The dopamine transporter (DAT) transports extracellular dopamine into the intracellular space contributing to the regulation of dopamine neurotransmission. A reduction of DAT density is implicated in Parkinson’s disease (PD) by neuroimaging; dopamine turnover is dopamine turnover is elevated in early symptomatic PD and in presymptomatic individuals with monogenic mutations causal for parkinsonism. As an integral plasma membrane protein, DAT surface expression is dynamically regulated through endocytic trafficking, enabling flexible control of dopamine signaling in time and space, which in turn critically modulates movement, motivation and learning behavior. Yet the cellular machinery and functional implications of DAT trafficking remain enigmatic. In this review we summarize mechanisms governing DAT trafficking under normal physiological conditions and discuss how PD-linked mutations may disturb DAT homeostasis. We highlight the complexity of DAT trafficking and reveal DAT dysregulation as a common theme in genetic models of parkinsonism.
DAT, a regulator of dopamine neurotransmission and homeostasis
Parkinson’s disease (PD) is the second most common neurodegenerative disease and is best known as a movement disorder. Motor symptoms correlate with the progressive loss of dopaminergic neurons in the substantia nigra and Lewy pathology. However, a relative preservation of dopamine synthesis and an increase in turnover is frequently observed in patients early in their symptom onset1,2,3,4. This supports the hypothesis that dysfunction in presynaptic dopamine neurotransmission may contribute to disease pathogenesis.
Midbrain dopaminergic neurons have a very distinct morphology and mechanism of action. In the rat a single dopaminergic neuron in the substantia nigra is estimated to influence ~75,000 striatal neurons via as many as 370,000 axonal boutons, and in humans the organization may be four times as complex5,6. Dopamine release can originate from varicosities without termination of the axons, from en passant synapses that are often perisynaptic and extrasynaptic. Hence dopamine signaling is not restricted to a single synaptic location but has a large sphere of influence, an architecture that leads to volume transmission7,8. Extracellular dopamine critically modulates movement, motivation and learning by acting on its receptor. Different dopamine receptor subtypes display heterogeneity in their regional expression, substrate affinity and G-protein coupling dynamics9. Depending on the type of receptor activated, dopamine can have completely opposing effects on target neurons. Volume transmission and dopamine receptor heterogeneity both highlight the need to dynamically regulate extracellular dopamine in time and space - a function diligently executed by the dopamine transporter (DAT, SLC6A3).
DAT is a plasma membrane protein selectively expressed in dopaminergic neurons and critically regulates dopamine neurotransmission10,11,12. As a member of SLC6 gene family of Na+/Cl- dependent neurotransmitter transporters, DAT couples the transport of Na+ ions down the electrochemical gradient with the reuptake of extracellular dopamine into the intracellular space. Lowering the concentration of extracellular dopamine limits its duration of action and regulates dopamine transmission. Deletion of the DAT gene in mice greatly reduces tissue dopamine content, despite a great increase in the rate of dopamine synthesis13, suggesting DAT reuptake is the primary mechanism for maintaining intracellular dopamine storage. Beyond simple reuptake of extracellular dopamine, DAT is capable of generating a depolarizing conductance that regulates the excitability of midbrain dopamine neurons both in vitro and in vivo14,15. Under certain conditions, DAT also mediates the release of intracellular dopamine via a reverse transport mechanism known as DAT-mediated dopamine efflux16. Recent studies have also identified DAT as a regulator of short-term plasticity in striatal dopamine release17.
DAT structure and modification
DAT contains twelve transmembrane helices that harbor the primary substrate binding site and have large N- and C- terminals extended into the cytoplasm. DAT undergoes N-linked glycosylation on extracellular loop 2, which is important for surface targeting of the transporter. Pathogenic amino acid substitutions have been described near the Na+ binding site that interfere with conformational changes during transport, resulting in dystonia-parkinsonism, and which highlight the functional significance of this transmembrane domain18,19. Additional rare substitutions have been implicated in attention deficit hyperactivity disorder (ADHD) and autism spectrum disorder (ASD)20,21,22. DAT N- and C- terminals have the most diverse structures among SLC6 family members, and these domains account for differential interaction profiles. Notably, the N-terminus of DAT harbors several secondary modification sites, including residues subject to phosphorylation23 and ubiquitination24, that are important for the activity and trafficking of the transporter. The C-terminus contains domains for interactions with other proteins including α-synuclein25, parkin26, flotillin27 and protein kinase C (PKC)28. Recently, RAS-like GTPase, Rit2 was shown to complex with DAT and regulate PKC-stimulated DAT trafficking29,30. Genetic variability in the Rit2 locus has been robustly associated with PD and several other dopaminergic disorders29,31,32.
The high-resolution crystal structure of human DAT (hDAT) has not been solved as it is lipid associated and the protein aggregates during purification. Nevertheless, recent studies have resolved a partial structure of Drosophila melanogaster DAT (dDAT) in multiple conformational states. Hence, the functional dynamics of DAT and its interactions with ligands are being elucidated33. At resting state, dDAT exists in an open and outward facing conformation. Upon substrate binding, an outward facing occluded conformation forms that is stabilized by salt bridges between key residues (the extracellular gate). Then the occluded complex transitions to become inward facing. Subsequent disruption of a separate set of salt bridges (the intracellular gate) allows substrate release into the intracellular space. Mutations that disrupt the conformational structure often lead to anomalous efflux or inefficient uptake activity20,21,22. However, it should be noted that dDAT intracellular N- and C- termini were removed to facilitate crystallization. In addition, dDAT was crystallized as a monomer34, whereas biochemical and microscopy data frequently detect dimers, oligomers and clusters of DAT molecules in DAT expressing model systems35,36,37,38,39,40,41. Oligomerization could influence DAT trafficking and surface expression. Small molecules, notably AIM100, may directly induce DAT oligomerization and subsequent endocytosis42. Readers are referred to the recent review for more detailed discussion on DAT oligomerization43.
Regulation of DAT endocytosis
Plasma membrane dopamine transporters are dynamically regulated by endocytic trafficking. Extensive studies have identified a variety of signaling pathways that lead to DAT internalization. The mechanisms of endocytic carrier formation and post-endocytic sorting of DAT largely depends on the signaling context. In this section, the mechanisms underlying DAT endocytosis are reviewed.
Clathrin-mediated endocytosis (CME) was the first mechanism identified for DAT regulation and is best characterized by PKC activation44,45, which robustly drives the loss of surface DAT in heterologous systems and striatal tissues46. New data suggests PKC activation may disrupt DAT interactions with Rit2, and with cytosolic nonreceptor tyrosine kinase (TNK2, formerly called activated p21CDC42 kinase; ACK1), that normally stabilize DAT in the plasma membrane30,47. AIM-100 may also inhibit TNK2 and lower surface DAT47,48. The effect of PKC can be arrested by blocking CME. For example, dynamin interacts with clathrin-coated pits and plays an important role in vesicle budding. Expression of dynamin p.K33E, a dominant-negative form of dynamin, or pharmacological inhibition of dynamin activity prevents phorbol 12-myristate 13-acetate (PMA)-induced loss of surface DAT in cell lines and ex-vivo striatal slices, respectively45,49. Down regulation of clathrin heavy chain by siRNA or acute inhibition of clathrin function by pitstop2 prevents PMA-mediated DAT internalization in DAT expressing cell lines44,47,50. However, dynamin is involved in both clathrin-dependent and clathrin-independent pathways including RhoA- and caveolar-mediated endocytosis51. Clathrin is also critically involved in a broad range of endocytic pathways including sorting of ubiquitinated proteins for lysosomal degradation52,53. Therefore, indirect regulation of clathrin and dynamin on PKC-mediated DAT internalization cannot be excluded. DAT complexes with Eps15, a component of clathrin-coated pits, in heterologous systems and midbrain neuronal cultures24,50. However, immunogold-labeling has failed to observed DAT localization in clathrin-coated pits in the axonal terminals and soma of dopaminergic neurons54,55,56. Assessing DAT’s interaction with clathrin and scaffold proteins, such as adaptor protein-2, in endogenously expressing systems may further clarify their role in DAT endocytosis.
