capacity of endogenous dendritic MTs. The relative insensitivity of axonal MTs to the destabilizing effect of tau overexpression suggests that the primary effect is a gain of a toxic function in the dendrites rather than the loss of normal MT stabilization axon in the axon.
4.2. MT Saturation and the Centrifugal Redistribution of Non-MT-Associated Tau
In the ABC model, the occurrence of tau-induced dendritic MT loss, vesicular tau, and tau secretion at the POD appear to be mechanistically related given that the POD is also the site of both the highest focal tau secretion levels and of the sharpest decrease in dendritic tubulin levels (Figure 5(b)). Our findings are also consistent with studies showing tau redistribution to MT-poor regions of the cell whenever it is present in excess of available MT tau binding capacity, whether this occurs by overexpression or by some disease-related mechanism that limits tau:MT binding . The limited tau binding capacity of dendritic MTs for tau in ABCs thus appears to serve as a threshold above which excess tau is processed by an alternative, toxicity-generating pathway. Moreover, since tau has been shown to modulate the activity of MT-associated motor proteins that mediate dendritic transport [64, 65], often in a disease-specific  or overexpression-induced  manner, it seems likely that toxicity resulting from tau accumulation at localized dendritic loci may have relevance to the pathogenesis of human tauopathies, which typically feature abnormal somatodendritic phosphotau accumulation.
4.3. A Significant Proportion of Non-MT-Bound Tau Is Vesicle Associated and Is Associated with Tau Toxicity
Hyperphosphorylated, non-MT-associated tau is widely considered to be the agent of neurodegeneration in human tauopathies, although little is known about its underlying toxicity mechanism. Here we confirm other demonstrations in the ABC model that a tight correlation exists between 9G3 phosphorylation and localized tau-induced neurodegeneration  (Figures 7 and 9), and that tau overexpression is associated with vesicle accumulation in ABC distal dendrites [8, 18]. Our observations show that the phosphorylated tau accumulating where dendritic MTs are being lost in ABC dendrites is largely vesicle associated and that some of these vesicles resemble endosomes and/or autophagosomes in their general appearance and colocalization with endosome (fyn) and autophagosome (LC3) markers (Figure 10). Moreover, this toxic, vesicle-associated tau accumulates selectively in MT-poor regions that are adjacent to more proximal dendritic segments containing organized MT bundles (Figure 9), suggesting (1) that it is translocated via MT-mediated transport in ABC dendrites and (2) that its accumulation is both the cause and the consequence of localized MT destabilization. We propose that abnormal tau involvement in the formation of trafficking vesicles originating from the plasma membrane and/or the autophagy pathway in the absence of MT association cause the accumulation of 9G3/12E8, positive tau, which in turn destabilizes nearby MTs via an as yet unknown mechanism. This could account for the selective MT loss associated with neurofibrillary pathology in humans [1, 2, 68, 69] and suggests that hyperphosphorylated, non-MT-associated tau may be bound to vesicles that are transported within the cell via MT-mediated mechanisms in human tauopathies. This idea has been little explored but is consistent with much of the relevant human tauopathy literature and could add a new dimension to our conception of abnormal tau processing in neurodegenerative disease. Neuropathological studies suggest that hyperphosphorylated tau may oligomerize into granular and ultimately fibrillar deposits and that an unknown element in this sequence of events mediates tau toxicity [3, 68, 69]. This is supported by demonstrations that “pretangle” deposits of granular, hyperphosphorylated tau precede NFT formation in murine models [70, 71] and appear to do so in humans [68, 69]. However, interactions between tau and membrane/vesicle-associated proteins are also associated with and may mediate aspects of neurofibrillary disease. Tau oligomerization can be driven by fatty acids in vitro [72, 73], while NFT formation is associated with membranous organelles in vivo [74, 75]. Misprocessed tau has been associated with abnormalities in several types of vesicular organelle in AD and tauopathy models, including the Golgi apparatus , lysosomes [76–78], autophagosomes [76, 79–81], and most recently exosomes . The last two are of particular interest in light of our findings here that vesicular tau is colocalized with the lipid raft-associated tyrosine kinase fyn, which itself is both required for extracellular beta-amyloid-mediated toxicity via tau [83, 84] and is mislocalized in AD [85, 86]. Since fyn has been identified in exosomes (along with other signal transduction associated kinases) , it appears that interaction with and phosphorylation of tau at the 9G3 site by fyn may be a key feature of both secretion and toxicity-associated tau processing. Fyn activation during signal transduction typically causes the oligomerization and endocytosis of downstream elements  and targets at least some oligomerized targets of fyn phosphorylation to exosomes [89, 90], a process which appears to be highly analogous to what we see with tau in the ABC system. Similarly, the involvement of the (macro)autophagy pathway of protein turnover in AD has long been known [79–81, 91], and this has more recently been extended to non-AD tauopathies [77–79], where it now appears to play a largely disruptive role in autophagic protein turnover mechanisms that may well exacerbate tau toxicity in these diseases . The association of non-MT-associated tau with fyn or LC3-positive is consistent with microvesicular or exosomal secretion, as discussed below.
