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TorsinA is an AAA+ ATPase located within the lumen of the endoplasmic reticulum and nuclear envelope, with a mutant form causing early onset torsion dystonia (DYT1). Here we report a new function for torsinA in endoplasmic reticulum-associated degradation (ERAD). Retro-translocation and proteosomal degradation of a mutant cystic fibrosis transmembrane conductance regulator (CFTRΔF508) was inhibited by downregulation of torsinA or overexpression of mutant torsinA, and facilitated by increased torsinA. Retro-translocation of cholera toxin was also decreased by downregulation of torsinA. TorsinA associates with proteins implicated in ERAD, including Derlin-1, VIMP, and p97. Further, torsinA reduces endoplasmic reticulum stress in nematodes overexpressing CFTRΔF508, and fibroblasts from DYT1 dystonia patients are more sensitive than controls to endoplasmic reticulum stress and less able to degrade mutant CFTR. Therefore, compromised ERAD function in the cells of DYT1 patients may increase sensitivity to endoplasmic reticulum stress with consequent alterations in neuronal function contributing to the disease state.
Most cases of the dominantly inherited human movement disorder, early onset torsion dystonia (DYT1), are caused by a 3 bp deletion (GAG), resulting in loss of a glutamic acid (ΔE302 or 303) in the carboxy terminal region of torsinA1. TorsinA is a member of the AAA+ ATPase superfamily of proteins, which have a variety of cellular locations and functions2,3, and has some homology to the bacterial chaperone protein, ClpB4. TorsinA is located predominantly in the contiguous lumen of the endoplasmic reticulum (ER) and nuclear envelope (NE)5, and thought to be retained there by association with membrane spanning proteins6,7. The ΔE deletion is thought to cause loss-of-function and to suppress wild-type torsinA activity8,9. Recent studies have implicated torsinA in interactions between proteins in the outer membrane of the NE and the cytoskeleton involved in nuclear polarization10, and in the inner and outer NE membranes contributing to NE morphology11,12, as well as participating in processing of proteins through the ER component of the secretory pathway13,14,15.
ER protein homeostasis depends on retro-translocation to the cytosol of abnormal proteins destined for destruction by the ubiquitin-dependent protease, known as ER-associated protein degradation (ERAD)16. Perturbations in the ERAD pathway can contribute to formation of inclusions, abnormal ER morphology and ER stress when the ER is overloaded with proteins and cannot process them through the Golgi/secretory pathway or eliminate them at a sufficient rate. ER chaperones recognize terminally misfolded proteins and target them for retro-translocation into the cytoplasm. Several membrane proteins have been identified and proposed to form one or a few conducting channels in retro-translocation. These include the Derlins, the Sec61 complex, and several ER-associated multi-spanning ubiquitin ligases, including Hrd1. Ubiquitin ligases are essential to the retro-translocation of many substrates, not only for their potential involvement in the translocation process per se, but also for decorating ERAD substrates with polyubiquitin chains, which are required for subsequent extraction of ERAD substrates by the p97 ATPase and its cofactors, Ufd1-Npl417. With the aid of another set of cofactors, p97 then transfers the substrates to the 26S proteasome for degradation18. Different ER exit/degradation strategies may be used by various proteins depending on whether misfolding signals are located in the lumen, membrane or exposed on the cytosolic face of the ER. For example, cholera toxin (CT) enters host cells by trafficking retrograde from the cell surface through the secretory pathway to the ER lumen. In the ER, protein disulfide isomerase (PDI) in its reduced state unfolds and dissociates the A1-chain from the B-subunit. When oxidized, PDI releases the A1-chain to subsequent steps in the retro-translocation reaction19. Unlike most ERAD substrates, the A1-chain does not require ubiquitination20 or interaction with p97 for retro-translocation21, and it rapidly refolds after entry into the cytosol escaping degradation by the proteasome long enough to induce massive intestinal chloride and water secretion that is the hallmark of cholera22.
