Dopamine controls diverse behaviors and their dysregulation contributes to many disorders. Our ability to understand and manipulate the function of dopamine is limited by the heterogenous nature of dopaminergic projections, the diversity of neurons that are regulated by dopamine, the varying distribution of the five dopamine receptors (DARs), and the complex dynamics of dopamine release. In order to improve our ability to specifically modulate distinct DARs, here we develop a photo-pharmacological strategy using a Membrane anchored Photoswitchable orthogonal remotely tethered agonist for the Dopamine receptor (MP-D). Our design selectively targets D1R/D5R receptor subtypes, most potently D1R (MP-D1ago), as shown in HEK293T cells. In vivo, we targeted dorsal striatal medium spiny neurons where the photo-activation of MP-D1ago increased movement initiation, although further work is required to assess the effects of MP-D1ago on neuronal function. Our method combines ligand and cell type-specificity with temporally precise and reversible activation of D1R to control specific aspects of movement. Our results provide a template for analyzing dopamine receptors.
Dopamine (DA) plays important roles in health (movement, reward, aversion, motivation) and disease (Parkinson’s, schizophrenia, addiction)1,2. To understand how DA action generates behavior, we need methods that can control specific aspects of DA function. DA neurons can be functionally interrogated by optogenetic stimulation of their cell bodies or axon terminals (Supplementary Fig. 1). However, DA neurons have diverse downstream targets, making it difficult to identify the casual basis of specific behavioral outcomes. For example, the striatum is a hub region that receives dense dopaminergic innervation from the midbrain1. Multiple distinct, spatially intermixed and inter-connected striatal cell types express various combinations of four of the five DA receptor (DAR) subtypes, the Gs/olf-coupled D1-like receptors D1R and D5R and the Gi/o/z-coupled D2-like receptors D2R and D3R (Supplementary Fig. 1e)1. Beyond the complex localization and distinct signaling properties of the different DARs, DA signals operate over phasic (hundreds of milliseconds) to slowly varying (tens of seconds to minutes) temporal domains3. Moreover, DA can be co-released with glutamate4 and/or GABA5, which may contribute to dynamic area-specific modulation6.
The relationship between DA release and the activation of specific striatal DARs in different cells is not well understood. In addition, there is evidence that local regulation of DA release in the striatum can occur independently of the action potential firing in DA neurons and is triggered or modulated by axo-axonal inputs onto the dopaminergic axons7,8. Indeed, different levels of DA input activity appear to selectively target D2R over D1R, according to distinct receptor affinities for DA9 but could also reflect targeted signaling.
Recent studies indicate that dopaminergic input from the substantia nigra compacta (SNc) to the dorsal striatum (dStr) initiates but does not sustain movement. SNc DA neurons become more active just before movement initiation6,10, and the brief optogenetic stimulation of these neurons increases the probability of movement initiation11. This raises the question: Which of the many targets of SNc DA neurons in the dStr (Supplementary Fig. 1e) triggers movement? A compelling candidate is D1R expressed in direct pathway medium spiny neurons (dMSNs) of the dStr. The activation of dMSNs has long been known to promote movement12,13,14. While some studies indicate that D1R can reduce dMSN excitability15,16,17, it is generally accepted that the activation of these receptors promotes dMSN excitability18,19,20,21,22. Moreover, a recent model suggests that D1R increases in activation in the dStr prior to movement initiation10, and the systemic activation of D1R with a synthetic agonist increases the probability of movement initiation23. For these reasons, D1R is a putative target for treatment of motor deficits in Parkinson’s disease24, where dopaminergic inputs from the SNc to the dStr degenerate. However, D1R agonists do not differentiate between D1R in dMSNs and the terminals of glutamatergic inputs in the dStr (Supplementary Figs. 1e and 2)1, and they also bind its close homolog D5R25, which is found in the four major classes of striatal interneurons (Supplementary Fig. 1e). Even if applied directly to the dStr, D1R agonists could diffuse and activate D1R and D5R in other brain areas with unpredictable kinetics. Alternatively, receptor knockout studies do not clearly define the role of D1R in movement (Supplementary Fig. 3)26,27,28,29 and suggest that D2R, which is also abundant in the dStr, can drive movement initiation30. Nevertheless, genetic modifications cannot be applied with temporal specificity and could result in system compensation, highlighting the need for a new method that can precisely control specific DARs.
Several approaches offer greater cell type and spatiotemporal specificity over GPCR signaling than conventional methods. Engineered DREADD and RASSL GPCRs enable orthogonal receptor activation through their use of an artificial ligand (Supplementary Fig. 2)31, but are non-native proteins that lack the localization and biochemical selectivity of endogenous receptors. Opto-XR chimeras of an opsin and the intracellular portions of a receptor of interest32 can be activated by light, but lack an endogenous ligand binding site and much of the native GPCR. DREADDs, RASSLs, and opto-XRs are more suited to overdrive signaling than substitute for the normal receptor. In contrast, t-toxins, DARTs, and Lumitoxins enable control of the endogenous receptor by tethering a ligand to a genetically-encoded plasma membrane protein anchor (Supplementary Fig. 2), but these are either persistently active33 or take minutes to hours to turn on or off34,35.
To examine D1R function in vivo, we implemented a photo-pharmacological strategy, along the lines that we developed recently for metabotropic glutamate receptors (mGluRs)36. In this strategy, a genetically-encoded membrane anchor (M) is selectively expressed in specific cells. The M captures a synthetic photoswitched ligand (P) by selective chemical conjugation to a protein tag, thereby restricting the P to a target class of cells in a specific location in the brain. Between the protein tag attachment and ligand ends of the P lies a flexible chain that is long enough to extend from the M anchor to a native receptor to which the ligand is suited. This approach follows the logic of DARTs34,35, with the key and unique feature that the P is photoswitchable37,38,39 and thus turns its target receptor on and off rapidly and reversibly in response to light, providing spatiotemporal control. We engineered the M to adapt the approach from the Family C mGluR, which has a large extracellular clamshell ligand binding domain “above” the transmembrane domain, to the Family A DAR, whose ligand binds within the transmembrane domain.
We developed a novel D1R/D5R selective-MP agonist that is most potent on D1R (hence called MP-D1ago). We targeted MP-D1ago to dMSNs, where it would selectively activate D1R and avoid D5Rs in other striatal neurons (Supplemental Fig. 1e). Photo-activation of MP-D1ago in the dMSNs of the dStr promoted movement initiation. Strikingly, this effect was as potent as optogenetic stimulation of dopaminergic nerve terminals that project to the dStr from the substantia nigra compacta (SNc). The MP method, which derives specificity from a combination of the P ligand and cell-specific expression of the M, should be applicable to other DARs and to neuronal receptors in general, providing insight into neural circuit function and neuromodulation.
Design of a D1R MP
MP is composed of two components, a photoswitchable orthogonal remotely tethered ligand (P) and a membrane anchor (M) that restricts the P to the cell surface (Fig. 1a). The P component contains a receptor ligand at one end, a protein-tag reactive moiety at the other end, an adjustable chemical linker in between, and an azobenzene that is flush to or merged with the receptor ligand. The azobenzene photoisomerizes between its trans and cis configurations in milliseconds40, rapidly switching the receptor ligand between two states: one that is exposed and can bind its receptor and one that is obstructed by the azobenzene and so cannot bind. The P is restricted via the reactive moiety to the membranes of cells that express the M, a genetically-encoded membrane-anchored protein-tag. The chemical linker between azobenzene and reactive moiety is long enough to allow the P to reach from its anchor point in the M to its binding site in the receptor.