4.4. Possible Mechanisms of Dendritic Tau Secretion
In a previous study, we found that tau secretion from ABC dendrites requires elements in both the tau N-terminal and MTBR domains and inferred that such secretion is transient, first appearing before the onset of overt degeneration and ending before complete fragmentation of the dendrite occurs . While these results showed tau secretion to be an active biological process rather than a passive release of tau from autolyzing neurons, they gave little indication as to the mechanism of tau secretion and why it is spatiotemporally correlated with dendritic degeneration in ABCs. The present study yields specific indications as to the secretion mechanism by (a) correlating MT loss and the distribution of non-MT-associated tau with “focal” secretion from ABC dendrites just before the onset of dendritic degeneration and by characterizing the (b) morphology of exocytotic profiles and (c) the phosphorylation state and proteins colocalized with the secreted tau. In particular, we show that at least some tau secretion is associated with fyn-positive, endosome-like vesicles in which tau has been phosphorylated at the site (Y18) characteristically phosphorylated by fyn, and that another subset of tau-containing vesicles is colocalized with the autophagy marker LC3, which also appears to be exocytosed. It is noteworthy that, in normal autophagy, LC3 is rarely seen among the exocytosed proteins due to its exposure to lysosomal hydrolases . However, tau appears to interfere with autophagy generally in tauopathies and with the acidification of autolysosomes in particular. A third subset of externalized tau appears to be morphologically dissimilar from vesicle exocytosis, suggesting a mechanism akin to plasma membrane blebbing  or the “membrane shedding” seen with the unconventional secretion of galectin-1  (Figure 10). A more general issue relevant to both dendritic tau secretion and toxicity was raised by a recent study by Ittner et al.  which showed that dendritic localization of tau can selectively mediate Abeta toxicity. This is consistent with the generally dendrite-specific toxicity observed in this study and suggests that the abnormal juxtaposition of tau and dendrite-specific signal transduction mechanisms might play a role in both tau-mediated toxicity and tau secretion.
Little is currently known about exactly how non-MT-associated tau becomes cytotoxic en route to its oligomerization and polymerization into neurofibrillary deposits in human tauopathies other than that (a) tau becomes a substrate for tyrosine as well as serine/threonine kinases and (b) tau undergoes progressive amino and carboxyl terminal cleavage at some point in the process. Here we show that, when tau becomes disassociated from MTs by virtue of overexpression, it is processed via a novel pathway that generates localized cytotoxicity manifested by MT loss and dendritic degeneration that is preceded by the secretion of some of the misprocessed tau via an unconventional mechanism that involves elements of both exosome and autophagy pathways. Tau misprocessing in ABCs involves (1) the interaction of tau with elements in the subcortical cytoskeleton and its phosphorylation of tau at characteristic AD-related sites, (2) the MT-mediated transport of hyperphosphorylated tau in association with vesicles and their accumulation in distal dendrites, and (3) the progressive MT loss and dendritic dysfunction in the immediate vicinity of these deposits, which may be exacerbated by localized secretion followed by extracellularly mediated toxicity. While the roles played by these events in the generation of neurofibrillary deposits, toxic tau oligomers, and the interneuronal spread of tau lesions are still unclear, our results lay the ground for acquiring a more detailed understanding of the role played by tau misprocessing in the cytopathogenesis of neurodegenerative disease.