In the present study we evaluated the association of endogenous and overexpressed torsinA, as well as mutant/variant forms of this protein, with members of the ER retro-translocation complex including Derlin-1, p97, VIMP and Hrd1 in different cell types in culture. Levels of torsinA, as regulated by siRNA or overexpression, altered ERAD of distinct test substrates, including the mutant cystic fibrosis transmembrane conductance regulator (CFTR), GFP-CFTRΔF50823 and an ER fusion protein, BAP31-RFP, as well as ER exit of the A1 peptide of cholera toxin (CTA1). Notably, overexpression of torsinA increased degradation of GFP-CFTRΔF508, with carboxy terminal truncated torsinAΔ313–332 (torsinAΔC) and torsinAΔE being less efficient in this function. Compromised ERAD function was also observed in fibroblasts from DYT1 patients as compared to controls manifested as a reduced ability to degrade GFP-CFTRΔF508. These studies support a role for torsinA in retro-translocation of abnormal proteins/toxin out of the ER, with mutant torsinA being compromised in this function. Our studies also implicate torsinA in modulation of sensitivity to ER stress, with overexpression of human torsinA in nematodes alleviating stress caused by high levels of GFP-CFTRΔF508, and DYT1 patient fibroblasts having abnormally high sensitivity to pharmacologically induced ER stress.
Initially we used immunocytochemistry to evaluate the association of torsinA with established members of ERAD membrane complexes, including Derlin-1, p97 and VIMP224 (see Fig. 1 a–c for typical localization patterns of tagged fusion proteins overexpressed individually). Previous studies have shown that when tagged His-p97, HA-Derlin-1, and Myc-VIMP are co-expressed in COS-7 cells, their multivalent interactions lead to the formation of large puncta around the nucleus, with the presence of Derlin-1 in these inclusions being dependent on VIMP25. When mCherry Derlin-1 and torsinA were co-expressed in COS-7 cells, they showed primarily a reticular ER-like distribution throughout the cell (with rare co-localization in puncta) (Fig. 1 d–f). When His-p97 and Myc-VIMP were included in the co-transfection mix, torsinA was recruited to puncta together with Derlin-1, p97 and VIMP (Fig. 1 g–n). When Derlin-1 was left out of this co-transfection mixture, Myc-VIMP/His-p97 formed puncta lacking torsinA (Fig. 2 a–f). Apparently levels of endogenous Derlin-1 are not sufficient to recruit torsinA into puncta. In these same cells, staining for the ER marker, PDI showed a reticular ER-like distribution, similar to torsinA, indicating that the basic ER structure was not disrupted in the presence of His-p97/Myc-VIMP puncta (Fig. 2 g–i). Thus, under these conditions, the association of torsinA with members of the ERAD complex, including p97 and VIMP is dependent on Derlin-1.
To evaluate whether endogenous torsinA and Derlin-1 participate in the ERAD complex, we immunoprecipitated p97 from microsomes isolated from 293T cells followed by western blotting for p97, torsinA, Derlin-1 and VIMP (Fig. 2 j). All four proteins co-immunoprecipitated, supporting an association of torsinA with Derlin-1 in an ERAD complex containing p97, VIMP and Derlin-1. When endogenous levels of Derlin-1 were decreased using siRNA, torsinA could no longer be co-precipitated with p97 (Fig. 2 k), indicating that Derlin-1 serves a bridging function between these two proteins.
Since torsion dystonia is a disease of neuronal dysfunction, we also evaluated the interaction between torsinA and Derlin-1 (the only Derlin found in brain)26 in primary mouse neurons. Neuronal cultures were infected with AAV vectors encoding either human torsinA or torsinAΔE and immunocytochemistry was carried out 70 h later. In the presence of human torsinA, torsinA and Derlin-1 immunoreactivity was found distributed throughout the cell, consistent with ER localization (Fig. 3 a–c). In contrast, in the presence of human torsinAΔE, torsinA immunoreactivity was concentrated around the nuclear envelope, and Derlin-1 was also enriched in that location (Fig. 3 d–f). When lysates of uninfected neuronal cultures were subject to immunoprecipitation with antibodies specific to mouse torsinA, the p97 and Derlin-1 proteins co-precipitated with torsinA (Fig. 3 g). In fact, the association of torsinA and Derlin-1 was so strong that the total lysate blot had to be overexposed to visualize endogenous Derlin-1 (inset box), while that bound to torsinA yielded a strong band at lower exposure.
We also evaluated the potential association of torsinA with Hrd1, a putative ERAD channel component known to interact with p9727. We used a Hrd1-GFP fusion protein previously shown to form perinuclear puncta with His-p97 and Myc-VIMP, which did not incorporate Sec61alpha or Derlin-127. Using 293T and COS-7 cells, we were not able to co-immunoprecipitate torsinA with either Hrd-1 or Hrd-1GFP.