To develop a P for D1R, we used a metabolically stable analog of DA, 2-(N-phenethyl-N-propyl)-amino-5-hydroxytetralin (PPHT; Supplementary Figure 4a), as a parent molecule. We showed previously that PPHT can tolerate the integration of azobenzene at its alkylbenzene41. When tethered directly to a cysteine introduced adjacent to the DA binding site of D1R via a maleimide group, azobenzene-PPHT binds the receptor in its trans state but not its cis state41. Analogously, we synthesized an azobenzene-PPHT analog containing the reactive moiety benzylguanine (photoswitchable D1 agonist or P-D1ago), which binds covalently and selectively to an M that is composed of SNAP-tag anchored to the plasma membrane via a single-pass transmembrane segment from low density lipoprotein receptor (Fig. 1b and Supplementary Fig. 4b). Molecular modeling was used to optimize the positioning (Supplementary Fig. 5a) and length (Supplementary Fig. 5b-e) of the polyethylene glycol (PEG) chemical linker between the azobenzene-PPHT and the benzylguanine attachment site.
Optimization and characterization of the D1R MP
P-D1ago switches from its trans-isomer to its cis-isomer under 370 nm (UV) light and back to trans-isomer under 460 nm (blue) light (Supplementary Fig. 6a, b). P-D1ago binds efficiently to the M on the cell surface (Supplementary Fig. 6c–f) and is a low potency full agonist of D1R in its untethered form (Supplementary Fig. 7).
To test the ability of P-D1ago to photo-activate D1R, we first attached it directly to a version of D1R that has SNAP fused to its extracellular N-terminus, which is adjacent to the ligand binding site of the receptor. SNAP-D1R was co-expressed in HEK293T cells with the G protein-coupled inwardly rectifying potassium (GIRK) channel as an effector. Following application and washout of unbound P-D1ago, blue light (trans) activated and UV light (cis) deactivated GIRK current (Supplementary Fig. 8), demonstrating P-D1ago as an effective light-switched tethered ligand. With this in hand, we turned to attaching P-D1ago to the M, which was co-expressed in HEK293T cells with the native D1R and the GIRK channel. In this inter-protein configuration, P-D1ago once again photoactivated ion current by blue light and was deactivated by UV light (Fig. 2a, e), an effect that required expression of GIRK channels (Supplementary Fig. 9a) and D1R (Supplementary Fig. 9b, c), which indicated that inter-protein photo-activation of native D1R works. To optimize D1R photoactivation, we adjusted the geometric positioning of P-D1ago using variants of M with “lift” peptides between the SNAP-tag and transmembrane segment. Photoactivation increased with an M variant containing a rigid, α-helical EAAAK peptide (MEAAAK Fig. 2b, c, e) and decreased as the lift peptide was further extended (Supplementary Fig. 9d–f), presumably because P-D1ago “rises” too far from the cell surface.
Pharmacological analyses suggested that when P-D1ago is tethered to MEAAAK, it partially activates D1R because it is present at a submaximal concentration at the cell surface (Supplemental Fig. 10a–g). To increase surface P-D1ago, we added to the C-terminus of MEAAAK an endoplasmic reticulum export ERE motif36,42 (MEAAAK:ERE), which approximately doubled surface SNAP-tag expression (Supplementary Fig. 10h). Remarkably, P-D1ago tethered to MEAAAK:ERE (MP-D1ago) that was stimulated by blue light activated D1R to near maximal possible levels (elicited by saturating, 10 μM, DA) (Fig. 2b, d, e) without altering baseline activation in the “off”-state, under UV light (Supplementary Fig. 10i–k). GIRK current elicited by MP-D1ago photo-activation and photo-deactivation of D1R rose and fell in seconds (Fig. 2f), with no loss in efficacy over multiple cycles (Fig. 2f), and in a bistable manner, i.e., the “on”-state was stable in the dark following a short flash of blue light and the “off”-state was stable after a short flash of UV light (Fig. 2g). This contrasts with slow off-kinetics and rundown of opto-D1R (Supplementary Fig. 11a–e)43. MP-D1ago was ~100-fold more sensitive to light than ChR2 (Fig. 2h and Supplementary Fig. 11f, g)44.
We assessed the specificity of MP-D1ago by profiling its effects on a variety of neuronal receptors, each co-expressed in HEK293T cells with the M. We first tested D5R, the closest homolog of D1R. D5R was photoactivated by MP-D1ago to about half the level of D1R (Fig. 2i; Supplementary Fig. 12a). We also evaluated other receptors that are co-expressed with D1R in the brain, including GPCRs and ionotropic receptors for DA, adenosine, cannabinoids, acetylcholine, opioids, glutamate, and GABA. MP-D1ago had no effect on any of these receptors (Fig. 2i; Supplementary Fig. 12b–m), indicating that it is a D1R/D5R-selective photo-agonist.
Activation of D1Rs in the dorsal striatum with MP-D1ago promotes movement initiation
The dStr expresses D1R and D5R (Fig. 3a), which are notoriously difficult to distinguish with conventional pharmacology25. However, dStr D1R and D5R are segregated into distinct classes of neurons: D1R is found in all dMSNs and the terminals of some glutamatergic afferents that innervate the dStr, whereas D5R is found in four types of interneurons (Fig. 3a)1. Thus, the targeted delivery of MP-D1ago to dStr-dMSNs in combination with its rapid on and off kinetics would allow us to control of D1R in the dStr with specificity and determine its effect on movement initiation.
The gene encoding the M component of MP-D1ago, MEAAAK:ERE, was delivered to dStr-dMSNs of D1-Cre mice (Fig. 3a) using a Cre recombinase (Cre)-dependent adeno-associated virus (AAV) that was stereotaxically injected (Supplementary Fig. 13a, b). An AAV containing only mVenus was used as a control. The M expressed throughout the dStr (Fig. 3b and Supplementary Fig. 13c), on the cell surface of dStr-dMSNs (Fig. 3c), and alongside endogenous D1Rs in the soma and neurites (Supplementary Fig. 13d)—prerequisites for MP-D1ago to interact with its target receptor. While we observed no obvious changes in morphology of striatal cells expressing the M, and our recent study of cultured cortical neurons expressing a similar M showed normal resting properties, action potential firing and neuromodulation36, it will be important to measure the properties of striatal neurons to assess whether M impacts their physiological parameters.
Mice expressing the M in dStr-dMSNs were infused with the UV-light induced inactive configuration of P-D1ago (cis). P-D1ago was infused into the dStr using conditions that were optimized for maximum conjugation to the M (Supplementary Fig. 14a, b). Locomotion was measured in an open field under conditions of optimized bilateral illumination (Fig. 3d and Supplementary Fig. 14c–h). Locomotion of mice with MP-D1ago increased following a flash of blue light (1 s) and returned to baseline following a flash of UV light (1 s; Supplementary Fig. 15a), an effect that was robust (Fig. 3e and Supplementary Fig. 15b, c) and repeatable (Supplementary Fig. 15d). The behavioral photo-effect was not observed in the absence of either the M or P-D1ago (Fig. 3e, f). We also tested MP-D1ago in the presence of the D1R antagonist SCH23390, which suppresses locomotion on its own45. The blue-light induced promotion of locomotion by MP-D1ago was blocked by SCH23390 (Fig. 3g and Supplementary Fig. 15e), consistent with a requirement for D1R to confer the MP-D1ago effect, though complicated by the suppression of baseline locomotion by SCH23390.