This study was supported by the Boston University, Alzheimer’s Disease Center (BUADC) NIA P30 AG13846 via a BUADC pilot Grant to G. F. Hall.
- K. Iqbal, I. Grundke-Iqbal, T. Zaidi, et al., “Defective brain microtubule assembly in Alzheimer's disease,” The Lancet, vol. 2, no. 8504, pp. 421–426, 1986.
- A. C. Mckee, N. W. Kowall, and K. S. Kosik, “Microtubular reorganization and dendritic growth response in Alzheimer's disease,” Annals of Neurology, vol. 26, no. 5, pp. 652–659, 1989.
- A. D. C. Alonso, T. Zaidi, M. Novak, I. Grundke-Iqbal, and K. Iqbal, “Hyperphosphorylation induces self-assembly of τ into tangles of paired helical filaments/straight filaments,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 12, pp. 6923–6928, 2001.
- J. Avila, “Tau phosphorylation and aggregation in Alzheimer's disease pathology,” FEBS Letters, vol. 580, no. 12, pp. 2922–2927, 2006.
- V. M. Y. Lee, M. Goedert, and J. Q. Trojanowski, “Neurodegenerative tauopathies,” Annual Review of Neuroscience, vol. 24, pp. 1121–1159, 2001.
- R. A. Crowther, O. F. Olesen, R. Jakes, and M. Goedert, “The microtubule binding repeats of tau protein assemble into filaments like those found in Alzheimer's disease,” FEBS Letters, vol. 309, no. 2, pp. 199–202, 1992.
- J. Götz, F. Chen, R. Barmettler, and R. M. Nitsch, “Tau filament formation in transgenic mice expressing P301L tau,” Journal of Biological Chemistry, vol. 276, no. 1, pp. 529–534, 2001.
- G. F. Hall, B. Chu, G. Lee, and J. Yao, “Human tau filaments induce microtubule and synapse loss in an in vivo model of neurofibrillary degenerative disease,” Journal of Cell Science, vol. 113, no. 8, pp. 1373–1387, 2000.
- G. F. Hall, J. Yao, and G. Lee, “Human tau becomes phosphorylated and forms filamentous deposits when overexpressed in lamprey central neurons in situ,” Proceedings of the National Academy of Sciences of the United States of America, vol. 94, no. 9, pp. 4733–4738, 1997.
- T. Ishihara, M. Hong, B. Zhang et al., “Age-dependent emergence and progression of a tauopathy in transgenic mice overexpressing the shortest human tau isoform,” Neuron, vol. 24, no. 3, pp. 751–762, 1999.
- J. Lewis, E. McGowan, J. Rockwood et al., “Neurofibrillary tangles, amyotrophy and progressive motor disturbance in mice expressing mutant (P301L) tau protein,” Nature Genetics, vol. 25, no. 4, pp. 402–405, 2000.
- C. W. Wittmann, M. F. Wszolek, J. M. Shulman et al., “Tauopathy in Drosophila: neurodegeneration without neurofibrillary tangles,” Science, vol. 293, no. 5530, pp. 711–714, 2001.
- W. H. Stoothoff and G. V. W. Johnson, “Tau phosphorylation: physiological and pathological consequences,” Biochimica et Biophysica Acta, vol. 1739, no. 2, pp. 280–297, 2005.
- M. Hasegawa, M. J. Smith, and M. Goedert, “Tau proteins with FTDP-17 mutations have a reduced ability to promote microtubule assembly,” FEBS Letters, vol. 437, no. 3, pp. 207–210, 1998.