RhoA-mediated Clathrin-independent Endocytosis
RhoA belongs to the Ras GTPase family and defines a clathrin-independent endocytic pathway57. RhoA-mediated DAT endocytosis is most studied in the context of substrate exposure including amphetamine (AMPH); AMPH-induced DAT internalization was first described in HEK293 cells58, and later confirmed in mid-brain neuronal cultures59, ex-vivo striatal and mid-brain slices46,59. AMPH-mediated DAT endocytosis is dynamin dependent58, accompanied by the activation of RhoA and Rac1 in mouse mid-brain slices, and prevented by the inhibition of RhoA through PKA59. Similarly, dopamine treatment of rat mid-brain slices also increases RhoA activation and reduces surface DAT expression, and such effects are inhibited by pharmacological activation of the PKA-coupled D1 receptor60. AMPH and dopamine-mediated DAT internalization is blocked by cocaine which occupies the substrate binding site of DAT and prevents transport activity14,16,58,59. Extracellular AMPH failed to induce internalization of an uptake-impaired mutant form of DAT (Y335A-hDAT); whereas direct intracellular application of AMPH via a whole cell patch pipette restored the trafficking of Y335A-hDAT, and revealed that its endocytic regulation is triggered by intracellular AMPH61. Subsequent study has identified the G-protein coupled receptor (GPCR) TAAR1 as the intracellular effector of AMPH-mediated RhoA activation and DAT endocytosis62.
An essential downstream effector of RhoA activation is Arp2/3, which directly regulates actin branching and polymerization to provide the necessary force for membrane remodeling in the absence of clathrin63,64 and highlights the role of actin dynamics in DAT trafficking. Actin depolymerization agents lead to reduced DAT surface expression in striatal tissue49. Piccolo, a component of the presynaptic cytoskeletal matrix, was shown to negatively regulate methamphetamine-induced DAT internalization, possibly through sequestering membrane phosphatidylinositol 4,5-bisphosphate (PIP2)65.
Lipid raft and DAT surface retention
Lipid rafts are cholesterol- and sphingolipid-enriched microdomains on the plasma membrane. DAT is proposed to distribute equally among raft and non-raft domains49,66. Although it is generally acknowledged that DAT association with lipid rafts negatively regulates the kinetics of the transporter activity67,68 and membrane mobility27,50,69, the role of lipid rafts on DAT endocytosis is controversial. While some studies report raft-associated DAT exhibits more resistance to constitutive and PKC mediated endocytosis66, others show DAT endocytosis arises equally from raft and non-raft associated populations49. DAT forms a stable protein complex with membrane protein flotillin-1, and that interaction appears to be required for DAT targeting to lipid rafts27,50. siRNA mediated flotillin-1 knock down may block PMA-mediated DAT endocytosis in heterologous systems and mid-brain dopaminergic neuronal cultures27. Paradoxically, in an independent study, the same treatment did not exhibit any effect in PMA-treated HA-DAT expressing cells50. Lipid rafts provide a scaffold for plasma membrane protein interactions with the cytoskeleton and promote DAT clustering40. It is possible that flotillin facilitates endocytosis by promoting DAT clustering prior to carrier formation, rather than being directly involved in carrier formation, as shown for other cargos70,71. However, the conflicting results might be due to the model system used to study raft and non-raft associated DAT trafficking. Future studies might directly examine the trafficking routes of DAT-flotillin complexes in mid-brain dopaminergic neurons expressing DAT endogenously.
DAT post-endocytic sorting
In general, degradative and recycling pathways are physically separated by distinct endosomal subdomains, and defined by their respective sorting machineries72. The endosomal sorting complexes required for transport (ESCRT) family of proteins defines degradative subdomains73 and orchestrates the recruitment of ubiquitinated cargos to budding intraluminal vesicles. Conversely, tubular extensions occupy most of the membrane surface and provide subdomains enriched in cargo retrieval complexes, including the retromer and retriever complexes. These generate tubulo-vesicles for plasma membrane recycling or retrograde transport to the Golgi network74,75,76. Extensive efforts have been invested to identify the subcellular localization of internalized DAT, to define its post-endocytic fate. However, the ambiguous colocalization pattern of DAT with known post-endocytic sorting markers, and lack of methodology to reliably track endogenous DAT have led to conflicting results, as reviewed below.
Although the field cannot reach a consensus on the exact post-endocytic fate of DAT, most studies provide evidence that DAT is, at least in part, targeted for lysosomal degradation following endocytosis. Studies using either antibody feeding assays or fluorescent cocaine analogs to visualize epitope-tagged or endogenous DAT in mid-brain neuronal cultures all confirm that internalized DAT partially localizes to late endosomes and lysosomes77,78,79,80,81. Electron microscopy studies also show that DAT localizes to the endolysosomal compartment, albeit less in axonal terminals than in soma54,55,56.
N-terminal ubiquitination may be the tag that sorts DAT to its degradative fate. DAT undergoes ubiquitylation on conserved lysine residues in heterologous systems and mid-brain neuronal cultures, which is significantly enhanced following PMA treatment79,82,83. Nedd4–2 has been identified to ubiquitinate DAT in a PKC dependent manner24. Either down regulation of Nedd4-2 or abolition of DAT N’-terminal lysines by mutagenesis impairs the PKC-mediated endocytosis of DAT24,83. However, Nedd4 regulates the trafficking and degradation of many membrane proteins so disruption of DAT trafficking could be a secondary consequence rather than a direct effect.
Interestingly, DAT is proposed to undergo monoubiquitylation and lys63-linked polyubiquitylation82,83,84, both of which serve to target cargos to a degradative fate by recruiting cargo to ESCRT-positive subdomains85. Supporting the theory, DAT localization to the ESCRT component ‘hepatocyte growth factor-regulated tyrosine kinase substrate (HRS)-positive’ endosomal compartment was also confirmed in PMA treated YFP-DAT expressing cells83. Conversely, modification that reduces DAT ubiquitination also reduces degradation and enhances DAT’s steady state level86. Collectively, these studies support the model where PKC-mediated ubiquitination recruits DAT to a degradative fate.
However, attempts to validate PKC-mediated degradation for endogenous DAT have proven challenging as multiple groups report PMA treatment fails to induce DAT internalization in mid-brain neuronal cultures77,80,81. Although PKC-induced loss of surface DAT can be robustly reproduced using a biotinylation assay of ex-vivo striatal and mid-brain slices, the total level of DAT is not significantly reduced compared to heterologous systems27,30,49. Conflicting results may be due to differences in PMA treatment times and/or use of heterologous model systems overexpressing DAT. More research is needed to validate DAT ubiquitination and subcellular localization in its native environments, including the soma and terminal regions of dopamine neurons.
Endocytic recycling pathways for DAT also remain elusive. Early electron microscopy (EM) studies in rodent brains observed DAT immunoreactivity in tubulovesicular structures in the soma, albeit less frequently in axonal varicosities, suggesting DAT may be subject to endocytic recycling55,56. Although DAT exhibits partial colocalization with recycling markers, such as syntaxin13, the transferrin receptor and Rab11, in cultured mid-brain neurons and in ex-vivo slices, the extent of that colocalization is quite ambiguous compared to bona fide recycling cargos such as transferrin and β2-adrenergic receptors77,80. Direct comparison between the trafficking of DAT and norepinephrine transporter (NET, a SLC6 family transporter closely related to DAT) shows that NET is more likely to recycle via Rab11 than DAT, due to the non-conserved N’-termini of the two transporters48. However, in N2A neuroblastoma cells, expression of dominant-active Rab11 upregulates DAT surface expression and uptake activity87. Multiple groups have also demonstrated DAT plasma membrane recycling with antibody feeding or biotinylation based assays in various cell lines and mid-brain neuronal cultures79,88,89. In support of its recycling fate, DAT was shown localize to VPS35 positive vesicles in dopaminergic cell lines and dopamine axons in mouse medial forebrain bundle axons89,90. Either knocking down or expression of PD-linked mutant Vps35 p.D620N leads to reduced total and surface expression of DAT in heterologous systems and mouse striatal tissues89,91, albeit without producing a PD-like motor phenotypes in this animal model91. Internalized DAT that undergoes retromer-mediated plasma membrane recycling or retrograde trafficking may potentially account for the comparatively decreased colocalization between DAT and Rab11.