To better understand the basis of the locomotor response to photo-activation of D1R in the dStr, we measured the locomotion dynamics of mice as we photo-switched MP-D1ago from the inactive state (UV illumination) to the active state (blue illumination; Fig. 3e). The mice locomoted for a greater percentage of the time under blue light (Fig. 4a–c). The increase in locomotion was due to an increase in movement initiation (Fig. 4d) without a change in movement bout duration (Fig. 4e). There was also a modest increase in the maximum speed of motion in response to blue light (Fig. 4f). None of these differences were observed in mice lacking MP-D1ago (Supplementary Fig. 16), and there was no difference in the time spent in the center of the open field under UV light and blue light (Fig. 4g). Therefore, activation of D1R in in the dStr increases locomotion by increasing the probability of movement initiation.
We also evaluated the longer-term effect of MP-D1ago on D1Rs in the dStr by infusing the active configuration of P-D1ago (trans), which is stable in the dark (Supplementary Fig 17a). The motor activity of mice expressing the M increased within 30 min of the start of infusion of trans-P-D1ago, remained high for many hours, and returned to baseline over a two-day period (Supplementary Fig. 17b). We conjecture that the delayed activation reflects the time it takes for P-D1ago to conjugate to the M. The slow decay of the trans-MP-D1ago effect matches that observed with a membrane-anchored AMPA receptor DART antagonist in dStr-dMSNs35, likely reflecting the turnover of the membrane anchor in these neurons. However, chronic D1R activation could also result in plasticity changes of dStr-dMSNs or network effects that return locomotion to baseline. Nevertheless, consistent with the acute effect of MP-D1ago, chronic dStr-dMSN D1R activation resulted in a selective enhancement in movement initiation (Supplementary Figs. 17c–f). Thus, MP-D1ago can be used to photo-activate D1Rs in the dMSNs of the dStr either acutely or persistently.
Comparison of MP-D1ago with optogenetic activation of a dopaminergic projection to the dorsal striatum
We wondered how the behavioral effect of photo-activation of D1Rs in the dMSNs of the dStr with MP-D1ago compares with that elicited by activity in dopaminergic inputs to the dStr, which is expected to activate not only dMSN D1Rs but also DARs in each cell type of the dStr, as well as GABA receptors (Supplementary Fig. 1e). To test this, a Cre-dependent AAV encoding ChR2-eYFP was injected into the SNc of DAT-Cre mice. Robust eYFP expression was observed in SNc DA neurons, the major DA input to the dStr46, and in the dStr, where SNc DA neurons make their axon terminal beds (Fig. 5b and Supplementary Fig. 18a). As described earlier6, activating ChR2 in SNc DA axon terminals in the dStr enhanced locomotion in the open field (Fig. 5c–f and Supplementary Fig. 18b). The enhanced locomotion was due to an increase in movement initiation, with no change in the duration of movement bouts (Fig. 5g and Supplementary Fig. 18c–f). The timing and magnitude of these effects closely resembled those elicited by photo-activation of D1Rs in the dMSNs of the dStr with MP-D1ago (Fig. 5h, i). This suggests that activation of D1Rs in the dMSNs of the dStr accounts for a significant portion of the ability of SNc DA neurons to enhance movement.
Comparison of MP-D1ago with a conventional D1R agonist
We compared the selective activation of D1R in dStr-dMSNs with MP-D1ago to infusion into the dStr of the conventional full D1R agonist SKF82958, which is expected to also activate D5R in multiple cell types. Like MP-D1ago, SKF82958 enhanced locomotion (Supplementary Fig. 19b–c). However, locomotion increased ~12-times faster with MP-D1ago than with SKF82958 (Supplementary Fig. 19d), reflecting the temporal difference between light propagation (fast) and pharmacologic diffusion (slow) in brain tissue. Moreover, although both increased the percentage of the time that the mice were in motion (Supplementary Fig. 19e, f), MP-D1ago selectively increased the probability of movement initiation (Fig. 4), whereas SKF82958 increased both movement initiation and the duration of the movement bouts (Supplementary Fig. 19g, h). This difference indicates that locally infused DAR ligands may not faithfully mimic the actions of dopaminergic input, either because of differences in the activation of different DAR subtypes and cell types or because they diffuse to other brain areas (Supplementary Fig. 19a).
D1Rs in the nucleus accumbens have no effect on movement
Whereas the dStr is specialized for movement control, the nucleus accumbens (NAc) is associated with reward6 and motivation47. However, studies suggest that dopaminergic input from the ventral tegmental area (VTA) to the NAc can also promote movement, possibly by increasing motivation and decreasing work-related response costs47,48 or promoting motor learning49. D2R in indirect pathway-MSNs of the NAc (NAc-iMSNs) promotes locomotion in an open field50. By contrast, the effect of D1R in the NAc on locomotion is less clear because existing methods have produced contradictory results43,51,52,53. To explore this, we probed the effect of MP-D1ago photo-activation in dMSNs of the NAc (NAc-dMSNs). We observed no effect on locomotion of switching fiber illumination from UV to blue light (Supplementary Fig. 20), suggesting that motor activation in the NAc is not driven by dMSN D1R.
DA plays central roles in behavior. To understand DA neuromodulation, we need to be able to control the activation of specific DARs in specific cell types and brain regions with temporal precision. Optogenetic tools like ChR2 tell us how behavior changes in response to the activation of specific DA neurons, providing a cellular view of DA action in the brain. MPs offer a complementary perspective: they tell us how behavior changes in response to the activation of just one of the many targets of those DA neurons (Fig. 6). MPs are uniquely suited to this task because they control endogenous DARs with receptor subtype, cell type, and spatiotemporal specificity. We present here an initial demonstration that the MP approach can modulate neuromodulatory receptors affecting behavior. An important caveat of this work is that the neural effects in vivo have not been investigated.
The activity of SNc neuron axons that release DA onto to the dStr promotes movement initiation11,54. SNc DA neurons co-release glutamate and GABA55,56, which may contribute to the effect. Moreover, multiple DAR subtypes in various combinations in each of the cell types of the dStr may be activated by DA released from SNc axon terminals (Supplementary Fig. 1e).
We used MP-D1ago to bypass the SNc DA neurons and directly activate a DAR on one SNc target: the D1R of dStr-dMSNs. To do this, we delivered the gene encoding M using AAV under Cre control into the dStr of D1-Cre mice to yield selective expression in dStr-dMSNs. Following expression, we infused P-D1ago into the same site. Illumination to photo-activate D1ago was found to promote locomotion as effectively, with the same selective boost of movement initiation, and with the same kinetics as optogenetic stimulation of SNc DA axon terminals. This supports the notion that dMSN D1R is the key target of DA in the dStr that contributes to movement initiation. This could not be ascertained with the conventional D1R agonist SKF82958, which does not match the actions of dopaminergic input from the SNc to the dStr, likely due to a lack of molecular, cell type, and/or spatiotemporal precision.
D1R activation in response to endogenous DA or synthetic D1R agonists increases dMSN excitability18,19,20,21,22, which is associated with enhanced movement12,13,14. Electrophysiological analysis of the effect of MP-D1ago on dMSN physiology will be required to demonstrate that this photo-activation of D1R enhances movement through the same mechanism and to determine whether M expression affects the physiological properties of dMSNs. Relevant to this, a similar M was not found to perturb cultured cortical neurons36. Nevertheless, MP-D1ago could provide insight into the effect of D1R activation on dMSN excitability and ion channels such as NMDA receptors with greater selectivity and temporal precision than that used in previous studies22,55.