- M. Hong, V. Zhukareva, V. Vogelsberg-Ragaglia et al., “Mutation-specific functional impairments in distinct tau isoforms of hereditary FTDP-17,” Science, vol. 282, no. 5395, pp. 1914–1917, 1998.
- P. Nacharaju, J. Lewis, C. Easson et al., “Accelerated filament formation from tau protein with specific FTDP-17 missense mutations,” FEBS Letters, vol. 447, no. 2-3, pp. 195–199, 1999.
- N. Sahara, T. Tomiyama, and H. Mori, “Missense point mutations of tau to segregate with FTDP-17 exhibit site-specific effects on microtubule structure in COS cells: a novel action of R406W mutation,” Journal of Neuroscience Research, vol. 60, no. 3, pp. 380–387, 2000.
- S. Lee, C. Jung, G. Lee, and G. F. Hall, “Exonic point mutations of human tau enhance its toxicity and cause characteristic changes in neuronal morphology, tau distribution and tau phosphorylation in the lamprey cellular model of tauopathy,” Journal of Alzheimer's Disease, vol. 16, no. 1, pp. 99–111, 2009.
- M. Goedert and R. Jakes, “Mutations causing neurodegenerative tauopathies,” Biochimica et Biophysica Acta, vol. 1739, no. 2, pp. 240–250, 2005.
- M. G. Spillantini and M. Goedert, “Tau protein pathology in neurodegenerative diseases,” Trends in Neurosciences, vol. 21, no. 10, pp. 428–433, 1998.
- N. J. Cairns, V. M. Y. Lee, and J. Q. Trojanowski, “The cytoskeleton in neurodegenerative diseases,” Journal of Pathology, vol. 204, no. 4, pp. 438–449, 2004.
- A. L. Guillozet-Bongaarts, F. Garcia-Sierra, M. R. Reynolds et al., “Tau truncation during neurofibrillary tangle evolution in Alzheimer's disease,” Neurobiology of Aging, vol. 26, no. 7, pp. 1015–1022, 2005.
- M. M. Mocanu, A. Nissen, K. Eckermann et al., “The potential for β-structure in the repeat domain of tau protein determines aggregation, synaptic decay, neuronal loss, and coassembly with endogenous tau in inducible mouse models of tauopathy,” Journal of Neuroscience, vol. 28, no. 3, pp. 737–748, 2008.
- H. Yin and J. Kuret, “C-terminal truncation modulates both nucleation and extension phases of τ fibrillization,” FEBS Letters, vol. 580, no. 1, pp. 211–215, 2006.
- N. Zilka, P. Filipcik, P. Koson et al., “Truncated tau from sporadic Alzheimer's disease suffices to drive neurofibrillary degeneration in vivo,” FEBS Letters, vol. 580, no. 15, pp. 3582–3588, 2006.
- S. Maeda, N. Sahara, Y. Saito et al., “Granular tau oligomers as intermediates of tau filaments,” Biochemistry, vol. 46, no. 12, pp. 3856–3861, 2007.
- R. Brandt, J. Léger, and G. Lee, “Interaction of tau with the neural plasma membrane mediated by tau's amino-terminal projection domain,” Journal of Cell Biology, vol. 131, no. 5, pp. 1327–1340, 1995.
- T. C. Gamblin, R. W. Berry, and L. I. Binder, “Tau polymerization: role of the amino terminus,” Biochemistry, vol. 42, no. 7, pp. 2252–2257, 2003.
- P. M. Horowitz, N. LaPointe, A. L. Guillozet-Bongaarts, R. W. Berry, and L. I. Binder, “N-terminal fragments of tau inhibit full-length tau polymerization in vitro,” Biochemistry, vol. 45, no. 42, pp. 12859–12866, 2006.
- G. S. Bloom, K. Ren, and C. G. Glabe, “Cultured cell and transgenic mouse models for tau pathology linked to β-amyloid,” Biochimica et Biophysica Acta, vol. 1739, no. 2, pp. 116–124, 2005.