The retromer complex orchestrates sequence-dependent cargo retrieval as opposed to sequence-independent bulk recycling92,93. However, the sequence responsible for DAT-retromer interaction remains to be determined. The PDZ domain is a well characterized recycling sequence recognized by retromer and its adaptor protein for plasma membrane recycling92. The same mechanism is proposed to regulate retromer-mediated recycling of DAT89. Indeed, mice harboring mutations in the putative PDZ domain of DAT exhibit reduced surface DAT expression in the striatum94. Furthermore, the DAT PDZ motif was required, at least partially, for exit out of retromer-positive endosomes89. However, unlike well-characterized retromer cargos such as beta 2 adrenergic receptor (β2AR) or glucose transporter1 (GLUT1)95,96,97 which have a type I PDZ domain, DAT has a type II PDZ domain. This is unlikely to be recognized by SNX27, the adaptor protein best characterized in retromer-mediated plasma membrane recycling98,99. Retromer binding is sometimes facilitated by palmitoylation of cysteine residues in the cytosolic tails of cargo proteins100, and notably, DAT undergoes C’-terminal cysteine palmitoylation101. Pharmacological inhibition or mutagenesis of those cysteine residues enhances PMA-induced downregulation of DAT in heterologous cells and rat striatal synaptosomes, suggesting palmitoylation may function to resist PKC-mediated DAT degradation101. The functional impact of palmitoylation on dopamine reuptake kinetics of surface DAT is well described102, but whether palmitoylation affects DAT endocytic sorting and trafficking is unknown.
DAT axonal targeting
Another puzzle in DAT trafficking is the mechanism of DAT axonal targeting. Midbrain dopaminergic neurons project long and extensively arborized terminals5. In rat a single dopaminergic neuron in the substantia nigra is estimated to influence ~75,000 striatal neurons5, via as many as 370,000 terminal axonal boutons6. DAT is found throughout the plasma membrane of the axons and varicosities of dopaminergic neurons54,55,56. It seems intuitive that with such a complex morphology, dopaminergic neurons might employ local DAT synthesis rather than long-range axonal trafficking. Surprisingly, the in-situ hybridization signal for DAT mRNA is primarily observed in the mid-brain and almost invisible in the striatum103,104, although that may reflect the probes used and the sensitivity of traditional in-situ methods. It remains possible that DAT mRNA may be found outside of the somatodendritic compartment. At the protein level, most DAT localizes to smooth endoplasmic reticulum in the soma and not in axonal terminals54,55,56. In mid-brain neuronal cultures from tagged HA-DAT knock-in mice, HA-DAT vesicles display rapid bi-directional movement along axons suggesting that DAT is synthesized in somal endoplasmic reticulum (ER) and subject to axonal trafficking. A recent study examined long-range DAT trafficking in medial forebrain bundle axonal tracts to reveal that most DAT is membrane localized with a more limited distribution in retromer positive vesicles90. The result raised the possibility that DAT might be trafficked by both membrane diffusion and vesicular transport90. Future studies examining DAT localization to microtubule markers and/or microtubule motor proteins such as kinesin would further clarify the mechanism of long-range DAT trafficking.
ER export relies heavily on coated-protein complex (COPII) coat-derived vesicles with SEC24 family proteins orchestrating cargo recognition105. Supporting the role of SEC24-mediated ER export in DAT axonal targeting, siRNA knockdown against SEC24D in heterologous cell lines slows down dopamine reuptake106. In C.elegans, deletion or mutagenesis of a conserved sequence 591PYRKR595 in the DAT-1 C′-terminus leads to somatic retention107. The PYRKR sequence contains a 3 R motif that mediates the interaction between SEC24 and α2β-adrenergic receptor107,108, suggesting the failure of DAT-1 synaptic localization might be due to reduced interaction with SEC24-1. In HEK293 cells, mutation of the corresponding sequence in DAT does not affect its interaction with SEC24D, nor significantly reduces DAT surface expression, but does disrupt the ability of SEC24D to enhance DAT surface expression107. However, HEK293 cells are not going to be an informative model for DAT axonal trafficking as they lack the bipolar morphology of dopaminergic neurons.
In conclusion, multiple molecular mechanisms are implicated in DAT trafficking and the specific trafficking route is highly dependent on signaling. Key mechanisms are summarized in Fig. 1. DAT trafficking studies have suffered from a lack of reagents to reliably track DAT in its native environment, and work conducted in heterologous systems had often produced conflicting results. More recent super-resolution microscopy has revealed the dynamic localization of neuronal transmembrane proteins, including DAT40,109,110, and may prove useful to dissect mechanisms governing endogenous DAT trafficking in bona fide dopaminergic terminals.
The dopamine transporter, monogenic parkinsonism, and models
Given the complex morphology of dopaminergic neurons and the onerous burden of long-term axonal trafficking, it is tempting to speculate that endocytic dysregulation of the dopaminergic transporter may lead to the selective vulnerability of dopaminergic neurons in PD. In this section, monogenic parkinsonism, and models based on those gene linkages are reviewed, albeit focused on their DAT biology. Most mice that model human gene mutations linked to PD do not exhibit overt motor symptoms but many have subtle alterations to their dopaminergic system, as illustrated in Table 1.
α-synuclein (SNCA) is a presynaptic protein and a major component of Lewy pathology. Studies of familial forms of Parkinson’s disease have identified SNCA missense mutations and genomic multiplications111. Mice models overexpressing mutant or wild type human α-synuclein mostly exhibit reduced DAT expression and dopamine reuptake112,113,114,115,116 with some exceptions117. α-synuclein may form a stable complex with DAT in heterologous systems, rodent and human striatal tissues25,118,119. Studies in dopaminergic neuronal cultures suggest DAT/α-synuclein association negatively regulates DAT reuptake activity120,121,122 possibly by redistributing surface DAT to cholesterol-rich microdomains and altering ionic coupling of DAT mediated current120,121. DAT surface expression, measured by biotinylation, is also reduced with co-expression of wild type α-synuclein123,124. When compared to wild type α-synuclein, the PD-linked missense mutation SNCA p.A30P enhances DAT α-synuclein interaction and further reduces DAT surface expression and function; in contrast, p.A53T does not form a strong protein-protein complex with DAT, nor modulates DAT function or surface expression. Although SNCA p.A30P and p.A53T have disparate effects on DAT-binding and trafficking, they are N’-terminal located on the hydrophobic face of α-synuclein’s amphipathic helix, highlighting the importance of maintaining that protein-lipid interaction.
Leucine-rich repeat kinase 2 (LRRK2), encodes a large multidomain protein containing kinase and GTPase enzymatic activities. LRRK2 genetic variability is found throughout the gene but pathogenic mutations cluster in the Roc-COR and kinase domains, and account for this common form of familial parkinsonism111. All mutations lead to upregulation of LRRK2 kinase activity. Investigations of in vivo dopaminergic function with PET imaging consistently reveal increased dopamine turnover rates in asymptomatic LRRK2 heterozygotes1,2,125. Interestingly, those asymptomatic individuals showed reduced DAT levels, measured by the commonly used PET tracer 11C-d-threo-methylphenidate (11C-MP)125, suggesting early dysfunction of DAT in the absence of significant loss of dopamine synthesis and storage. In rodent models, temporal overexpression of human LRRK2 p.G2019S in dopaminergic neurons impairs DAT mediated dopamine reuptake126. Constitutive Lrrk2 p.G2019S knock-in mice also exhibit impairment in striatal dopamine reuptake at various ages127,128. Although there are limited number of studies that directly examine the role of LRRK2 in DAT regulation, growing evidence has established LRRK2 as an important regulator of intracellular membrane trafficking129, at a nexus between actin-dependent and tubulin-dependent cargo transport130,131,132. Mutant LRRK2 leads to dysregulated endocytic sorting133 through phosphorylation of Rab proteins134,135 whose coordinated action critically regulates vesicular transport and endosome maturation136,137. LRRK2 binding to microtubules is also associated with tau phosphorylation138,139, microtubule acetylation132,140 and impaired axonal transport132. Hence, DAT endosomal recycling and axonal trafficking may be dysregulated by chronic LRRK2 hyperactivity. Exploring the increased (or compensatory) dopamine turnover observed in asymptomatic LRRK2 heterozygous individuals may provide mechanistic insight into the physiological and pathological role of LRRK2 in DAT regulation.
VPS35 is a component of the retromer complex required for recycling cargo protein in the early endosome to the trans-Golgi network or plasma membrane76. A missense mutation, VPS35 p.D620N has been linked to a familial form of parkinsonism that is clinically indistinguishable from idiopathic late-onset PD141,142. VPS35 colocalizes with DAT and mediates DAT plasma membrane recycling both in vitro and in vivo89. Mice harboring Vps35 p.D620N exhibit reduced striatal DAT expression and altered striatal dopamine neurotransmission in the absence of motor deficits or neurodegeneration91. Although the exact pathological mechanism of VPS35 p.D620N remains elusive, multiple studies show the mutation disrupts the interaction between VPS35 and the WASH complex143,144 whose primary function is to coordinate actin branching and stabilize endosomal subdomains for VPS35-mediated cargo sorting of recycling proteins145. Failure to adequately recruit or retain WASH complex may lead to the mis-sorting of DAT, as illustrated by other retromer cargos143,145,146. These data are consistent with the hypothesis that expression of VPS35 p.D620N can impair DAT recruitment and recycling.