We found that both the optogenetic stimulation of SNc terminals and the direct photo-activation of dMSN D1Rs with MP-D1ago increase movement gradually over minutes. This contrasts with the rapid second-timescale kinetics of DA release in the dStr, as detected by voltammetry22 and optical reporters54,56,57, and of D1R effector activation and deactivation by MP-D1ago in cultured cells that we report here. The mismatch is consistent with dStr-dMSN D1R signaling increasing the response to locomotor drive from other inputs, such as projections from motor cortex. Although we have not deployed it here, the ability to rapidly turn MPs on and off provides the opportunity to establish the dependence of behavioral output on the temporal dynamics of activating specific DARs in specific striatal cells. In principle, this could apply to movement, Pavlovian conditioning, or reward prediction error, wherein extracellular DA rises transiently for less than a second to tens of seconds54.
Recent work indicates that adjacent subregions of the dStr have distinct functional properties58,59. Whereas the dorsomedial striatum (DMS) controls the initial stages of motor learning, the dorsolateral striatum (DLS) facilitates the acquisition of habitual and automatic behavior60,61. Unlike diffusible conventional agonists or antagonists, our approach could be used to selectively target specific DAR subtypes in specific subregions of the dStr by limiting the expression of the M component of the MP.
A major hurdle in the study of DA has been our inability to selectively target specific DARs. For example, there are currently no conventional agonists and antagonists that can differentiate between these D1R and D5R17 due to the high similarity between these receptors21. In recent years considerable effort has gone towards developing allosteric modulators of D1R, which bind non-conserved regions and thus are more likely to be receptor selective. However, existing allosteric modulators are not sufficiently D1R-selective62 or have very low affinity for rodent D1R63,64 so are not compatible with rodent studies. In contrast, MPs can bestow receptor subtype selectivity onto otherwise non-selective ligands by taking advantage of the inherent cellular segregation of closely related DARs in DA neurons. MP-D1ago, which contains a non-selective D1R/D5R agonist, was restricted to striatal dMSNs that express D1R but not D5R. A similar strategy could be used to target D2R, for which there are no highly selective ligands due to its high homology with D3R65. For example, a MP that contains an inherently non-selective D2R/D3R ligand could be used to selectively control D2R in striatal iMSNs because these neurons lack D3R (Supplemental Fig. 1e). Although the MP approach can take advantage of the cellular segregation of closely related receptors, the development of MP analogs that contain DAR subtype selective ligands will be need for cases when closely related receptors are expressed in the same cells.
Optogenetics tools like ChR2 require one component (Supplementary Fig. 2), a genetically encoded protein, and light. MPs require an additional custom chemical component. Considering that DARs have similar architecture, we expect that modular changes to the agonist moiety of P-D1ago will make it possible to create a repertoire of ligands, each with narrow action, but which, as a group, cover a wide range of functionalities. Like optogenetic stimulation, DAR activation with MP agonists, like MP-D1ago, is an unnatural manipulation that occurs separately from the actions of DA. Substitution of the PPHT agonist moiety of MP-D1ago with an MP antagonist or negative allosteric modulator could provide the advantage of rapid and reversible block of receptor activation in response to natural DA signals. Furthermore, just as DAR subtypes are targeted to various subcellular compartments, MPs could be modified through the addition of genetically-encoded targeting motifs to the M to enable additional experimental specificity. For all of these applications, it will be important in future work to characterize how MP-Ds photo-modulate the biochemical and physiological signaling of cells in both brain slice and in vivo.
With the current DAR MP and the recent MP for mGluRs36, we have shown the approach to work for both Family A and Family C GPCRs, suggesting that the approach will be generalizable to diverse neuronal receptors and channels. Given that the problem of receptor complexity is not unique to DA circuits, MPs have the potential to be used as a general approach to crack neural circuits and their relationship to behavior.
All reactions were carried out with magnetic stirring, and, if moisture- or air- sensitive, under nitrogen or argon atmosphere using standard Schlenk techniques in oven-dried glassware (140 °C oven temperature). External bath temperatures were used to record all reaction temperatures. Low temperature reactions were carried out in a Dewar vessel filled with distilled water/ice (0 °C). High temperature reactions were conducted using a heated silicon oil bath in reaction vessels equipped with a reflux condenser or in a sealed flask. Tetrahydrofuran (THF) was distilled over sodium and benzophenone prior to use. Dichloromethane (CH2Cl2), triethylamine (Et3N) and diisopropylethylamine (DIPEA) were distilled over calcium hydride under a nitrogen atmosphere. All other solvents were purchased from Acros Organics as ‘extra dry’ reagents. All other reagents with a purity >95% were obtained from commercial sources (Sigma Aldrich, Acros, Alfa Aesar, Base Click, and others) and used without further purification.
Flash column chromatography was carried out with Merck silica gel 60 (0.040–0.063 mm). Analytical thin layer chromatography (TLC) was carried out using Merck silica gel 60 F254 glass-backed plates and visualized under UV light at 254 nm. Staining was performed with ceric ammonium molybdate (CAM) or by oxidative staining with an aqueous basic potassium permanganate (KMnO4) solution and subsequent heating. HPLC was performed with HPLC grade solvents and deionized H2O that was purified on a TKA MicroPure H2O purification system. All solvents were degassed with helium gas prior to use. Unless noticed otherwise, all experiments were carried out at room temperature.
NMR spectra (1H NMR and 13C NMR) were recorded in deuterated chloroform (CDCl3) or deuterated methanol (d4-MeOH) on a Bruker Avance III HD 400 MHz spectrometer equipped with a CryoProbe™, a Varian VXR400 S spectrometer, a Bruker AMX600 spectrometer or a Bruker Avance III HD 800 MHz spectrometer equipped with a CryoProbe™ and are reported as follows: chemical shift δ in ppm (multiplicity, coupling constant J in Hz, number of protons) for 1H NMR spectra and chemical shift δ in ppm for 13C NMR spectra. Multiplicities are abbreviated as follows: s = singlet, d = doublet, t = triplet, q = quartet, quint = quintet, br = broad, m = multiplet, or combinations thereof. Residual solvent peaks of CDCl3 (δH = 7.26 ppm, δC = 77.16 ppm) and d4-MeOH (δH = 3.31 ppm, δC = 49.00 ppm) were used as an internal reference. NMR spectra were assigned using information ascertained from COSY, HMBC, HSQC, and NOESY experiments.
High resolution mass spectra (HRMS) were recorded on a Varian MAT CH7A or a Varian MAT 711 MS instrument by electron impact (EI) or electrospray ionization (ESI) techniques at the Department of Chemistry, Ludwig-Maximilians-University Munich. Infrared spectra (IR) were recorded from 4000 cm−1 to 600 cm−1 on a PERKIN ELMER Spectrum BX II, FT-IR instrument. For detection, a SMITHS DETECTION DuraSamplIR II Diamond ATR sensor was used. Samples were prepared as a neat film or a thin powder layer. IR data in frequency of absorption (cm−1) is reported as follows: w = weak, m = medium, s = strong, br = broad, or combinations thereof. P-D1ago is available from the authors upon reasonable request.