In initial experiments, co-immunoprecipitation and western blotting showed an association between the mutant fusion protein, GFP-CFTRΔF508 and torsinA (Fig. 4 a). To evaluate whether torsinA was involved in ERAD of this mutant protein, we tested whether overexpression of torsinA, torsinAΔE or torsinAΔC in 293T cells would alter the rate of degradation of GFP-CFTRΔF508. Mutant forms of CFTR are known to be primarily degraded through a Derlin-1 dependent mechanism23. Following co-transfection of cells with appropriate expression constructs, levels of GFP- CFTRΔF508 were markedly reduced when wild-type torsinA was overexpressed, and were decreased to a lesser degree with overexpression of torsinAΔE or torsinAΔΔC, as assessed by western blot analysis (Fig. 4 b). When band densities were normalized to protein loading (βactin) and amount of torsinA expressed, it was clear that elevated levels of torsinA facilitated degradation of GFP-CFTRΔF508, while mutant forms of torsinA were less efficient, with torsinAΔC being even less effective than torsinAΔE (Fig. 4 c). The disparity in levels of GFP-CFTRΔF508 in combination with expression of wild-type and mutant forms of torsinA was abrogated by treatment with MG132, which blocks proteolytic degradation of proteins exiting the ER through the ERAD pathway (Fig. 4 b). When rates of degradation of GFP-CFTRΔF508 were monitored over time after cycloheximide inhibition of synthesis, the rate of degradation was approximately 2-fold faster in the presence of elevated torsinA than under endogenous conditions (Supplementary Fig. S1). Overexpression of different forms of torsinA showed a differential distribution in cells. Overexpression of wild-type torsinA had no marked effect on its ER distribution (Supplementary Fig. S2 a–c) as compared to endogenous torsinA5,7, showing the typical reticular pattern throughout the cell body. In contrast, when torsinAΔE was overexpressed torsinA-immunoreactivity tended to accumulate in the NE region (Fig. 3 d), and when torsinAΔC was overexpressed, the ER assumed a “honeycomb” vacuolar appearance for both torsinA and PDI (Supplementary Fig. S2 d–f), similar to that observed when p97 function is inhibited (Dr. George DeMartino, personal communication)28.
To further evaluate whether torsinA functions in ERAD degradation of GFP-CFTRΔF508, 293T cells were transfected with siRNAs which downregulate endogenous torsinA levels15. Degradation of GFP-CFTRΔF508 was evaluated under conditions of normal levels or >80% reduction of endogenous torsinA (Fig. 4 d). Lowering torsinA levels markedly reduced the degradation of this mutant fusion protein, and this difference disappeared when the proteosomal pathway was inhibited. Quantitation of GFP-CFTRΔF508 band density, normalized as above, showed a 2–3-fold increase in this mutant fusion protein with downregulation of torsinA (Fig. 4 e). In addition, lowering of Derlin-1 levels with siRNA reduced the degradation of GFP- CFTRΔF508 and significantly decreased the ability of overexpressed torsinA to augment degradation (Fig. 4 f and g). Together these findings support a role for torsinA in ERAD of GFP-CFTRΔF508, with mutation/deletion in the carboxy terminal region of torsinA or decreased levels of Derlin-1 compromising this function.
We also explored the role of torsinA in ERAD of two other ER membrane substrates - the alpha chain of the T cell receptor (TCRalpha), which is degraded by a Derlin-1 independent mechanism29, and a novel substrate consisting of RFP fused to the ER membrane protein, BAP3130. 293T cells were co-transfected with a control plasmid or expression cassettes for torsinA or torsinAΔE and TCRalpha-YFP in the presence and absence of tunicamycin, which causes protein misfolding and increases ERAD, and lysates were analyzed by western blot staining for YFP, torsinA and p97 (Supplementary Fig. S3 a). No marked changes were found in the levels TCRalpha-YFP in the presence of either form of torsinA, as compared to controls, indicating that torsinA does not appear to participate in the ERAD of this substrate.
As another potential ERAD substrate, we generated an expression cassette for an ER membrane protein, BAP31 fused to RFP (apparent molecular weight of ~55 kD). When 293T cells were transfected with this expression cassette and endogenous torsinA was decreased by transfection with an siRNA, levels of BAP31-RFP increased (Supplementary Fig. S3 b), consistent with a role for torsinA in degradation of this substrate. When BAP31-RFP was overexpressed in cells overexpressing mGFP, torsinA-mGFP, torsinAΔE-mGFP or torsinAΔC-mGFP, western blot analysis verified a marked decrease in the amount of BAP31-RFP in the presence of torsinA-mGFP, which was less than with torsinAΔE-mGFP and torsinAΔC-mGFP, as compared to the control mGFP (Supplementary Fig. S3 c). This enhanced degradation of BAP31-RFP by torsinA-mGFP was substantially blocked by inhibition of proteolytic degradation, indicating a role for torsinA in ERAD of BAP31-RFP. By way of control, endogenous BAP31 levels were not affected by overexpression of torsinA-mGFP, torsinAΔE-mGFP or torsinAΔC-mGFP (Supplementary Fig. S3 c).