Increasing evidence suggests that VPS35 and LRRK2 functionally interact and converge on endocytic trafficking. VPS35 and LRRK2 directly interact, decorate endosomes, and may work in concert in synaptic vesicle recycling147. VPS35 p.D620N significantly elevates LRRK2-mediated phosphorylation of Rab proteins in mouse brain and human neutrophils148. Endolysosomal dysfunction induced by mutant LRRK2 can be rescued by overexpression of VPS35149, although toxic to synapses in primary culture96. Given VPS35 and LRRK2 mouse models exhibit similar deficits in DAT mediated reuptake, it is possible that they also cooperate in the regulation of DAT trafficking. Interestingly, acute treatment with the LRRK2 kinase inhibitor, MLi2, in Vps35 p.D620N knock-in mice rescues the reduction in striatal DAT levels and the reduction in dopamine reuptake91 (Farrer lab, unpublished data). However, it is currently unknown which step in DAT trafficking (e.g., endocytosis, endocytic sorting, axonal targeting) is involved and whether VPS35 and LRRK2 work in concert or in competition.
Parkin is a protein-ubiquitin E3 ligase which ubiquitinates and targets substrate to proteasome degradation150. Mutations in Parkin lead to loss of function of its ubiquitin ligase activity and are linked to autosomal recessively inherited, early-onset Parkinson’s disease with a central role in mitophagy151. However, patients with mutations in Parkin often exhibit a marked reduction of DAT expression or uptake activity152,153. DAT ubiquitination was previously shown to be increased in Parkin transfected human dopaminergic SH-SY5Y cells26. WT Parkin, but not PD-linked mutants, significantly increase DAT surface expression and dopamine reuptake, and possibly enhance degradation of misfolded DAT26. An association between Parkin and DAT has also been shown to disrupt the interaction between DAT and α-synculein154; however, further validation using a more sensitive approach, such as Förster resonance energy transfer (FRET) or yeast 2-hybrid methods, is warranted. Parkin is reported to ubiquitinate Rab7, Eps15, and VPS35 and so contributes to the regulation of the endo-lysosomal pathway155,156,157. Parkin knock-out mice exhibit reduced striatal levels of DAT and dopamine uptake158,159. In patient-derived IPSCs, loss of Parkin function also leads to reduced [3H]CFT (2-β-carbomethoxy-3-β-(4-fluorophenyl)tropane, a cocaine analog) binding to DAT and increased Ca2+-independent dopamine release, potentially via a reverse transport mechanism160. Several studies support the hypothesis in which loss of parkin function reduces DAT activity either directly, through impaired protein quality control, or indirectly through dysregulation of DAT endocytic trafficking.
RIT2 was identified as a PD risk gene in multiple GWAS studies and in different ethnic groups31,32,161,162,163,164, and Rit2 expression is significantly reduced in the substantia nigra of PD patients165. Rit2 encodes a small neuronal GTPase that associates with DAT and may act as DAT endocytic brake30. Studies in heterologous systems reveal RIT2 associates with the C-terminus of DAT, but not SERT, and that RIT2 GTPase activity is critical for PKC-mediated DAT internalization29. Although Rit2 was shown to co-immunoprecipitate with DAT in mouse striatum29 this result appears to be an artifact as the antibody used was unspecific30. Nevertheless, the effects of Rit2 in bona fide dopaminergic terminals are confirmed in mouse striatal slices30,46. In Pitx3IRES2-tTA shRit2 mice, where Rit2 is selectively knockdown in dopaminergic neurons, PKC-stimulated DAT internalization in acute striatal slices is significantly reduced30. Interestingly, Pitx3IRES2-tTA shRit2 mice exhibit sex-dimorphism in dopamine related phenotypes166. Conditional Rit2 knockout leads to a blunted response to acute cocaine treatment in female mice, but an increased response in males166. Accordingly, [3H] dopamine uptake in male striatal slices is enhanced without significant change in surface DAT expression166, whereas in females surface DAT is reduced in the ventral striatum30. Considering the important role of sex in DAT function and PD risk167,168,169,170,171,172, RIT2 poses a promising target to study the effect of sexual dimorphism in DAT regulation and in the etiology of PD.
A variety of signaling pathways have been identified that dynamically regulate dopamine reuptake through DAT plasma membrane trafficking, and many overlap with key molecular mechanisms compromised by PD-linked mutations as illustrated in Fig. 2. Down regulation of DAT-mediated dopamine reuptake and increase in striatal dopamine release are often observed in genetic models of parkinsonism. Why would the neurons employ so many complicated signaling pathways to regulate DAT trafficking? DAT critically maintains dopamine homeostasis to regulate dopamine signaling that is absolutely required for movement initiation and survival. Cytosolic dopamine is also easily oxidized, may lead to the production of free radicals, and drives neuromelanin biosynthesis173. Direct administration of dopamine and overexpression of dopamine transporter both lead to neuronal loss174,175. Conversely, dopamine reuptake by DAT is the primary mechanism for the maintenance of dopamine storage, and loss of DAT leads to dopamine depletion13. The depolarizing currents generated by dopamine reuptake also directly regulate the excitability of presynaptic boutons15. Thus, DAT surface expression must be controlled to allow dopaminergic neurons to optimally function. The complexities of DAT regulation may enable multiple compensatory mechanisms to maintain dopamine signaling despite early dysfunction. Given the role of DAT in the regulation of dopamine release and the long-hypothesized connection between altered dopamine neurotransmission and PD, studies of DAT regulation in physiological and pathological conditions remain a promising avenue to identify early biomarkers and therapeutic targets for PD.
Wile, D. J. et al. Serotonin and dopamine transporter PET changes in the premotor phase of LRRK2 parkinsonism: cross-sectional studies. Lancet Neurol. 16, 351–359 (2017).
Sossi, V. et al. Dopamine turnover increases in asymptomatic LRRK2 mutations carriers. Mov. Disord. 25, 2717–2723 (2010).
Lee, C. S. et al. In vivo positron emission tomographic evidence for compensatory changes in presynaptic dopaminergic nerve terminals in Parkinson’s disease. Ann. Neurol. 47, 493–503 (2000).
Sossi, V. et al. Increase in dopamine turnover occurs early in Parkinson’s disease: evidence from a new modeling approach to PET 18F-fluorodopa data. J. Cereb. Blood Flow. Metab. 22, 232–239 (2002).
Matsuda, W. et al. Single nigrostriatal dopaminergic neurons form widely spread and highly dense axonal arborizations in the neostriatum. J. Neurosci. 29, 444–453 (2009).
Arbuthnott, G. W. & Wickens, J. Space, time and dopamine. Trends Neurosci. 30, 62–69 (2007).
Rice, M. E. & Cragg, S. J. Dopamine spillover after quantal release: rethinking dopamine transmission in the nigrostriatal pathway. Brain Res. Rev. 58, 303–313 (2008).
Cragg, S. J. & Rice, M. E. DAncing past the DAT at a DA synapse. Trends Neurosci. 27, 270–277 (2004).
Andersen, P. H. et al. Dopamine receptor subtypes: beyond the D1/D2 classification. Trends Pharmacol. Sci. 11, 231–236 (1990).
Ciliax, B. J. et al. Immunocytochemical localization of the dopamine transporter in human brain. J. Comp. Neurol. 409, 38–56 (1999).
Ciliax, B. J. et al. The dopamine transporter: Immunochemical characterization and localization in brain. J. Neurosci. 15, 1714–1723 (1995).
Shimada, S., Kitayama, S., Walther, D. & Uhl, G. Dopamine transporter mRNA: dense expression in ventral midbrain neurons. Mol. Brain Res. 13, 359–362 (1992).
Jones, S. R. et al. Profound neuronal plasticity in response to inactivation of the dopamine transporter. Proc. Natl Acad. Sci. USA 95, 4029–4034 (1998).