A homology model of D1R was generated using Bioluminate (Schrodinger, Inc)66. The model was based on β2-adrenergic receptor (β2AR) because of the high relative degree of homology between D1R and β2AR. The amino acid sequence of D1R was aligned to β2AR in BLAST67 and the TM segments were then structurally aligned with the crystal structure of β2AR bound to the inverse agonist carazolol (pdb: 2RH1). The three extracellular loops of D1R were refined using extended sampling. For docking DA into D1R, DA was prepared using LigPrep (Schrodinger, Inc) and docked with extra precision (XP) using Glide68. The hydroxyl groups of the three TM5 serines (Ser1945.42, Ser1955.43 and Ser1995.46) in D1R that contribute to the OBS were allowed to rotate during the docking procedure. As expected, the protonated amine and hydroxyls of DA were oriented towards Asp1003.32 in TM3 and the TM5 serines, respectively.
To dock the P-D1ago analog PEG4-azobenzene-PPHT in the D1R model, the protonated ligand was first prepared in ChemDraw (PerkinElmer) and Chimera (developed by the Resource for Biocomputing, Visualization, and Informatics at the University of California, San Francisco and supported by NIGMS P41-GM103311). It was then docked in the D1R model using Autodock Vina69. The following orthosteric binding site residues in D1R70 were allowed to rotate during the docking procedure: Asp1003.32, Ile1013.33, Ser1043.36, Ser1945.42, Ser1955.43, Ser1995.46, Trp2826.48, Phe2856.51, Phe2866.52, Asn2896.55, Val3147.39, and Trp3187.43.
To measure the distance from the benzylguanine binding site in the membrane-anchor (M) to the ligand binding site in D1R or mGluR5, a model of the M was made by placing the C-terminus of SNAP-tag (pdb: 3L00) flush with the N-terminus of a single-pass transmembrane segment (pdb: 2K1A). The M was then positioned adjacent to mGluR5 or D1R. The benzylguanine binding site in the M was oriented facing towards the receptor ligand binding site. To measure the lengths of P-D1ago or BGAG, their extended states were first prepared in ChemDraw and end-to-end distances for each chemical component were measured in Chimera.
All molecular representations were prepared using Chimera.
Molecular biology and heterologous expression
All constructs are in mammalian expression vectors. For the receptor mediated-GIRK activation assay, HEK293T cells were seeded onto 18 mm coverslips and transiently transfected overnight with Lipofectamine 2000 and the following constructs: a receptor, a variant of the membrane-anchor (M; 0.7 µg), GIRK1(F137S) (0.7 µg), and tdTomato (0.2 µg). The following receptors were tested: D1R (0.525 µg), opto-D1R (0.7 µg), D3R (0.2 µg), D5R (0.35 µg), A1R (0.7 µg), CB1R (0.7 µg), M1R (0.7 µg), M4R (0.7 µg), MOR (0.7 µg), mGluR1 (0.7 µg), and GABABR (0.7 µg of each subunit, B1 and B2). Some of these receptors do not couple to GIRK channels in HEK293T cells unless coexpressed with certain Gα subunits. D1R, D5R, or opto-D1R were cotransfected with Gαis13 (0.35 µg), D3R with GαoA (0.7 µg), and M1R or mGluR1 with Gαiq5. Transfected cells were used for electrophysiology, imaging, or flow cytometry experiments.
For ligand gated-ion channel (LGIC) electrophysiology, HEK293T cells were seeded onto 18 mm coverslips and transiently transfected for 48 h with Lipofectamine 2000 and the following constructs: MAEAAAK:ERE (0.7 µg), tdTomato (0.2 µg), and one of the following: a non-desensitizing mutant of AMPAR GluRA1 (L497Y; 1.4 µg), the kainite receptor GluK2 (0.7 µg), or GABAARα1β2γ2 (0.2 µg α1: 0.2 µg β2: 0.7 µg γ2).
Confocal imaging and flow cytometric analysis of cultured cells
Untransfected or membrane-anchor (M) expressing HEK293T cells were labeled with 1.5 µM BG-TMR or BG-Alexa647 (NEB) for 20–30 min in the dark at 37 °C and 5% CO2 in a standard extracellular solution. Cells were then (i) mounted on an upright, scanning confocal microscope (Zeiss LSM 780) and imaged with a 20× objective or (ii) washed in DPBS and measured by flow cytometry (BD LSR II) using FACSDiva 6.0 software (BD Biosciences).
HEK293T cells were sparsely seeded and maintained in DMEM (Invitrogen) with 10% fetal bovine serum on poly-L-lysine-coated coverslips at 37 °C and 5% CO2. HEK293T cells were voltage clamped in whole-cell configuration 16–48 h after transfection. For GIRK experiments, the extracellular solution contained 120 mM KCl, 25 mM NaCl, 10 mM HEPES, 2 mM CaCl2, and 1 mM MgCl2, pH 7.4. opto-D1R cells were preincubated for 45 min with and patched in the presence of 1 µM 11-cis-retinal. For LGIC experiments, the extracellular solution contained 135 mM NaCl, 5.4 mM KCl, 10 mM HEPES, 2 mM CaCl2, and 1 mM MgCl2, pH 7.4. GluK2 electrophysiology was performed in the presence of 0.3 mg/mL concanavalin A to prevent desensitization. Glass pipettes with a resistance of 3-7 MΩ were filled with intracellular solution containing 120 mM Gluconic acid δ-lactone, 15 mM CsCl, 10 mM BAPTA, 10 mM HEPES, 1 mM CaCl2, 3 MgCl2, 3 mM MgATP, pH 7.2. Cells were voltage clamped to −60 or −80 mV using an Axopatch 200 A (Molecular Devices) amplifier.
To conjugate P-D1ago to variants of the membrane-anchor (M), cells were incubated with varying concentrations of P-D1ago for up to 60 min in the dark at 37 °C in standard extracellular buffers. For all experiments, compounds were applied using a gravity-driven perfusion system and illumination was applied to the entire field of view using a Polychrome V monochromator (TILL Photonics) through a 20× objective (maximum 0.05 mW/mm2 at 370 nm and 0.5 mW/mm2 at 460 nm or 473 nm) or a DG4 (Sutter) through a 20× objective (maximum 0.06 mW/mm2 at 370 nm and 0.6 mW/mm2 at 445 nm). pClamp software (Clampex 10; Axon Instruments) was used for both data acquisition and control of illumination.
The selection criteria for electrophysiological experiments are that a cell (i) expresses the fluorescent protein transfection marker, and (ii) responds to agonist, indicating the presence of either receptor and GIRK or an LGIC. We did not exclude cells unless the recording was of poor quality (e.g., unstable baseline).
The following mouse lines were used for the experiments: D1-Cre (GENSAT, stock number: 017264-UCD, strain code: Tg(Drd1-cre)EY262Gsat/Mmucd) and DAT::IRES-Cre (Jackson Laboratory, stock number: 006660, strain code: B6.SJL-Slc6a3tm1.1(cre)Bkmn/J). The mice were 20–30 grams and 8–20 weeks old. Males and females were counterbalanced across conditions with no effects of sex observed. Mice were maintained on a 12:12 light cycle (lights on at 07:00) at ambient temperature (20–25 °C) and humidity (30–70%). All procedures complied with the animal care standards set forth by the National Institutes of Health and were approved by University of California Berkeley’s Administrative Panel on Laboratory Animal Care.