We also evaluated the role of torsinA in the retro-translocation of the cholera toxin A1-chain (CTA1). Retro-translocation was measured by the presence of the A1-chain in the cytosolic fractions of intoxicated cells treated or not with siRNA against torsinA by SDS-PAGE and immunoblot using antibodies against the CTA- and B-subunits. In cells with reduced torsinA (Fig. 5 a), the levels of CTA1 in the cytosol were dramatically reduced to 34%±0.05 and 47%±0.09, respectively, compared to negative control cells (Fig. 5 b and c). Immunoblot for CTB, which does not retro-translocate, and the ER lumenal protein BiP were detected only in membrane fractions, showing that ER membranes were intact in this assay with no leakage of luminal proteins to the cytosol and that only the A1-chain was retro-translocated (Fig. 5 b). Equal amounts of CTA and CTB were observed in the membrane fractions showing that equal amounts of toxin were taken up by control and torsinA knock-down cells (Fig. 5 b). β-actin and Hsp90 as controls indicating equal loading of each lane. The same results were obtained whether or not the cells were treated with MG132, showing that the loss of A1-chain in the cytosol cannot be explained by enhanced proteasome degradation (Supplementary Fig. S4). Finally, to exclude an unexpected effect of torsinA on the retrograde trafficking pathways, which could also reduce the amount of A1-chain in the cytosol by blocking entry of CT into the ER, we used the mutant toxin CTB-GS that contains tyrosine-sulfation and N-glycosylation motifs and reports quantitatively on toxin entry into the transGolgi network (TGN) and ER, respectively31. For these studies, the fraction of CTB-GS entering the ER was assessed by affinity isolation on concanavalin beads, which bind all N-glycosylated proteins. We found the same amount of N-glycosylated CTB-GS in cells lacking torsinA compared to control cells (Fig. 5 d and e). To confirm these results, we measured trafficking of CT into the ER by morphology. Here, CT transport into the ER was assessed by three blinded investigators as the fraction of cells with fluorophore-labeled CTB staining the entire circumference of the NE and co-localized with the ER luminal protein, PDI. Again, we found no difference in toxin entry into the ER in cells lacking torsinA compared to controls (Fig. 5 f and g). Both studies show that retrograde trafficking of CT from the plasma membrane into the ER is not affected by depletion of torsinA. Thus, torsinA has an active role in retro-translocation of CTA1 from the lumen of the ER into the cytosol.
A nematode model was used to further explore an important functional consequence of torsinA activity in eliminating abnormal proteins from the ER, the capacity to protect cells from ER stress. We combined a well characterized transgenic ER stress model, in which a GFP reporter is under the control of the hsp-4 promoter expressed in the intestine (a tissue type which lacks endogenous worm torsin expression14), with transgenic worms producing human wild-type CFTR or mutant CFTRΔF508 raised at 20°C32. We confirmed strong induction of GFP expression in these worms in intestinal cells in response to CFTRΔF508 and found a marked reduction in this induction in worms co-expressing torsinA (Fig. 6 a and b), consistent with alleviation of ER stress. Analysis of mRNA levels did not indicate a difference in levels of expression of CFTRΔF508 mRNA as normalized to ama-1 mRNA (Fig. 6 c). Notably, co-expression of torsinAΔE and CFTRΔF508 caused embryonic lethality, so we were unable to assess the relative effectiveness of torsinAΔE in this ER stress paradigm. This in vivo assessment supports the hypothesis that elevated levels of torsinA can reduce ER stress caused by mutant proteins.
To evaluate whether endogenous levels of torsinAΔE in patient cells contribute to increased sensitivity to ER stress, we monitored one of the first responses to different kinds of ER stress, a temporary decrease in translation of most proteins33. We previously developed a sensitive assay to measure this initial ER stress response by quantitating release of the naturally secreted Gaussia luciferase (Gluc) into the cell medium34. Note. Release of Gluc by patient and DYT1 cells was not affected by the presence of MG132, indicating that most is secreted from cells. We exposed cultured primary skin fibroblasts from controls and DYT1 patients expressing Gluc to two agents known to cause ER stress, dithiothreitol (DTT) and 6-hydroxydopamine (6-OHDA)35. ER stress was assessed by Gluc activity in the culture medium at 4 h after exposure to increasing drug concentrations. Two DYT1 fibroblast lines showed a 40–60% decrease in Gluc activity at 0.1 mM DTT, while control cells showed little to no decrease in activity up to 0.5 mM; for 6-OHDA there was a 50–60% decrease at 10 μM for DYT1 cells and a 20–30% decrease at 25 μM for control cells (Fig. 7 a and b). Thus, the DYT1 fibroblasts were more sensitive to ER stress caused by either DTT (about 5-fold), or by 6-OHDA (greater than 2-fold), when compared to control fibroblasts. These data support an increased sensitivity of DYT1 patient cells to ER stress, consistent with higher resident level of misfolded proteins in the ER presumably due to reduced ability to remove them through the ERAD pathway.