Ingram, S. L., Prasad, B. M. & Amara, S. G. Dopamine transporter-mediated conductances increase excitability of midbrain dopamine neurons. Nat. Neurosci. 5, 971–978 (2002).
Carvelli, L., McDonald, P. W., Blakely, R. D. & DeFelice, L. J. Dopamine transporters depolarize neurons by a channel mechanism. Proc. Natl Acad. Sci. USA 101, 16046–16051 (2004).
Kahlig, K. M. et al. Amphetamine induces dopamine efflux through a dopamine transporter channel. Proc. Natl Acad. Sci. USA 102, 3495–3500 (2005).
Condon, M. D. et al. Plasticity in striatal dopamine release is governed by release-independent depression and the dopamine transporter. Nat. Commun. 10, 1–15 (2019).
Kurian, M. A. et al. Homozygous loss-of-function mutations in the gene encoding the dopamine transporter are associated with infantile parkinsonism-dystonia. J. Clin. Invest. 119, 1595–1603 (2009).
Hansen, F. H. et al. Missense dopamine transporter mutations associate with adult parkinsonism and ADHD. J. Clin. Invest. 124, 3107–3120 (2014).
DiCarlo, G. E. et al. Autism-linked dopamine transporter mutation alters striatal dopamine neurotransmission and dopamine-dependent behaviors. J. Clin. Invest. 129, 3407–3419 (2019).
Mazei-Robison, M. S. et al. Anomalous dopamine release associated with a human dopamine transporter coding variant. J. Neurosci. 28, 7040–7046 (2008).
Mazei-Robison, M. S., Couch, R. S., Shelton, R. C., Stein, M. A. & Blakely, R. D. Sequence variation in the human dopamine transporter gene in children with attention deficit hyperactivity disorder. Neuropharmacology 49, 724–736 (2005).
Foster, J. D., Cervinski, M. A., Gorentla, B. K. & Vaughan, R. A. Regulation of the dopamine transporter by phosphorylation. Handb. Exp. Pharmacol. 175, 197–214 (2006).
Sorkina, T. et al. RNA interference screen reveals an essential role of Nedd4-2 in dopamine transporter ubiquitination and endocytosis. J. Neurosci. 26, 8195–8205 (2006).
Lee, F. J. S., Liu, F., Pristupa, Z. B. & Niznik, H. B. Direct binding and functional coupling of α‐synuclein to the dopamine transporters accelerate dopamine‐induced apoptosis. FASEB J. 15, 916–926 (2001).
Jiang, H., Jiang, Q. & Feng, J. Parkin increases dopamine uptake by enhancing the cell surface expression of dopamine transporter. J. Biol. Chem. 279, 54380–54386 (2004).
Cremona, M. L. et al. Flotillin-1 is essential for PKC-triggered endocytosis and membrane microdomain localization of DAT. Nat. Neurosci. 14, 469–477 (2011).
Vaughan, R. A. & Foster, J. D. Mechanisms of dopamine transporter regulation in normal and disease states. Trends Pharmacol. Sci. 34, 489–496 (2013).
Navaroli, D. M. et al. The plasma membrane-associated gtpase rin interacts with the dopamine transporter and is required for protein kinase c-regulated dopamine transporter trafficking. J. Neurosci. 31, 13758–13770 (2011).
Fagan, R. R. et al. Dopamine transporter trafficking and Rit2 GTPase: Mechanism of action and in vivo impact. J. Biol. Chem. 295, 5229–5244 (2020).
Foo, J. N. et al. Genome-wide association study of Parkinson’s disease in East Asians. Hum. Mol. Genet. 26, 226–232 (2017).
Pankratz, N. et al. Meta-analysis of Parkinson’s Disease: Identification of a novel locus, RIT2. Ann. Neurol. 71, 370–384 (2012).
Cheng, M. H. & Bahar, I. Monoamine transporters: structure, intrinsic dynamics and allosteric regulation. Nat. Struct. Mol. Biol. 26, 545–556 (2019).
Penmatsa, A., Wang, K. H. & Gouaux, E. X-ray structure of dopamine transporter elucidates antidepressant mechanism. Nature 503, 85–90 (2013).
Hastrup, H., Karlin, A. & Javitch, J. A. Symmetrical dimer of the human dopamine transporter revealed by cross-linking Cys-306 at the extracellular end of the sixth transmembrane segment. Proc. Natl Acad. Sci. USA 98, 10055–10060 (2001).
Hastrup, H., Sen, N. & Javitch, J. A. The human dopamine transporter forms a tetramer in the plasma membrane: Cross-linking of a cysteine in the fourth transmembrane segment is sensitive to cocaine analogs. J. Biol. Chem. 278, 45045–45048 (2003).
Sorkina, T., Doolen, S., Galperin, E., Zahniser, N. R. & Sorkin, A. Oligomerization of dopamine transporters visualized in living cells by fluorescence resonance energy transfer microscopy. J. Biol. Chem. 278, 28274–28283 (2003).
Chen, N. & Reith, M. E. A. Substrates dissociate dopamine transporter oligomers. J. Neurochem. 105, 910–920 (2008).
Zhen, J. et al. Dopamine transporter oligomerization: Impact of combining protomers with differential cocaine analog binding affinities. J. Neurochem. 133, 167–173 (2015).
Rahbek-Clemmensen, T. et al. Super-resolution microscopy reveals functional organization of dopamine transporters into cholesterol and neuronal activity-dependent nanodomains. Nat. Commun. 8, 1–14 (2017).
Das, A. K. et al. Dopamine transporter forms stable dimers in the live cell plasma membrane in a phosphatidylinositol 4,5-bisphosphate independent manner. J. Biol. Chem. 294, 5632–5642 (2019).
Sorkina, T., Ma, S., Larsen, M. B., Watkins, S. C. & Sorkin, A. Small molecule induced oligomerization, clustering and clathrin-independent endocytosis of the dopamine transporter. Elife 7, e32293 (2018).
Jayaraman, K. et al. SLC6 transporter oligomerization. J. Neurochem, (2020), https://doi.org/10.1111/jnc.15145.
Sorkina, T., Hoover, B. R., Zahniser, N. R. & Sorkin, A. Constitutive and protein kinase C-induced internalization of the dopamine transporter is mediated by a clathrin-dependent mechanism. Traffic 6, 157–170 (2005).
Daniels, G. M. & Amara, S. G. Regulated trafficking of the human dopamine transporter. Clathrin-mediated internalization and lysosomal degradation in response to phorbol esters. J. Biol. Chem. 274, 35794–35801 (1999).
Fagan, R. R., Kearney, P. J. & Melikian, H. E. In situ regulated dopamine transporter trafficking: there’s no place like home. Neurochem. Res. 45, 1335–1343 (2020).
Wu, S., Bellve, K. D., Fogarty, K. E. & Melikian, H. E. Ack1 is a dopamine transporter endocytic brake that rescues a trafficking-dysregulated ADHD coding variant. Proc. Natl Acad. Sci. USA 112, 15480–15485 (2015).
Vuorenpää, A. et al. Differential internalization rates and postendocytic sorting of the norepinephrine and dopamine transporters are controlled by structural elements in the N termini. J. Biol. Chem. 291, 5634–5651 (2016).
Gabrie, L. R. et al. Dopamine transporter endocytic trafficking in striatal dopaminergic neurons: Differential dependence on dynamin and the actin cytoskeleton. J. Neurosci. 33, 17836–17846 (2013).
Sorkina, T., Caltagarone, J. & Sorkin, A. Flotillins regulate membrane mobility of the dopamine transporter but are not required for its protein kinase C dependent endocytosis. Traffic 14, 709–724 (2013).
Mayor, S., Parton, R. G. & Donaldson, J. G. Clathrin-independent pathways of endocytosis. Cold Spring Harb. Perspect. Biol. 6, a016758 (2014).
Sachse, M., Urbé, S., Oorschot, V., Strous, G. J. & Klumperman, J. Bilayered clathrin coats on endosomal vacuoles are involved in protein sorting toward lysosomes. Mol. Biol. Cell 13, 1313–1328 (2002).
Raiborg, C., Wesche, J., Malerød, L. & Stenmark, H. Flat clathrin coats on endosomes mediate degradative protein sorting by scaffolding Hrs in dynamic microdomains. J. Cell Sci. 119, 2414–2424 (2006).
Block, E. R. et al. Brain region-specific trafficking of the dopamine transporter. J. Neurosci. 35, 12845–12858 (2015).