Light intensity calibration in brain
To calibrate the intensity of light applied to the brain for in vivo behavioral experiments with MP-D1ago, we followed a protocol similar that described for measuring blue light transmission through rodent cortex71. Because light transmission depends on wavelength72 and brain area73, we adjusted the protocol to measure the transmission of UV and blue light through striatal tissue. Mice were deeply anaesthetized with pentobarbital (200 mg/kg i.p.; Vortech) and then decapitated. Intracardial perfusion was not performed to avoid removing blood from the brain. Striatal tissue was excised and immediately placed in ice-cold artificial cerebrospinal fluid (ACSF) containing 50 mM sucrose, 125 mM NaCl, 25 mM NaHCO3, 2.5 mM KCl, 1.25 mM NaH2PO4, 0.1 mM CaCl2, 4.9 mM MgCl2, and 2.5 mM glucose (oxygenated with 95% O2:5% CO2). The tissue was then placed in an ACSF-filled petri dish directly above a power meter (Thorlabs) with a ~200 µM pinhole. Using a micromanipulator (Sutter), the tip of a fiber (200 µM, 0.22 NA) emitting 375 nm or 450 nm light was placed directly above the power meter pinhole and then progressively lowered in 200 µM steps through air or striatal tissue. Power intensity values of each wavelength at each depth were used to calculate % transmission, % initial power density, and light intensity at each depth.
The adeno-associated virus (AAV) encoding MEAAAK:ERE and mVenus or mVenus alone were made in the Isacoff lab. These cDNAs were inserted into an established Cre-dependent double-floxed inverted orientation (DIO) viral cassette under control of the CAG promoter and then packaged in the AAV5 capsid. The purified vectors contained 10 viral genomes/ml. The AAV encoding ChR2, AAV-EF1a-DIO-hChR2(H134R)-eYFP, was obtained from the UNC vector core.
All stereotaxic injections were performed under general ketamine–dexmedetomidine anesthesia using a stereotaxic instrument (Kopf Instruments, Model 1900). For AAV injections, 400 nL of concentrated viral solution was injected into either the dStr (bregma: 0.5 mm, lateral: ±1.9 mm, ventral: −3.0 mm), the NAc (bregma: 1.4 mm, lateral: ±1.0 mm, ventral: −4.1 mm), or the SNc (bregma: 3.3 mm, lateral: ±1.3 mm, ventral: −4.1 mm) using a syringe pump (Harvard Apparatus) at 150 nL/min. The injection needle was withdrawn 10 min after the end of each infusion. In some cases, immediately after viral injection mice were implanted with a bilateral guide cannula 0.5 mm dorsal to the injection site in the dStr or NAc. After injecting the ChR2 AAV into the SNc, a guide cannula was implanted in the dStr (bregma: 0.5 mm, lateral: ±1.9 mm, ventral: −2.5 mm). One layer of adhesive cement (C&B Metabond; Parkell) followed by cranioplastic cement (Dental cement) was used to secure the cannula to the skull. The incision was closed with tissue adhesive (Vetbond; 3 M). The animals were kept on a heating pad until they recovered from anesthesia. Experiments were performed 4–12 weeks after stereotactic injection. Injection sites and cannula placements were confirmed in all animals by preparing coronal or sagittal sections (50 μm) of the brain.
Open field test
The open field test was conducted to measure locomotor ability. Mice were placed in a custom-made white polycarbonate open field chamber (20 × 20 × 20 inches). Their movement was recorded with a video camera (Logitech) at ~20–30 Hz and analyzed using the video-tracking software Viewer3 (Biobserve). Mice were subjected to one or more of the following prior to or during the behavioral test: (i) intraperitoneal injection, (ii) striatal infusion using a combination of infusion cannulas and a syringe pump (200 nL/min; Harvard Apparatus), and (iii) light stimulation using optical cannulas (200 µM, 0.22 NA). See figure legends for specifics on the dosing used for each experiment. For all behavioral experiments wherein MP-D1ago was used, 1 nL of P-D1ago (100 µM) was infused into both hemispheres of the brain. In all cases, mice were habituated to infusion, optical fibers, and the open field chamber (15 min sessions) for two days prior to the test day.
The sub-second velocity traces recorded using Viewer3 were smoothed in MATLAB using a first order Butterworth filter (normalized cutoff frequency ωn = 0.02). Using original code written in MATLAB, a velocity threshold was manually set for each mouse to distinguish movements from tracking artifacts, as verified by visual inspection of each movie. The movement thresholds were similar across mice, e.g., the average threshold was 5.0 ± 0.7 cm/s for MP-D1ago mice and 4.9 ± 0.3 cm/s for ChR2 mice. Movement bouts were counted when the velocity surpassed this threshold and lasted for at least 0.3 s. Bouts were considered finished after the velocity remained below the manually defined threshold for 0.1 s. The percent time moving was calculated as the time that velocity was above the movement threshold divided by the time of the entire measurement. Movement initiation frequency was calculated as the number of times velocity surpassed the movement threshold per second. Movement bout duration was calculated by averaging the duration of all movement bouts that occurred during the entire measurement. Max velocity was calculated by averaging the maximum velocity of all movement bouts that occurred during the entire measurement.
Histology and confocal microscopy
After intracardial perfusion with 4% paraformaldehyde in PBS, pH 7.4, the brains were fixed overnight, placed in PBS with 30% sucrose for at least 24 h, and then sliced into 50 μm coronal or sagittal sections with a vibratome (Leica). The following primary antibodies were used: rabbit anti-HA tag (1:500; Cell Signaling), rat anti-D1R (1:500; Sigma-Aldrich), chicken anti-GFP/mVenus (1:1000; Abcam). The following secondary antibodies were used: goat anti-rabbit IgG-Alexa Flour 647 (1:750; Thermo Fisher Scientific), goat anti-rat IgG-Alexa 546 (1:750; Thermo Fisher Scientific), goat anti-chicken IgG-Alexa Flour 488 (1:1000; Thermo Fisher Scientific). Image acquisition was performed with a Zeiss LSM780 laser scanning confocal microscope using a 20× objective and on a Zeiss AxioImager M1 upright widefield fluorescence/differential interference contrast microscope with charge-coupled device camera using 5× objectives. Confocal images were collected using Zen Black 3.0 (Zeiss) and analyzed using Zen Blue 3.0 (Zeiss) and ImageJ. Sections were identified using landmarks and neuroanatomical nomenclature74. In some cases, AAV-injected mice received a dStr-infusion of 100 µM SNAP-Surface Alexa Fluor 647 (400 nL per hemisphere; NEB) followed by intracardial perfusion 24–48 h later.
Statistics and data analysis
Data were analyzed using GraphPad Prism (GraphPad), Clampfit (Axon instruments), Origin 8E (OriginLab), MATLAB R2020a, or ImageJ 1.52b software. For dose-response curves, data were normalized to vehicle (0%) and DA (100%) and nonlinear regression analysis was performed using the sigmoidal dose-response function in GraphPad Prism. Statistical analyses were performed using GraphPad Prism. All values reported are mean ± S.E.M.
Source data are provided with this paper. Additional data have been deposited in the Figshare repository under the filename MP-D_data.xlsx. MP-D1ago and D1-Cre mice are available upon request from the authors. Source data are provided with this paper.
The custom code written for this study are available in the GitHub repository under the filename BehavioralAnalaysis_Donthamsetti_2021.m.
Tritsch, N. X. & Sabatini, B. L. Dopaminergic modulation of synaptic transmission in cortex and striatum. Neuron 76, 33–50 (2012).
Wise, R. A. Dopamine, learning and motivation. Nat. Rev. Neurosci. 5, 483–494 (2004).
Schultz, W. Multiple dopamine functions at different time courses. Annu. Rev. Neurosci. 30, 259–288 (2007).