In order to express GFP-CFTRΔF508 in primary skin fibroblasts, it was necessary to use a viral vector, as these cells have a very low DNA transfection efficiency. DYT1 and control fibroblasts were infected with adenoviral vectors expressing GFP (to monitor infection efficiency) or GFP- CFTRΔF508. A representative western blot to assess levels of GFP-CFTRΔF508, GFP and βactin showed more degradation of GFP-CFTRΔF508 in control as compared to DYT1 fibroblasts (Fig. 7 c). Relative levels of GFP-CFTRΔF508 expressed as the mean + S.D. for two control and two DYT1 lines, demonstrated about a 10-fold decrease in degradation by DYT1 cells (Fig. 7 d). One additional DYT1 patient line and two additional control lines were also evaluated and gave results consistent with these differences.
Our findings support an active role for torsinA in the retro-translocation of select abnormal proteins targeted for degradation from the lumen of the ER through the cytosolic proteosome pathway, as well as retro-translocation of cholera toxin peptide, CTA1. This retro-translocation function appears to be mediated, at least in part, through association of torsinA with Derlin-1, p97, and VIMP, all of which are implicated in ERAD. However, no indication of an interaction between torsinA and Hrd1 was found. Either downregulation of torsinA or overexpression of torsinAΔE (associated with early onset dystonia) was associated with decreased efficiency of ERAD for a mutant membrane-spanning protein, GFP-CFTRΔF508, thus, potentially sensitizing cells expressing mutant torsinA to ER stress associated with the unfolded protein response33. As a corollary, elevated expression of human torsinA in cultured cells facilitated degradation of GFP-CFTRΔF508 and an ER-membrane fusion protein, BAP31-RFP. In nematodes, expression of human torsinA reduced ER stress caused by overexpression of wild-type or mutant CFTR. Further, fibroblasts from DYT1 patients showed an increased sensitivity to ER stress-inducing drugs, and a decreased ability to degrade GFP-CFTRΔF508, as compared to control fibroblasts. Our data are consistent with torsinA functioning as a shuttle or chaperone protein transferring substrates to an ERAD channel translocon complex (Fig. 8), with mutant torsinA being deficient in this process and thus predisposing cells to ER stress.
ERAD is a complex process in which diverse protein substrates may use different retro- translocation channel complexes to exit the ER. For example, CFTR and mutant forms, e.g. ΔF508, as well as the ER membrane protein, CD3delta appear to require Derlin-1 for retro-translocation, while the degradation of TCRalpha is independent of Derlin-129. Our findings indicate that downregulation of torsinA or the presence of torsinAΔE found in DYT1 patients significantly inhibited elimination of GFP-CFTRΔF508 and BAP31-RFP out of the ER for proteolytic degradation. Likewise, downregulation of torsinA also inhibited the retro-translocation of the CTA1-peptide. However, upregulation of torsinA levels did not appear to affect ERAD of TCRalpha-YFP. Thus, torsinA appears to be involved in the retro-translocation of a subset of ER proteins.
Defective ERAD function and ER stress have a contributing role in neurologic diseases36. In response to stress, cells temporarily decrease protein synthesis, increase movement of unfolded proteins out of the ER into the cytoplasm via ERAD, and upregulate transcription of some chaperone proteins33. This response serves to protect cells from a variety of toxic insults which interfere with protein processing. When this response is overwhelmed by acute or long term ER stress, cellular physiology can be compromised, and in extreme cases lead to cell death. Protein components of the ERAD pathway, e.g. p97, as well as torsinA, have been found in inclusion bodies in brain and peripheral nerves from patients with a variety of neurodegenerative diseases, as well as dystonia37,38,39,40. Additional, complementary evidence indicates that torsinA can reduce ER stress caused by ER protein overload in nematodes and that torsinA deficient mouse embryonic fibroblasts (MEFs) have increased levels of ER stress as compared to wild-type MEFs41.