Nirenberg, M. J., Vaughan, R. A., Uhl, G. R., Kuhar, M. J. & Pickel, V. M. The dopamine transporter is localized to dendritic and axonal plasma membranes of nigrostriatal dopaminergic neurons. J. Neurosci. 16, 436–447 (1996).
Hersch, S. M., Yi, H., Heilman, C. J., Edwards, R. H. & Levey, A. I. Subcellular localization and molecular topology of the dopamine transporter in the striatum and substantia nigra. J. Comp. Neurol. 388, 211–227 (1997).
Grant, B. D. & Donaldson, J. G. Pathways and mechanisms of endocytic recycling. Nat. Rev. Mol. Cell Biol. 10, 597–608 (2009).
Saunders, C. et al. Amphetamine-induced loss of human dopamine transporter activity: an internalization-dependent and cocaine-sensitive mechanism. Proc. Natl. Acad. Sci. USA 97 www.pnas.org (2000).
Wheeler, D. S. et al. Amphetamine activates Rho GTPase signaling to mediate dopamine transporter internalization and acute behavioral effects of amphetamine. Proc. Natl Acad. Sci. USA 112, E7138–E7147 (2015).
Lohani, S. et al. Burst activation of dopamine neurons produces prolonged post-burst availability of actively released dopamine. Neuropsychopharmacology 43, 2083–2092 (2018).
Kahlig, K. M. et al. Regulation of dopamine transporter trafficking by intracellular amphetamine. Mol. Pharmacol. 70, 542–548 (2006).
Underhill, S. M. et al. Amphetamines signal through intracellular TAAR1 receptors coupled to Gα13 and GαS in discrete subcellular domains. Mol. Psychiatry 1–16 (2019), https://doi.org/10.1038/s41380-019-0469-2.
Chi, X., Wang, S., Huang, Y., Stamnes, M. & Chen, J. L. Roles of Rho GTPases in intracellular transport and cellular transformation. Int. J. Mol. Sci. 14, 7089–7108 (2013).
Hinze, C. & Boucrot, E. Local actin polymerization during endocytic carrier formation. Biochem. Soc. Trans. 46, 565–576 (2018).
Cen, X. et al. Identification of Piccolo as a regulator of behavioral plasticity and dopamine transporter internalization. Mol. Psychiatry 13, 451–463 (2008).
Foster, J. D., Adkins, S. D., Lever, J. R. & Vaughan, R. A. Phorbol ester induced trafficking-independent regulation and enhanced phosphorylation of the dopamine transporter associated with membrane rafts and cholesterol. J. Neurochem. 105, 1683–1699 (2008).
Hong, W. C. & Amara, S. G. Membrane cholesterol modulates the outward facing conformation of the dopamine transporter and alters cocaine binding. J. Biol. Chem. 285, 32616–32626 (2010).
Jones, K. T., Zhen, J. & Reith, M. E. A. Importance of cholesterol in dopamine transporter function. J. Neurochem. 123, 700–715 (2012).
Adkins, E. M. et al. Membrane mobility and microdomain association of the dopamine transporter studied with fluorescence correlation spectroscopy and fluorescence recovery after photobleaching. Biochemistry 46, 10484–10497 (2007).
Schneider, A. et al. Flotillin-dependent clustering of the amyloid precursor protein regulates its endocytosis and amyloidogenic processing in neurons. J. Neurosci. 28, 2874–2882 (2008).
Amaddii, M. et al. Flotillin-1/Reggie-2 protein plays dual role in activation of receptor-tyrosine kinase/mitogen-activated protein kinase signaling. J. Biol. Chem. 287, 7265–7278 (2012).
Cullen, P. J. & Steinberg, F. To degrade or not to degrade: mechanisms and significance of endocytic recycling. Nat. Rev. Mol. Cell Biol. 19, 679–696 (2018).
Schöneberg, J., Lee, I. H., Iwasa, J. H. & Hurley, J. H. Reverse-topology membrane scission by the ESCRT proteins. Nat. Rev. Mol. Cell Biol. 18, 5–17 (2016).
Bonifacino, J. S. & Rojas, R. Retrograde transport from endosomes to the trans-Golgi network. Nat. Rev. Mol. Cell Biol. 7, 568–579 (2006).
Möbius, W. et al. Recycling compartments and the internal vesicles of multivesicular bodies harbor most of the cholesterol found in the endocytic pathway. Traffic 4, 222–231 (2003).
Seaman, M. N. J. The retromer complex-endosomal protein recycling and beyond. J. Cell Sci. 125, 4693–4702 (2012).
Eriksen, J. et al. Visualization of dopamine transporter trafficking in live neurons by use of fluorescent cocaine analogs. J. Neurosci. 29, 6794–6808 (2009).
Eriksen, J., Bjørn-Yoshimoto, W. E., Jørgensen, T. N., Newman, A. H. & Gether, U. Postendocytic sorting of constitutively internalized dopamine transporter in cell lines and dopaminergic neurons. J. Biol. Chem. 285, 27289–27301 (2010).
Hong, W. C. & Amara, S. G. Differential targeting of the dopamine transporter to recycling or degradative pathways during amphetamine-or PKC-regulated endocytosis in dopamine neurons. FASEB J. 27, 2995–3007 (2013).
Rao, A., Richards, T. L., Simmons, D., Zahniser, N. R. & Sorkin, A. Epitope‐tagged dopamine transporter knock‐in mice reveal rapid endocytic trafficking and filopodia targeting of the transporter in dopaminergic axons. FASEB J. 26, 1921–1933 (2012).
Rao, A., Simmons, D. & Sorkin, A. Differential subcellular distribution of endosomal compartments and the dopamine transporter in dopaminergic neurons. Mol. Cell. Neurosci. 46, 148–158 (2011).
Miranda, M., Dionne, K. R., Sorkina, T. & Sorkin, A. Three ubiquitin conjugation sites in the amino terminus of the dopamine transporter mediate protein kinase C-dependent endocytosis of the transporter. Mol. Biol. Cell 18, 313–323 (2007).
Miranda, M., Wu, C. C., Sorkina, T., Korstjens, D. R. & Sorkin, A. Enhanced ubiquitylation and accelerated degradation of the dopamine transporter mediated by protein kinase C. J. Biol. Chem. 280, 35617–35624 (2005).
Vina-Vilaseca, A. & Sorkin, A. Lysine 63-linked polyubiquitination of the dopamine transporter requires WW3 and WW4 domains of Nedd4-2 and UBE2D ubiquitin-conjugating enzymes. J. Biol. Chem. 285, 7645–7656 (2010).
Clague, M. J., Liu, H. & Urbé, S. Governance of endocytic trafficking and signaling by reversible ubiquitylation. Dev. Cell 23, 457–467 (2012).
Cartier, E. et al. The SUMO-conjugase Ubc9 prevents the degradation of the dopamine transporter, enhancing its cell surface level and dopamine uptake. Front. Cell. Neurosci. 13, 35 (2019).
Furman, C. A., Lo, C. B., Stokes, S., Esteban, J. A. & Gnegy, M. E. Rab 11 regulates constitutive dopamine transporter trafficking and function in N2A neuroblastoma cells. Neurosci. Lett. 463, 78–81 (2009).
Loder, M. K. & Melikian, H. E. The dopamine transporter constitutively internalizes and recycles in a protein kinase C-regulated manner in stably transfected PC12 cell lines. J. Biol. Chem. 278, 22168–22174 (2003).
Wu, S. et al. The dopamine transporter recycles via a retromer-dependent postendocytic mechanism: Tracking studies using a novel fluorophore-coupling approach. J. Neurosci. 37, 9438–9452 (2017).
Bagalkot, T. R. et al. Dopamine transporter localization in medial forebrain bundle axons indicates its long-range transport primarily by membrane diffusion with a limited contribution of vesicular traffic on retromer-positive compartments. J. Neurosci. JN-RM-0744-20 (2020), https://doi.org/10.1523/jneurosci.0744-20.2020.
Cataldi, S. et al. Altered dopamine release and monoamine transporters in Vps35 p.D620N knock-in mice. npj Park. Dis. 4, 27 (2018).
Lauffer, B. E. L. et al. SNX27 mediates PDZ-directed sorting from endosomes to the plasma membrane. J. Cell Biol. 190, 565–574 (2010).
Burd, C. & Cullen, P. J. Retromer: a master conductor of endosome sorting. Cold Spring Harb. Perspect. Biol. 6, a016774 (2014).