Stuber, G. D., Hnasko, T. S., Britt, J. P., Edwards, R. H. & Bonci, A. Dopaminergic terminals in the nucleus accumbens but not the dorsal striatum corelease glutamate. J. Neurosci. 30, 8229–8233 (2010).
Tritsch, N. X., Ding, J. B. & Sabatini, B. L. Dopaminergic neurons inhibit striatal output through non-canonical release of GABA. Nature 490, 262–266 (2012).
Howe, M. W. & Dombeck, D. A. Rapid signalling in distinct dopaminergic axons during locomotion and reward. Nature 535, 505–510 (2016).
Threlfell, S. et al. Striatal dopamine release is triggered by synchronized activity in cholinergic interneurons. Neuron 75, 58–64 (2012).
Cachope, R. & Cheer, J. F. Local control of striatal dopamine release. Front. Behav. Neurosci. 8, 188 (2014).
Marcellino, D., Kehr, J., Agnati, L. F. & Fuxe, K. Increased affinity of dopamine for D(2) -like versus D(1) -like receptors. Relevance for volume transmission in interpreting PET findings. Synapse 66, 196–203 (2012).
Dodson, P. D. et al. Representation of spontaneous movement by dopaminergic neurons is cell-type selective and disrupted in parkinsonism. Proc. Natl Acad. Sci. USA 113, E2180–E2188 (2016).
da Silva, J. A., Tecuapetla, F., Paixao, V. & Costa, R. M. Dopamine neuron activity before action initiation gates and invigorates future movements. Nature 554, 244–248 (2018).
Albin, R. L., Young, A. B. & Penney, J. B. The functional anatomy of basal ganglia disorders. Trends Neurosci. 12, 366–375 (1989).
DeLong, M. R. Primate models of movement disorders of basal ganglia origin. Trends Neurosci. 13, 281–285 (1990).
Kravitz, A. V. et al. Regulation of parkinsonian motor behaviours by optogenetic control of basal ganglia circuitry. Nature 466, 622–626 (2010).
Schiffmann, S. N., Lledo, P. M. & Vincent, J. D. Dopamine D1 receptor modulates the voltage-gated sodium current in rat striatal neurones through a protein kinase A. J. Physiol. 483, 95–107 (1995). Pt 1.
Surmeier, D. J. et al. Dopamine receptor subtypes colocalize in rat striatonigral neurons. Proc. Natl Acad. Sci. USA 89, 10178–10182 (1992).
Pacheco-Cano, M. T., Bargas, J., Hernandez-Lopez, S., Tapia, D. & Galarraga, E. Inhibitory action of dopamine involves a subthreshold Cs(+)-sensitive conductance in neostriatal neurons. Exp. Brain Res. 110, 205–211 (1996).
Carter, A. G. & Sabatini, B. L. State-dependent calcium signaling in dendritic spines of striatal medium spiny neurons. Neuron 44, 483–493 (2004).
Surmeier, D. J., Bargas, J., Hemmings, H. C. Jr., Nairn, A. C. & Greengard, P. Modulation of calcium currents by a D1 dopaminergic protein kinase/phosphatase cascade in rat neostriatal neurons. Neuron 14, 385–397 (1995).
Hernandez-Lopez, S., Bargas, J., Surmeier, D. J., Reyes, A. & Galarraga, E. D1 receptor activation enhances evoked discharge in neostriatal medium spiny neurons by modulating an L-type Ca2+ conductance. J. Neurosci.: Off. J. Soc. Neurosci. 17, 3334–3342 (1997).
Nisenbaum, E. S., Mermelstein, P. G., Wilson, C. J. & Surmeier, D. J. Selective blockade of a slowly inactivating potassium current in striatal neurons by (+/−) 6-chloro-APB hydrobromide (SKF82958). Synapse 29, 213–224 (1998).
Lahiri, A. K. & Bevan, M. D. Dopaminergic transmission rapidly and persistently enhances excitability of D1 receptor-expressing striatal projection neurons. Neuron 106, 277–290 (2020).
Dracheva, S. et al. Paradoxical locomotor behavior of dopamine D1 receptor transgenic mice. Exp. Neurol. 157, 169–179 (1999).
Mailman, R., Huang, X. & Nichols, D. E. Parkinson’s disease and D1 dopamine receptors. Curr. Opin. Investig. Drugs 2, 1582–1591 (2001).
Giorgioni, G., Piergentili, A., Ruggieri, S. & Quaglia, W. Dopamine D5 receptors: a challenge to medicinal chemists. Mini Rev. Med. Chem. 8, 976–995 (2008).
Abraham, A. D., Neve, K. A. & Lattal, K. M. Effects of D1 receptor knockout on fear and reward learning. Neurobiol. Learn Mem. 133, 265–273 (2016).
Drago, J. et al. Altered striatal function in a mutant mouse lacking D1A dopamine receptors. Proc. Natl Acad. Sci. USA 91, 12564–12568 (1994).
Nakamura, T. et al. Distinct motor impairments of dopamine D1 and D2 receptor knockout mice revealed by three types of motor behavior. Front Integr. Neurosci. 8, 56 (2014).
Ikegami, M., Uemura, T., Kishioka, A., Sakimura, K. & Mishina, M. Striatal dopamine D1 receptor is essential for contextual fear conditioning. Sci. Rep. 4, 3976 (2014).
Kelly, M. A. et al. Locomotor activity in D2 dopamine receptor-deficient mice is determined by gene dosage, genetic background, and developmental adaptations. J. Neurosci.: Off. J. Soc. Neurosci. 18, 3470–3479 (1998).
Urban, D. J. & Roth, B. L. DREADDs (Designer Receptors Exclusively Activated by Designer Drugs): chemogenetic tools with therapeutic utility. Annu. Rev. Pharmacol. Toxicol. 55, 399–417 (2015).
Airan, R. D., Thompson, K. R., Fenno, L. E., Bernstein, H. & Deisseroth, K. Temporally precise in vivo control of intracellular signalling. Nature 458, 1025–1029 (2009).
Ibanez-Tallon, I. et al. Tethering naturally occurring peptide toxins for cell-autonomous modulation of ion channels and receptors in vivo. Neuron 43, 305–311 (2004).
Schmidt, D., Tillberg, P. W., Chen, F. & Boyden, E. S. A fully genetically encoded protein architecture for optical control of peptide ligand concentration. Nat. Commun. 5, 3019 (2014).
Shields, B. C. et al. Deconstructing behavioral neuropharmacology with cellular specificity. Science 356, 2161 (2017).
Donthamsetti, P. C. et al. Genetically targeted optical control of an endogenous G protein-coupled receptor. J. Am. Chem. Soc. 141, 11522–11530 (2019).
Broichhagen, J. et al. Orthogonal optical control of a G protein-coupled receptor with a SNAP-tethered photochromic ligand. ACS Cent. Sci. 1, 383–393 (2015).
Levitz, J. et al. Dual optical control and mechanistic insights into photoswitchable group II and III metabotropic glutamate receptors. Proc. Natl Acad. Sci. USA 114, E3546–E3554 (2017).
Acosta-Ruiz, A. et al. Branched photoswitchable tethered ligands enable ultra-efficient optical control and detection of G protein-coupled receptors in vivo. Neuron 105, 446–463 e413 (2020).
Beharry, A. A. & Woolley, G. A. Azobenzene photoswitches for biomolecules. Chem. Soc. Rev. 40, 4422–4437 (2011).