- M. E. King, H. M. Kan, P. W. Baas, A. Erisir, C. G. Glabe, and G. S. Bloom, “Tau-dependent microtubule disassembly initiated by prefibrillar β-amyloid,” Journal of Cell Biology, vol. 175, no. 4, pp. 541–546, 2006.
- G. Amadoro, A. L. Serafino, C. Barbato et al., “Role of N-terminal tau domain integrity on the survival of cerebellar granule neurons,” Cell Death and Differentiation, vol. 11, no. 2, pp. 217–230, 2004.
- S. Y. Park and A. Ferreira, “The generation of a 17 kDa neurotoxic fragment: an alternative mechanism by which tau mediates β-amyloid-induced neurodegeneration,” Journal of Neuroscience, vol. 25, no. 22, pp. 5365–5375, 2005.
- V. Corsetti, G. Amadoro, A. Gentile et al., “Identification of a caspase-derived N-terminal tau fragment in cellular and animal Alzheimer's disease models,” Molecular and Cellular Neuroscience, vol. 38, no. 3, pp. 381–392, 2008.
- K. Bhaskar, S. H. Yen, and G. Lee, “Disease-related modifications in tau affect the interaction between fyn and tau,” Journal of Biological Chemistry, vol. 280, no. 42, pp. 35119–35125, 2005.
- G. Lee, S. Todd Newman, D. L. Gard, H. Band, and G. Panchamoorthy, “Tau interacts with src-family non-receptor tyrosine kinases,” Journal of Cell Science, vol. 111, no. 21, pp. 3167–3177, 1998.
- I. E. Vega, L. Cui, J. A. Propst, M. L. Hutton, G. Lee, and S. H. Yen, “Increase in tau tyrosine phosphorylation correlates with the formation of tau aggregates,” Molecular Brain Research, vol. 138, no. 2, pp. 135–144, 2005.
- T. A. Fulga, I. Elson-Schwab, V. Khurana et al., “Abnormal bundling and accumulation of F-actin mediates tau-induced neuronal degeneration in vivo,” Nature Cell Biology, vol. 9, no. 2, pp. 139–148, 2007.
- C. A. Farah, S. Perreault, D. Liazoghli et al., “Tau interacts with golgi membranes and mediates their association with microtubules,” Cell Motility and the Cytoskeleton, vol. 63, no. 11, pp. 710–724, 2006.
- W. Kim, S. Lee, and G. F. Hall, “Secretion of human tau fragments resembling CSF-tau in Alzheimer's disease is modulated by the presence of the exon 2 insert,” FEBS Letters, vol. 584, no. 14, pp. 3085–3088, 2010.
- W. Kim, S. Lee, C. Jung, A. Ahmed, G. Lee, and G. F. Hall, “Interneuronal transfer of human tau between lamprey central neurons in situ,” Journal of Alzheimer's Disease, vol. 19, no. 2, pp. 647–664, 2010.
- B. Frost, R. L. Jacks, and M. I. Diamond, “Propagation of tau misfolding from the outside to the inside of a cell,” Journal of Biological Chemistry, vol. 284, no. 19, pp. 12845–12852, 2009.
- F. Clavaguera, T. Bolmont, R. A. Crowther et al., “Transmission and spreading of tauopathy in transgenic mouse brain,” Nature Cell Biology, vol. 11, no. 7, pp. 909–913, 2009.
- S. J. Pleasure, M. E. Selzer, and V. M. Y. Lee, “Lamprey neurofilaments combine in one subunit the features of each mammalian NF triplet protein but are highly phosphorylated only in large axons,” Journal of Neuroscience, vol. 9, no. 2, pp. 698–709, 1989.
- G. F. Hall, B. Chu, S. Lee, Y. Liu, and J. Yao, “The single neurofilament subunit of the lamprey forms filaments and regulates axonal caliber and neuronal size in vivo,” Cell Motility and the Cytoskeleton, vol. 46, no. 3, pp. 166–182, 2000.
- G. F. Hall, A. Poulos, and M. J. Cohen, “Sprouts emerging from the dendrites of axotomized Lamprey central neurons have axonlike ultrastructure,” Journal of Neuroscience, vol. 9, no. 2, pp. 588–599, 1989.