TorsinA has been found to associate with several different proteins, and may have different functions in the NE and ER. Interacting partners in the NE include proteins which span the inner or outer membranes, including LAP1, LULL1, Sun2 and the nesprins, and appear to influence the morphology of the NE11,8,42,12 and positioning of the nucleus during cell migration10. Within the ER, proteins associated with torsinA include the chaperone protein, calnexin43 and proteins implicated in ERAD, including Derlin-1, p97 and VIMP (this study). Thus, within the ER torsinA appears to participate in decisions concerning the fate of proteins being processed through the secretory pathway.
Ongoing investigations suggest several ways in which the nervous system may become dysfunctional in DYT1 mutant gene carriers. First, reduced ability of mutant torsinA to degrade some abnormal proteins, as compared to wild-type torsinA (this study), may cause increased sensitivity of DYT1 neurons to ER stress. Thus, under stressful conditions, e.g. high body temperature, oxidative stress, trauma or exposure to specific drugs, neurons in DYT1 carriers may experience toxic effects that compromise their function and alter neurotransmission44. As a corollary, ischemia or resection of nervous tissue in experimental animals results in upregulation of torsinA transcription, possibly as a compensatory mechanism45. Second, a number of studies have implicated torsinA in processing proteins through the secretory pathway, showing that reduced torsinA, the presence of torsinAΔE or abnormally high levels of wild-type torsinA can interfere with protein processing13,14,15. This may explain the apparently reduced/altered function of the D2 receptor46 and the dopamine release process47,48 in neurons in the basal ganglia of transgenic mice expressing human torsinAΔE. Third, the normally very high levels of torsinA in the embryonic/perinatal in rodents49,50 and humans51 supports a role in neuronal development. Studies using torsinA knock-out embryos52 indicate that tangential migration of GABAergic neuroprecursor cells is compromised in the absence of torsinA53, possibly leading to reduced numbers of inhibitory GABAergic neurons in the adult brain. Thus, dystonia may result from abnormalities at multiple cellular and system levels in the brain with contributions from increased sensitivity to environmental insults, compromised processing of components of neurotransmission, and subtle developmental neuroanatomical anomalies.
This study expands our mechanistic understanding of torsinA in facilitating retro-translocation of abnormal protein substrates, as well as a toxin, from the ER to the cytosol. This function of torsinA helps to explain the increased sensitivity of cells with loss of or mutant torsinA to ER stress, which may be a factor in neuronal dysfunction underlying abnormal movements in DYT1 carriers41. These data further suggest that increasing levels or function of torsinA to facilitate ERAD degradation of abnormal proteins and thereby alleviate ER stress may have therapeutic benefit. Enhancement of torsinA activity, including increased secretion of a reporter protein and degradation of misfolded proteins, has been achieved using a drug discovered by screening in nematodes54. Thus, given the low penetrance of DYT1 dystonia (30–40%) it may be possible to prevent onset of dystonic symptoms or alleviate their manifestations by treatment with small molecules that increase torsinA function and/or reduce ER stress during the period of susceptibility in children and adolescents.
The following cell lines were used: human embryonic kidney fibroblast line, 293T (from Dr. D. Baltimore; MIT); and two COS cell lines: COS-1 and COS-7 derived from African Green Monkey Kidney cells [from the American Type Culture Collection (ATCC); Manassas, VA]. Primary human skin fibroblasts were established from forearm punch biopsies from controls (HF19, HF74 and HF77, XOB laboratory and L2131, CK laboratory), as well as DYT1 patients (HF49, D2551 and D2306, XOB laboratory) under IRB approved protocols. 293T cells stably expressing TCRalpha-YFP were generated, as described55. Cells were grown in culture, as described10.
Cells were transfected with 0.5 to 1 μg plasmid DNA using Lipofectamine 2000 (for 293T cells) or Lipofectamine Plus reagent (for COS-1 and COS-7 cells) according to instructions of the manufacturer (Invitrogen, Carlsbad, CA) and harvested 48 or 72 h later. In some experiments cells were incubated with 20 μM MG132 (Sigma-Aldrich, St. Louis, MO) for 16 h prior to harvesting or with 5μg/ml tunicamycin.