Donthamsetti, P. C. et al. Optical control of dopamine receptors using a photoswitchable tethered inverse agonist. J. Am. Chem. Soc. 139, 18522–18535 (2017).
Gradinaru, V., Thompson, K. R. & Deisseroth, K. eNpHR: a Natronomonas halorhodopsin enhanced for optogenetic applications. Brain cell Biol. 36, 129–139 (2008).
Gunaydin, L. A. et al. Natural neural projection dynamics underlying social behavior. Cell 157, 1535–1551 (2014).
Boyden, E. S., Zhang, F., Bamberg, E., Nagel, G. & Deisseroth, K. Millisecond-timescale, genetically targeted optical control of neural activity. Nat. Neurosci. 8, 1263–1268 (2005).
Steiner, H. & Kitai, S. T. Regulation of rat cortex function by D1 dopamine receptors in the striatum. J. Neurosci.: Off. J. Soc. Neurosci. 20, 5449–5460 (2000).
Bjorklund, A. & Dunnett, S. B. Dopamine neuron systems in the brain: an update. Trends Neurosci. 30, 194–202 (2007).
Salamone, J. D., Correa, M., Farrar, A. & Mingote, S. M. Effort-related functions of nucleus accumbens dopamine and associated forebrain circuits. Psychopharmacology 191, 461–482 (2007).
Kelley, A. E., Baldo, B. A., Pratt, W. E. & Will, M. J. Corticostriatal-hypothalamic circuitry and food motivation: Integration of energy, action and reward. Physiol. Behav. 86, 773–795 (2005).
Rothwell, P. E. et al. Autism-associated neuroligin-3 mutations commonly impair striatal circuits to boost repetitive behaviors. Cell 158, 198–212 (2014).
Donthamsetti, P. et al. Arrestin recruitment to dopamine D2 receptor mediates locomotion but not incentive motivation. Mol. Psychiatry 25, 2086–2100 (2020).
Gore, B. B. & Zweifel, L. S. Genetic reconstruction of dopamine D1 receptor signaling in the nucleus accumbens facilitates natural and drug reward responses. J. Neurosci.: Off. J. Soc. Neurosci. 33, 8640–8649 (2013).
Phillips, G. D., Howes, S. R., Whitelaw, R. B., Robbins, T. W. & Everitt, B. J. Analysis of the effects of intra-accumbens SKF-38393 and LY-171555 upon the behavioural satiety sequence. Psychopharmacology 117, 82–90 (1995).
Plaznik, A., Stefanski, R. & Kostowski, W. Interaction between accumbens-D1 and accumbens-D2 receptors regulating rat locomotor-activity. Psychopharmacology 99, 558–562 (1989).
Patriarchi, T. et al. Ultrafast neuronal imaging of dopamine dynamics with designed genetically encoded sensors. Science 360, eaat4422 (2018).
Yano, H. et al. Gs- versus Golf-dependent functional selectivity mediated by the dopamine D1 receptor. Nat. Commun. 9, 486 (2018).
Beyene, A. G. et al. Imaging striatal dopamine release using a nongenetically encoded near infrared fluorescent catecholamine nanosensor. Sci. Adv. 5, eaaw3108 (2019).
Sun, F. et al. A genetically encoded fluorescent sensor enables rapid and specific detection of dopamine in flies, fish, and mice. Cell 174, 481–496 e419 (2018).
Menegas, W., Akiti, K., Amo, R., Uchida, N. & Watabe-Uchida, M. Dopamine neurons projecting to the posterior striatum reinforce avoidance of threatening stimuli. Nat. Neurosci. 21, 1421–1430 (2018).
Lerner, T. N. et al. Intact-brain analyses reveal distinct information carried by SNc dopamine subcircuits. Cell 162, 635–647 (2015).
Miyachi, S., Hikosaka, O., Miyashita, K., Karadi, Z. & Rand, M. K. Differential roles of monkey striatum in learning of sequential hand movement. Exp. Brain Res. 115, 1–5 (1997).
Miyachi, S., Hikosaka, O. & Lu, X. Differential activation of monkey striatal neurons in the early and late stages of procedural learning. Exp. Brain Res. 146, 122–126 (2002).
Luderman, K. D. et al. Identification of positive allosteric modulators of the D1 dopamine receptor that act at diverse binding sites. Mol. Pharmacol. 94, 1197–1209 (2018).
Lewis, M. A. et al. Discovery of D1 dopamine receptor positive allosteric modulators: characterization of pharmacology and identification of residues that regulate species selectivity. J. Pharmacol. Exp. Therapeutics 354, 340–349 (2015).
Svensson, K. A., Hao, J. & Bruns, R. F. Positive allosteric modulators of the dopamine D1 receptor: a new mechanism for the treatment of neuropsychiatric disorders. Adv. Pharm. 86, 273–305 (2019).
Zou, M. F. et al. Novel analogues of (R)-5-(Methylamino)-5,6-dihydro-4H-imidazo[4,5,1-ij]quinolin-2(1H)-one (Sumanirole) provide clues to dopamine D2/D3 receptor agonist selectivity. J. Med. Chem. 59, 2973–2988 (2016).
Zhu, K. et al. Antibody structure determination using a combination of homology modeling, energy-based refinement, and loop prediction. Proteins 82, 1646–1655 (2014).
Coordinators, N.R. Database resources of the National Center for biotechnology information. Nucleic acids Res. 45, D12–D17 (2017).
Friesner, R. A. et al. Glide: a new approach for rapid, accurate docking and scoring. 1. Method and assessment of docking accuracy. J. Med. Chem. 47, 1739–1749 (2004).
Trott, O. & Olson, A. J. Software news and update autodock vina: improving the speed and accuracy of docking with a new scoring function, efficient optimization, and multithreading. J. Comput Chem. 31, 455–461 (2010).
Michino, M. et al. What can crystal structures of aminergic receptors tell us about designing subtype-selective ligands? Pharmacol. Rev. 67, 198–213 (2015).
Aravanis, A. M. et al. An optical neural interface: in vivo control of rodent motor cortex with integrated fiberoptic and optogenetic technology. J. Neural Eng. 4, S143–S156 (2007).
Yizhar, O., Fenno, L. E., Davidson, T. J., Mogri, M. & Deisseroth, K. Optogenetics in neural systems. Neuron 71, 9–34 (2011).
Al-Juboori, S. I. et al. Light scattering properties vary across different regions of the adult mouse brain. PLoS ONE 8 (2013).
Franklin, K. B. J. & Paxinos, G. Paxinos and Franklin’s The mouse brain in stereotaxic coordinates. (2013).
We thank the members of the Isacoff and Lammel labs for helpful discussion. We also thank Helen Bateup (University of California, Berkeley) for generously providing the D1-Cre mice and much additional support. This work was supported by the National Institutes of Health (DA044696, P.D.; DA042889, S.L.; R01NS108151, D.T.; RF1MH123246, E.I. and D.T.). The McKnight Endowment for Neuroscience (048240; E.I. and D.T.), the European Research Council (268795; D.T.), and Weill Neurohub (E.I.).
The authors declare no competing interests.
Peer review information Nature Communications thanks the anonymous reviewer(s) for their contribution to the peer review of this work.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Donthamsetti, P., Winter, N., Hoagland, A. et al. Cell specific photoswitchable agonist for reversible control of endogenous dopamine receptors. Nat Commun 12, 4775 (2021). https://doi.org/10.1038/s41467-021-25003-w
This article is cited by
By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.