- G. F. Hall, V. M. Y. Lee, and K. S. Kosik, “Microtubule destabilization and neurofilament phosphorylation precede dendritic sprouting after close axotomy of lamprey central neurons,” Proceedings of the National Academy of Sciences of the United States of America, vol. 88, no. 11, pp. 5016–5020, 1991.
- G. F. Hall, J. Yao, M. E. Selzer, and K. S. Kosik, “Cytoskeletal changes correlated with the loss of neuronal polarity in axotomized lamprey central neurons,” Journal of Neurocytology, vol. 26, no. 11, pp. 733–753, 1997.
- G. F. Hall and V. M. Y. Lee, “Neurofilament sidearm proteolysis is a prominent early effect of axotomy in lamprey giant central neurons,” Journal of Comparative Neurology, vol. 353, no. 1, pp. 38–49, 1995.
- D. S. Pijak, G. F. Hall, P. J. Tenicki, A. S. Boulos, D. I. Lurie, and M. E. Selzer, “Neurofilament spacing, phosphorylation, and axon diameter in regenerating and uninjured lamprey axons,” Journal of Comparative Neurology, vol. 368, no. 4, pp. 569–581, 1996.
- M. Goedert, C. P. Baur, J. Ahringer et al., “PTL-1, a microtubule-associated protein with tau-like repeats from the nematode Caenorhabditis elegans,” Journal of Cell Science, vol. 109, no. 11, pp. 2661–2672, 1996.
- G. F. Hall, V. M. Y. Lee, G. Lee, and J. Yao, “Staging of neurofibrillary degeneration caused by human tau overexpression in a unique cellular model of human tauopathy,” American Journal of Pathology, vol. 158, no. 1, pp. 235–246, 2001.
- A. Schneider, J. Biernat, M. Von Bergen, E. Mandelkow, and E. M. Mandelkow, “Phosphorylation that detaches tau protein from microtubules (Ser262, Ser214) also protects it against aggregation into Alzheimer paired helical filaments,” Biochemistry, vol. 38, no. 12, pp. 3549–3558, 1999.
- D. Fischer, M. D. Mukrasch, J. Biernat et al., “Conformational changes specific for pseudophosphorylation at serine 262 selectively impair binding of tau to microtubules,” Biochemistry, vol. 48, no. 42, pp. 10047–10055, 2009.
- P. Seubert, M. Mawal-Dewan, R. Barbour et al., “Detection of phosphorylated Ser262 in fetal tau, adult tau, and paired helical filament tau,” Journal of Biological Chemistry, vol. 270, no. 32, pp. 18917–18922, 1995.
- H. Kameda, T. Furuta, W. Matsuda et al., “Targeting green fluorescent protein to dendritic membrane in central neurons,” Neuroscience Research, vol. 61, no. 1, pp. 79–91, 2008.
- J. B. McCabe and L. G. Berthiaume, “Functional roles for fatty acylated amino-terminal domains in subcellular localization,” Molecular Biology of the Cell, vol. 10, no. 11, pp. 3771–3786, 1999.
- J.-P. Brion, G. Tremp, and J.-N. Octave, “Transgenic expression of the shortest human tau affects its compartmentalization and its phosphorylation as in the pretangle stage of Alzheimer's disease,” American Journal of Pathology, vol. 154, no. 1, pp. 255–270, 1999.
- J. Gotz, A. Probst, M. G. Spillantini et al., “Somatodendritic localization and hyperphosphorylation of tau protein in transgenic mice expressing the longest human brain tau isoform,” The EMBO Journal, vol. 14, no. 7, pp. 1304–1313, 1995.
- Y. Kanai and N. Hirokawa, “Sorting mechanisms of tau and MAP2 in neurons: suppressed axonal transit of MAP2 and locally regulated microtubule binding,” Neuron, vol. 14, no. 2, pp. 421–432, 1995.