For adenovirus vector infections, control and patient fibroblasts were plated at a density of 3.5 × 104 cells per well in 6-well plates one day prior to infection. Cells were co-infected with Ad-CMV-CFTRΔF508 and Ad-CMV-EGFP viruses (from the Univ. Penn Vector Core), at multiplicity of infections M.O.I.s of 100 and 25, respectively. To better optimize infection efficiency, cells were spin-infected in Opti-MEM 1X reduced serum media (Gibco, Invitrogen Life Technologies) in the presence of 5 μg/mL hexadimethrine bromide (Sigma-Aldrich). Plates were then centrifuged at 540 x g for 90 min using a TTH-750 high-capacity swing-out rotor in a Sorvall Legend RT benchtop centrifuge (Thermo Fisher Scientific, Agawam, MA). Cells were harvested 24 h after infection and lysates used for protein analysis.
Timed-pregnant C57Bl/6 mice were purchased from Charles River. Cortical neuron cultures were prepared from mouse embryos at embryonic day (E) 15, as described56. Cortical neurons were then grown in complete culture medium with half of the media replaced with fresh media every two days. The cells were treated with 5 μM cytosine arabinoside (Sigma-Aldrich) 4 days after plating and the total media changed after 24 h. Cultures were confirmed to consist predominantly of neurons, as shown by staining of most cells for the early neuronal marker, beta-III tubulin and not the glial marker, GFAP. After 4 days in culture, the neurons were infected with pAAV-CBA-torsinAwt and pAAV-CBA-torsinAΔE (M.O.I. = 50) overnight (CBA refers to the chicken beta-actin promoter). After 72 h, the neurons were stained to visualize endogenous Derlin-1 (1: 300) and torsinA (D-M2A8 1:500), and lysates were used for immunoprecipitation.
293T cells (7 × 106) were plated in a 10 cm plate. After 24 h the cells were transfected with expression cassettes for GFP-CFTRΔF508 or pcDNA (negative control) and pcDNA-torsinAwt using a lipid-based transfection reagent: TransIT-2020, following the protocol of the manufacturer (Mirus Bio, WI). After 24 h transfection, the cells were re-plated in equal amount in 6-well plate. After 1 h cycloheximide was added at a concentration of 100 μg/ml. Cells were collected at 0, 1, 2, 3 and 4 h and were lysed in RIPA buffer containing protease inhibitors. For each time point 250 μg lysate was immunoprecipitated with 4 μl of rabbit GFP antibody and analyzed by western blotting. Total density of CFTR bands was quantified using an ImageJ and rates of degradation were calculated using regression analysis (Microsoft Excel).
293T cell extracts were prepared using Endoplasmic Reticulum Isolation Kit (ER0100, Sigma-Aldrich) following protocol of the manufacturer. Briefly, whole cell extracts were isolated by physical shearing followed by sequential centrifugation using a TTH-750 high-capacity swing-out rotor in a Sorvall Legend RT benchtop centrifuge (Thermo Fisher Scientific) and a TLA 55 rotor in a TL100 ultracentrifuge (Beckman Coulter, Fullerton, CA). The microsomal pellet was solubilized, as described in the immunoprecipitation method (below).
Immunocytochemistry was carried out, as described57. The dilutions of antibodies were: monoclonal anti-RGS-His (1:200), Myc antibodies: 1:500 (polyclonal, Sigma-Aldrich) or 1:300 monoclonal (Invitrogen), torsinA antibodies: 1:1000 (polyclonal TA913) or 1:300 (monoclonal DM2A8), Derlin-1 (polyclonal 1:300), PDI Rabbit 1:300 (SPA-890, Assay designs) and Alexa secondary antibodies 1:1000.
For immunoprecipitations of ERAD components from 293T cells, the microsomal fraction from approximately 106 293T cells was prepared using an ER extraction kit (ER0100, Sigma-Aldrich; as described above). Microsomes were solubilized in 50 mM HEPES, pH 7.4, 200 mM potassium acetate and 10 mM magnesium chloride, with 2.5% digitonin plus protease inhibitor cocktail. This extract was incubated with anti-p97 or anti-IgG as control. The samples were washed 3 times with RIPA lysis buffer and the proteins were subjected to SDS-PAGE and immunoblotted, as described57. For immunoprecipitations of ERAD components in absence of Derlin-1, 293T cells were exposed to a control siRNA (scramble; scr.) or a siRNA targeted to Derlin-1 for 72 h. Cell pellets were treated with digitonin buffer [150 μg/ml digitonin in 50 mM Hepes (pH 7.4)/100 mM KAc/2.5 mM MgAc] to remove cytoplasmic proteins and the remaining membrane fractions were resuspended in RIPA buffer and immunoprecipitated, as above. Samples were resolved by SDS-PAGE and immunoblotted with antibodies to p97, torsinA and Derlin-1.