Rickhag, M. et al. A C-terminal PDZ domain-binding sequence is required for striatal distribution of the dopamine transporter. Nat. Commun. 4, 1580 (2013).
Mecozzi, V. J. et al. Pharmacological chaperones stabilize retromer to limit APP processing. Nat. Chem. Biol. 10, 443–449 (2014).
Munsie, L. N. et al. Retromer-dependent neurotransmitter receptor trafficking to synapses is altered by the Parkinson’s disease VPS35 mutation p.D620N. Hum. Mol. Genet. 24, 1691–1703 (2015).
Temkin, P. et al. SNX27 mediates retromer tubule entry and endosome-to-plasma membrane trafficking of signalling receptors. Nat. Cell Biol. 13, 715–723 (2011).
Steinberg, F. et al. A global analysis of SNX27-retromer assembly and cargo specificity reveals a function in glucose and metal ion transport. Nat. Cell Biol. 15, 461–471 (2013).
Clairfeuille, T. et al. A molecular code for endosomal recycling of phosphorylated cargos by the SNX27-retromer complex. Nat. Struct. Mol. Biol. 23, 921–932 (2016).
McCormick, P. J. et al. Palmitoylation controls recycling in lysosomal sorting and trafficking. Traffic 9, 1984–1997 (2008).
Foster, J. D. & Vaughan, R. A. Palmitoylation controls dopamine transporter kinetics, degradation, and protein kinase C-dependent regulation. J. Biol. Chem. 286, 5175–5186 (2011).
Rastedt, D. E., Vaughan, R. A. & Foster, J. D. Palmitoylation mechanisms in dopamine transporter regulation. J. Chem. Neuroanat. 83–84, 3–9 (2017).
Jones, A. R., Overly, C. C. & Sunkin, S. M. The allen brain atlas: 5 years and beyond. Nat. Rev. Neurosci. 10, 821–828 (2009).
Cerruti, C., Walther, D. M., Kuhar, M. J. & Uhl, G. R. Dopamine transporter mRNA expression is intense in rat midbrain neurons and modest outside midbrain. Molecular Brain Research vol. 18 (1993).
Malhotra, V. & Erlmann, P. Protein export at the ER: Loading big collagens into COPII carriers. EMBO J. 30, 3475–3480 (2011).
Sucic, S. et al. The serotonin transporter is an exclusive client of the coat protein complex II (COPII) component SEC24C. J. Biol. Chem. 286, 16482–16490 (2011).
Robinson, S. B. et al. Sequence determinants of the Caenhorhabditis elegans dopamine transporter dictating in vivo axonal export and synaptic localization. Mol. Cell. Neurosci. 78, 41–51 (2017).
Dong, C. et al. A Triple Arg Motif Mediates α 2B-Adrenergic Receptor Interaction with Sec24C/D and Export. Traffic 13, 857–868 (2012).
Hoze, N. et al. Heterogeneity of AMPA receptor trafficking and molecular interactions revealed by superresolution analysis of live cell imaging. Proc. Natl Acad. Sci. U. S. A. 109, 17052–17057 (2012).
Bar-On, D. et al. Super-resolution imaging reveals the internal architecture of nano-sized syntaxin clusters. J. Biol. Chem. 287, 27158–27167 (2012).
Trinh, J. & Farrer, M. Advances in the genetics of Parkinson disease. Nat. Rev. Neurol. 9, 445–454 (2013).
Lam, H. A. et al. Elevated tonic extracellular dopamine concentration and altered dopamine modulation of synaptic activity precede dopamine loss in the striatum of mice overexpressing human α-synuclein. J. Neurosci. Res. 89, 1091–1102 (2011).
Unger, E. L. et al. Locomotor hyperactivity and alterations in dopamine neurotransmission are associated with overexpression of A53T mutant human α-synuclein in mice. Neurobiol. Dis. 21, 431–443 (2006).
Kurz, A. et al. A53T-alpha-synuclein overexpression impairs dopamine signaling and striatal synaptic plasticity in old mice. PLoS One 5, 1–15 (2010).
Nuber, S. et al. Neurodegeneration and motor dysfunction in a conditional model of Parkinson’s disease. J. Neurosci. 28, 2471–2484 (2008).
Lundblad, M., Decressac, M., Mattsson, B. & Björklund, A. Impaired neurotransmission caused by overexpression of α-synuclein in nigral dopamine neurons. Proc. Natl Acad. Sci. U. S. A. 109, 3213–3219 (2012).
Richfield, E. K. et al. Behavioral and neurochemical effects of wild-type and mutated human α-synuclein in transgenic mice. Exp. Neurol. 175, 35–48 (2002).
Wersinger, C., Prou, D., Vernier, P., Niznik, H. B. & Sidhu, A. Mutations in the lipid-binding domain of α-synuclein confer overlapping, yet distinct, functional properties in the regulation of dopamine transporter activity. Mol. Cell. Neurosci. 24, 91–105 (2003).
Longhena, F., Faustini, G., Missale, C., Pizzi, M. & Bellucci, A. Dopamine transporter/α-synuclein complexes are altered in the post mortem caudate putamen of Parkinson’s disease: An in situ proximity ligation assay study. Int. J. Mol. Sci. 19, 1611 (2018).
Butler, B. et al. Dopamine transporter activity is modulated by α-synuclein. J. Biol. Chem. 290, 29542–29554 (2015).
Swant, J. et al. Α-Synuclein Stimulates a Dopamine Transporter-Dependent Chloride Current and Modulates the Activity of the Transporter. J. Biol. Chem. 286, 43933–43943 (2011).
Wersinger, C. & Sidhu, A. Attenuation of dopamine transporter activity by α-synuclein. Neurosci. Lett. 340, 189–192 (2003).
Wersinger, C., Prou, D., Vernier, P. & Sidhu, A. Modulation of dopamine transporter function by alpha-synuclein is altered by impairment of cell adhesion and by induction of oxidative stress. FASEB J. 17, 2151–2153 (2003).
Wersinger, C., Vernier, P. & Sidhu, A. Trypsin Disrupts the Trafficking of the Human Dopamine Transporter by α-Synuclein and Its A30P Mutant. Biochemistry 43, 1242–1253 (2004).
Adams, J. R. et al. PET in LRRK2 mutations: Comparison to sporadic Parkinson’s disease and evidence for presymptomatic compensation. Brain 128, 2777–2785 (2005).
Zhou, H. et al. Temporal expression of mutant LRRK2 in adult rats impairs dopamine reuptake. Int. J. Biol. Sci. 7, 753–761 (2011).
Longo, F. et al. Age-dependent dopamine transporter dysfunction and Serine129 phospho-α-synuclein overload in G2019S LRRK2 mice. Acta Neuropathol. Commun. 5, 22 (2017).
Volta, M. et al. Initial elevations in glutamate and dopamine neurotransmission decline with age, as does exploratory behavior, in LRRK2 G2019S knock-in mice. Elife 6, (2017).
Roosen, D. A. & Cookson, M. R. LRRK2 at the interface of autophagosomes, endosomes and lysosomes. Mol. Neurodegeneration 11, 1–10 (2016).
Schreij, A. M. et al. LRRK 2 localizes to endosomes and interacts with clathrin‐light chains to limit Rac1 activation. EMBO Rep. 16, 79–86 (2015).
Law, B. M. H. et al. A direct interaction between leucine-rich repeat kinase 2 and specific β-Tubulin isoforms regulates tubulin acetylation. J. Biol. Chem. 289, 895–908 (2014).
Godena, V. K. et al. Increasing microtubule acetylation rescues axonal transport and locomotor deficits caused by LRRK2 Roc-COR domain mutations. Nat. Commun. 5, (2014).
Gómez-Suaga, P. et al. LRRK2 delays degradative receptor trafficking by impeding late endosomal budding through decreasing Rab7 activity. Hum. Mol. Genet. 23, 1–18 (2014).
Steger, M. et al. Phosphoproteomics reveals that Parkinson’s disease kinase LRRK2 regulates a subset of Rab GTPases. Elife 5, 1–28 (2016).
Di Maio, R. et al. LRRK2 activation in idiopathic Parkinson’s disease. Sci. Transl. Med. 10, eaar5429 (2018).
Kiral, F. R., Kohrs, F. E., Jin, E. J. & Hiesinger, P. R. Rab GTPases and Membrane Trafficking in Neurodegeneration. Curr. Biol. 28, R471–R486 (2018).
Tang, B. L. Rabs, Membrane Dynamics, and Parkinson’s Disease. J. Cell. Physiol. 232, 1626–1633 (2017).