- P. Litman, J. Barg, L. Rindzoonski, and I. Ginzburg, “Subcellular localization of tau mRNA in differentiating neuronal cell culture: implications for neuronal polarity,” Neuron, vol. 10, no. 4, pp. 627–638, 1993.
- A. J. Myers, A. M. Pittman, A. S. Zhao et al., “The MAPT H1c risk haplotype is associated with increased expression of tau and especially of 4 repeat containing transcripts,” Neurobiology of Disease, vol. 25, no. 3, pp. 561–570, 2007.
- A. Samsonov, J. Z. Yu, M. Rasenick, and S. V. Popov, “Tau interaction with microtubules in vivo,” Journal of Cell Science, vol. 117, no. 25, pp. 6129–6141, 2004.
- R. Dixit, J. L. Ross, Y. E. Goldman, and E. L. F. Holzbaur, “Differential regulation of dynein and kinesin motor proteins by tau,” Science, vol. 319, no. 5866, pp. 1086–1089, 2008.
- L. C. Kapitein, M. A. Schlager, M. Kuijpers et al., “Mixed microtubules steer dynein-driven cargo transport into dendrites,” Current Biology, vol. 20, no. 4, pp. 290–299, 2010.
- L. M. Ittner, Y. D. Ke, and J. Götz, “Phosphorylated tau interacts with c-Jun N-terminal kinase-interacting protein 1 (JIP1) in Alzheimer disease,” Journal of Biological Chemistry, vol. 284, no. 31, pp. 20909–20916, 2009.
- T. L. Falzone, G. B. Stokin, C. Lillo et al., “Axonal stress kinase activation and tau misbehavior induced by kinesin-1 transport defects,” Journal of Neuroscience, vol. 29, no. 18, pp. 5758–5767, 2009.
- E. Braak, H. Braaak, and E. M. Mandelkow, “A sequence of cytoskeleton changes related to the formation of neurofibrillary tangles and neuropil threads,” Acta Neuropathologica, vol. 87, no. 6, pp. 554–567, 1994.
- C. Bancher, C. Brunner, H. Lassmann et al., “Accumulation of abnormally phosphorylated τ precedes the formation of neurofibrillary tangles in Alzheimer's disease,” Brain Research, vol. 477, no. 1-2, pp. 90–99, 1989.
- N. Sahara, S. Maeda, and A. Takashima, “Tau oligomerization: a role for tau aggregation intermediates linked to neurodegeneration,” Current Alzheimer Research, vol. 5, no. 6, pp. 591–598, 2008.
- K. Santacruz, J. Lewis, T. Spires et al., “Medicine: tau suppression in a neurodegenerative mouse model improves memory function,” Science, vol. 309, no. 5733, pp. 476–481, 2005.
- C. N. Chirita, M. Necula, and J. Kuret, “Anionic micelles and vesicles induce tau fibrillization in vitro,” Journal of Biological Chemistry, vol. 278, no. 28, pp. 25644–25650, 2003.
- P. Barré and D. Eliezer, “Folding of the repeat domain of tau upon binding to lipid surfaces,” Journal of Molecular Biology, vol. 362, no. 2, pp. 312–326, 2006.
- E. G. Gray, M. Paula-Barbosa, and A. Roher, “Alzheimer's disease: paired helical filaments and cytomembranes,” Neuropathology and Applied Neurobiology, vol. 13, no. 2, pp. 91–110, 1987.
- I. Grundke-Iqbal, K. Iqbal, and Y.-C. Tung, “Abnormal phosphorylation of the microtubule-associated protein τ (tau) in Alzheimer cytoskeletal pathology,” Proceedings of the National Academy of Sciences of the United States of America, vol. 83, no. 13, pp. 4913–4917, 1986.
- A. M. Cataldo, D. J. Hamilton, and R. A. Nixon, “Lysosomal abnormalities in degenerating neurons link neuronal compromise to senile plaque development in Alzheimer disease,” Brain Research, vol. 640, no. 1-2, pp. 68–80, 1994.