For immunoprecipitation of ERAD substrate proteins, total cell lysates were resuspended in 1 ml RIPA lysis buffer57 and incubated for 30 min at 4°C. The samples were sonicated briefly (usually for 10 seconds, but for GFP-CFTRΔF508 lysates sonication was carried out 3 times for 10 seconds on ice). Then, samples were centrifuged at 12640 × g at 4°C for 10 min. Supernatant lysates containing 500 μg protein in 1 ml were mixed with antibodies, for example 7 μl each D-M2A8 and D-MG10 (1:1) or 7 μl TAB1 for torsinA, 4 μl polyclonal anti-p97 or 4 μl monoclonal anti-p97, as well as 7 μl goat monoclonal or polyclonal anti-mouse IgG and 3 mg/ml Protein A (Roche Applied Science, Indianapolis, IN) for polyclonal antibodies or Protein G for monoclonal antibodies bound to agarose beads and incubated overnight at 4°C, as described7. For immunoprecipitation of GFP-CFTRΔF508 we used 3 μl polyclonal anti-GFP. The next day, the immunocomplexes were released from beads by boiling, resolved by electrophoresis in 10% SDS-polyacrylamide gels, stained for protein using Ponceau-S (P7170, Sigma-Aldrich) and immunoblotted, as described57.
The lentivirus vector encoding Gluc and the fluorescent protein, cerulean34, was packaged in the NINDS Neuroscience Vector Core. Human fibroblasts were plated in 6-well plates (3.5 × 104 cells/well) and infected with this vector at a M.O.I. of 7 transducing units per cell over 18 h to achieve >90% infection. Infection efficiency was increased by centrifuging cells with vector at 540 x g for 90 min using a TTH-750 high-capacity swing-out rotor in a Sorvall Legend RT benchtop centrifuge (Thermo Fisher Scientific). Forty-eight h after infection, cells were replated in a 96-well plate (2 × 103 cells/well) and 24 h later rinsed with medium and treated with different concentrations of DTT (200290, Thermo Fisher Scientific) or 6-OHDA (H8523, Sigma-Aldrich). Four h later, conditioned medium was assayed for Gluc activity by adding 20 μM coelenterazine (Prolume Ltd./Nanolight, Pinetop, AZ) to an aliquot of the cell-free conditioned medium and acquiring photon counts for 10 sec using a luminometer (Dynex, Richfield, MN).
Statistical analysis was performed using Prism Software (Version 3.0). Results are expressed as mean ± S.E.M. or S.D. (see Figure Legends) and multiple comparison analyses of variance between the groups by two-way ANOVA test. P values were determined using a two-tailed Student’s t-test.
The following methods can be found in the Supplementary Methods: Plasmid expression constructs and antibodies; siRNA; Confocal microscopy; Cholera toxin retro-translocation assays; Nematode experiments.
We thank Nathan Roberts (Dystonia Support Group of Alabama), Nathan Spielberg, Igor Bagayev and Xuan Zhang for help with experiments; Ms. Suzanne McDavitt for skilled editorial assistance; Ms. Trisha Multhaupt-Buell for IRB submissions; Dr. Phyllis Hanson (Wash. U.) for torsinA constructs; Dr. Pedro Gonzalez-Allegre (Univ. Iowa) for torsinA antibodies; Drs. Dinah Sah and Pei Ge (Alnylam Pharmaceuticals) for siRNAs for torsinA; and the Imaging Core of the Harvard Digestive Disease Center DK034854 (WIL) for assistant with confocal imaging. Adenovirus vectors were provided by the Vector Core at the Univ. Penn. Sch. Med.; AAV vectors were provided by Dr. Miguel Sena-Esteves (U. Mass. Med. Ctr.). This work was supported by: NINDS NS037409 (XOB); the Dystonia Medical Research Foundation (FN); NINDS P30NS045776 and NSF CAREER Award (KAC); QRxPharma, Ltd. (KAC, GAC); Volkswagen Fdn. and Hermann and Lilly Schilling Fdn. (CK); HD007466-11, DK083894 and Crohn’s & Colitis Foundation of America 3042 (JAC); and DK48106 and DK0484424 (WIL).
Author contributions – FCN, IAA, JEF, JAC, KAC, GAC, WIL, YY and XOB were involved in conception, organization, execution, statistical analysis and writing of the first draft of this paper. UY, PC, CCH, QW, MT, CK, and BT were involved in execution of experiments, analysis of data and editing of the manuscript.
Competing financial interests: The authors declare no competing financial interest.