Bailey, R. M. et al. LRRK2 phosphorylates novel tau epitopes and promotes tauopathy. Acta Neuropathol. 126, 809–827 (2013).
Melrose, H. L. et al. Impaired dopaminergic neurotransmission and microtubule-associated protein tau alterations in human LRRK2 transgenic mice. Neurobiol. Dis. 40, 503–517 (2010).
Lucas, R. M. et al. LRRK2-mediated phosphorylation of HDAC6 regulates HDAC6-cytoplasmic dynein interaction and aggresome formation. bioRxiv 554881 (2019), https://doi.org/10.1101/554881.
Vilariño-Güell, C. et al. VPS35 mutations in parkinson disease. Am. J. Hum. Genet. 89, 162–167 (2011).
Zimprich, A. et al. A mutation in VPS35, encoding a subunit of the retromer complex, causes late-onset parkinson disease. Am. J. Hum. Genet. 89, 168–175 (2011).
Zavodszky, E. et al. Mutation in VPS35 associated with Parkinson’s disease impairs WASH complex association and inhibits autophagy. Nat. Commun. 5, 3828 (2014).
Huang, Y. et al. VPS35 Interacts with Dopamine Transportor and Disrupts Dopamine Transporter Recycling Pathway. SSRN Electron. J. (2020), https://doi.org/10.2139/ssrn.3315811.
Puthenveedu, M. A. et al. Sequence-dependent sorting of recycling proteins by actin-stabilized endosomal microdomains. Cell 143, 761–773 (2010).
Lee, S., Chang, J. & Blackstone, C. FAM21 directs SNX27-retromer cargoes to the plasma membrane by preventing transport to the Golgi apparatus. Nat. Commun. 7, (2016).
Inoshita, T. et al. Vps35 in cooperation with LRRK2 regulates synaptic vesicle endocytosis through the endosomal pathway in Drosophila. Hum. Mol. Genet. 26, 2933–2948 (2017).
Mir, R. et al. The Parkinson’s disease VPS35[D620N] mutation enhances LRRK2-mediated Rab protein phosphorylation in mouse and human. Biochem. J. 475, 1861–1883 (2018).
MacLeod, D. A. et al. RAB7L1 Interacts with LRRK2 to Modify Intraneuronal Protein Sorting and Parkinson’s Disease Risk. Neuron 77, 425–439 (2013).
Kahle, P. J. & Haass, C. How does parkin ligate ubiquitin to Parkinson’s disease? First in molecular medicine review series. EMBO Rep. 5, 681–685 (2004).
Lücking, C. B. et al. Association between Early-Onset Parkinson’s Disease and Mutations in the Parkin Gene. N. Engl. J. Med. 342, 1560–1567 (2000).
Isaacs, D., Claassen, D., Bowman, A. B. & Hedera, P. Phenotypic discordance in siblings with identical compound heterozygous PARK2 mutations. Brain Sci. 7, (2017).
Varrone, A. et al. Imaging of dopaminergic dysfunction with [123I]FP-CIT SPECT in early-onset parkin disease. Neurology 63, 2097–2103 (2004).
Moszczynska, A. et al. Parkin disrupts the α-synuclein/dopamine transporter interaction: Consequences toward dopamine-induced toxicity. J. Mol. Neurosci. 32, 217–227 (2007).
Song, P., Trajkovic, K., Tsunemi, T. & Krainc, D. Parkin modulates endosomal organization and function of the endo-lysosomal pathway. J. Neurosci. 36, 2425–2437 (2016).
Williams, E. T. et al. Parkin mediates the ubiquitination of VPS35 and modulates retromer-dependent endosomal sorting. Hum. Mol. Genet. 27, 3189–3205 (2018).
Fallon, L. et al. A regulated interaction with the UIM protein Eps15 implicates parkin in EGF receptor trafficking and PI(3)K-Akt signalling. Nat. Cell Biol. 8, 834–842 (2006).
Itier, J. M. et al. Parkin gene inactivation alters behaviour and dopamine neurotransmission in the mouse. Hum. Mol. Genet. 12, 2277–2291 (2003).
Oyama, G. et al. Impaired in vivo dopamine release in parkin knockout mice. Brain Res. 1352, 214–222 (2010).
Jiang, H. et al. Parkin controls dopamine utilization in human midbrain dopaminergic neurons derived from induced pluripotent stem cells. Nat. Commun. 3, 1–9 (2012).
Wang, J. Y. et al. The RIT2 and STX1B polymorphisms are associated with Parkinson’s disease. Park. Relat. Disord. 21, 300–302 (2015).
Emamalizadeh, B. et al. RIT2, a susceptibility gene for Parkinson’s disease in Iranian population. Neurobiol. Aging 35, e27–e28 (2014).
Lu, Y. et al. Genetic association of RIT2 rs12456492 polymorphism and Parkinson’s disease susceptibility in Asian populations: a meta-analysis. Sci. Rep. 5, 13805 (2015).
Li, J. Y. et al. Genetic association study between RIT2 and Parkinson’s disease in a Han Chinese population. Neurol. Sci. 38, 343–347 (2017).
Bossers, K. et al. Analysis of gene expression in Parkinson’s disease: possible involvement of neurotrophic support and axon guidance in dopaminergic cell death. Brain Pathol. 19, 91–107 (2009).
Sweeney, C. G. et al. Conditional, inducible gene silencing in dopamine neurons reveals a sex-specific role for Rit2 GTPase in acute cocaine response and striatal function. Neuropsychopharmacology 45, 384–393 (2020).
Walker, Q. D., Rooney, M. B., Wightman, R. M. & Kuhn, C. M. Dopamine release and uptake are greater in female than male rat striatum as measured by fast cyclic voltammetry. Neuroscience 95, 1061–1070 (1999).
Thompson, T. L. Attenuation of dopamine uptake in vivo following priming with estradiol benzoate. Brain Res. 834, 164–167 (1999).
Bossé, R., Rivest, R. & Di Paolo, T. Ovariectomy and estradiol treatment affect the dopamine transporter and its gene expression in the rat brain. Mol. Brain Res. 46, 343–346 (1997).
Disshon, K. A., Boja, J. W. & Dluzen, D. E. Inhibition of striatal dopamine transporter activity by 17β-estradiol. Eur. J. Pharmacol. 345, 207–211 (1998).
Walker, Q. D., Ray, R. & Kuhn, C. M. Sex differences in neurochemical effects of dopaminergic drugs in rat striatum. Neuropsychopharmacology 31, 1193–1202 (2006).
Gillies, G. E., Pienaar, I. S., Vohra, S. & Qamhawi, Z. Sex differences in Parkinson’s disease. Front. Neuroendocrinol. 35, 370–384 (2014).
Sulzer, D. et al. Neuromelanin biosynthesis is driven by excess cytosolic catecholamines not accumulated by synaptic vesicles. Proc. Natl Acad. Sci. USA 97, 11869–11874 (2000).
Masoud, S. T. et al. Increased expression of the dopamine transporter leads to loss of dopamine neurons, oxidative stress and l-DOPA reversible motor deficits. Neurobiol. Dis. 74, 66–75 (2015).
Filloux, F. & Townsend, J. J. Pre- and postsynaptic neurotoxic effects of dopamine demonstrated by intrastriatal injection. Exp. Neurol. 119, 79–88 (1993).
Li, X. et al. Enhanced Striatal Dopamine Transmission and Motor Performance with LRRK2 Overexpression in Mice Is Eliminated by Familial Parkinson’s Disease Mutation G2019S. J. Neurosci. 30, 1788–1797 (2010).
Yanping, L. et al. Mutant LRRK2R1441G BAC transgenic mice recapitulate cardinal features of Parkinson’s disease. Nat. Neurosci. 12, 826–828 (2009).
Ramonet, D. et al. Dopaminergic Neuronal Loss, Reduced Neurite Complexity and Autophagic Abnormalities in Transgenic Mice Expressing G2019S Mutant LRRK2. PLoS ONE 6, e18568 (2011).
Tong, Y. et al. R1441C mutation in LRRK2 impairs dopaminergic neurotransmission in mice. Proc. Natl Acad. Sci. 106, 14622–14627 (2009).
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Bu, M., Farrer, M.J. & Khoshbouei, H. Dynamic control of the dopamine transporter in neurotransmission and homeostasis. npj Parkinsons Dis. 7, 22 (2021). https://doi.org/10.1038/s41531-021-00161-2
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