- T. Hamano, T. F. Gendron, E. Causevic et al., “Autophagic-lysosomal perturbation enhances tau aggregation in transfectants with induced wild-type tau expression,” European Journal of Neuroscience, vol. 27, no. 5, pp. 1119–1130, 2008.
- V. Khurana, I. Elson-Schwab, T. A. Fulga et al., “Lysosomal dysfunction promotes cleavage and neurotoxicity of tau in vivo,” PLoS Genetics, vol. 6, no. 7, Article ID e1001026, 11 pages, 2010.
- B. Boland, A. Kumar, S. Lee et al., “Autophagy induction and autophagosome clearance in neurons: relationship to autophagic pathology in Alzheimer's disease,” Journal of Neuroscience, vol. 28, no. 27, pp. 6926–6937, 2008.
- P. J. Dolan and G. V. W. Johnson, “A caspase cleaved form of tau is preferentially degraded through the autophagy pathway,” Journal of Biological Chemistry, vol. 285, no. 29, pp. 21978–21987, 2010.
- R. A. Nixon, J. Wegiel, A. Kumar et al., “Extensive involvement of autophagy in Alzheimer disease: an immuno-electron microscopy study,” Journal of Neuropathology and Experimental Neurology, vol. 64, no. 2, pp. 113–122, 2005.
- S. Saman, W. Kim, M. Raya et al., “Exosome-associated tau is secreted in tauopathy models and is selectively phosphorylated in cerebrospinal fluid (CSF) in early Alzheimer's Disease,” The Journal of Biological Chemistry. In press.
- M. P. Lambert, A. K. Barlow, B. A. Chromy et al., “Diffusible, nonfibrillar ligands derived from Aβ1-42 are potent central nervous system neurotoxins,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 11, pp. 6448–6453, 1998.
- M. Rapoport, H. N. Dawson, L. I. Binder, M. P. Vitek, and A. Ferreira, “Tau is essential to β-amyloid-induced neurotoxicity,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 9, pp. 6364–6369, 2002.
- G. Lee, R. Thangavel, V. M. Sharma et al., “Phosphorylation of tau by fyn: implications for Alzheimer's disease,” Journal of Neuroscience, vol. 24, no. 9, pp. 2304–2312, 2004.
- G. J. Ho, M. Hashimoto, A. Adame et al., “Altered p59Fyn kinase expression accompanies disease progression in Alzheimer's disease: implications for its functional role,” Neurobiology of Aging, vol. 26, no. 5, pp. 625–635, 2005.
- N. Blanchard, D. Lankar, F. Faure et al., “TCR activation of human T cells induces the production of exosomes bearing the TCR/CD3/ζ complex,” Journal of Immunology, vol. 168, no. 7, pp. 3235–3241, 2002.
- M. Sverdlov, A. N. Shajahan, and R. D. Minshall, “Tyrosine phosphorylation-dependence of caveolae-mediated endocytosis,” Journal of Cellular and Molecular Medicine, vol. 11, no. 6, pp. 1239–1250, 2007.
- Y. Fang, N. Wu, X. Gan, W. Yan, J. C. Morrell, and S. J. Gould, “Higher-order oligomerization targets plasma membrane proteins and HIV gag to exosomes,” PLoS Biology, vol. 5, no. 6, article e158, 2007.
- W. Nickel, “Unconventional secretory routes: direct protein export across the plasma membrane of mammalian cells,” Traffic, vol. 6, no. 8, pp. 607–614, 2005.
- Y. Wang, M. Martinez-Vicente, U. Krüger et al., “Tau fragmentation, aggregation and clearance: the dual role of lysosomal processing,” Human Molecular Genetics, vol. 18, no. 21, pp. 4153–4170, 2009.
- O. T. Fackler and R. Grosse, “Cell motility through plasma membrane blebbing,” Journal of Cell Biology, vol. 181, no. 6, pp. 879–884, 2008.
- L. M. Ittner, Y. D. Ke, F. Delerue et al., “Dendritic function of tau mediates amyloid-β toxicity in alzheimer's disease mouse models,” Cell, vol. 142, no. 3, pp. 387–397, 2010.