Amphetamines bind to the plasmalemmal transporters for the monoamines dopamine (DAT), noradrenaline (NET) and 5-HT (SERT); influx of amphetamine leads to efflux of substrates. Various models have been proposed to account for this amphetamine-induced reverse transport in mechanistic terms. A most notable example is the molecular stent hypothesis, which posits a special amphetamine-induced conformation that is not likely in alternative access models of transport. The current study was designed to evaluate the explanatory power of these models and the molecular stent hypothesis.
Xenopus laevis oocytes and HEK293 cells expressing human (h) SERT were voltage-clamped and exposed to 5-HT, p-chloroamphetamine (pCA) or methylenedioxyamphetamine (MDMA).
In contrast to the currents induced by 5-HT, pCA-triggered currents through SERT decayed slowly in Xenopus laevis oocytes once the agonist was removed (consistent with the molecular stent hypothesis). However, when SERT was expressed in HEK293 cells, currents induced by 3 or 100 μM pCA decayed 10 or 100 times faster, respectively, after pCA removal.
Conclusions and Implications
This discrepancy in decay rates is inconsistent with the molecular stent hypothesis. In contrast, a multistate version of the alternative access model accounts for all the observations and reproduces the kinetic parameters extracted from the electrophysiological recordings. A crucial feature that explains the action of amphetamines is their lipophilic nature, which allows for rapid diffusion through the membrane.
Amphetamine and its congeners act on the three closely related plasmalemmal monoamine transporters, that is the transporters for dopamine (DAT), noradrenaline (NET) and 5-HT (SERT) (Kristensen et al., 2011). The individual amphetamine-derived compounds differ in their affinity for specific transporters but their principal mechanism of action is identical: they bind to the outward facing conformation of the transporter and translocate together with Na+ and Cl− from the extracellular side into the cell interior (Rudnick and Wall, 1992; Sitte et al., 1998; Seidel et al., 2005).
Amphetamines induce substrate efflux (Rothman and Baumann, 2003; Hilber et al., 2005; Baumann et al., 2012) and most if not all of their biological actions are due to their ability to raise the extracellular levels of dopamine, NA and 5-HT. Increased monoamine efflux by amphetamines is caused by a combination of effects and not all of them occur at the level of the monoamine transporters; that is it is known that amphetamines increase cytosolic monoamine concentrations by the depletion of storage vesicles (Sulzer et al., 1993). The elevated cytosolic concentrations of monoamines are then thought to enhance the outwardly directed substrate flux through SERT, DAT or NET (Sulzer et al., 1995). Amphetamine-induced release is also known to be regulated by PKC and CaM-kinase-dependent phosphorylation (Gnegy, 2003; Seidel et al., 2005; Fog et al., 2006; Steinkellner et al., 2012). Phosphorylation of intracellular portions of the transporter is likely to affect the rate at which the transporter moves from the inward to the outward conformation. In fact, mutations within the N-terminus shift the transporter into the inward-facing conformation and hamper amphetamine-induced substrate efflux (Sucic et al., 2010). Several studies have proposed that amphetamines enhance and stabilize transporter conformations that are not induced by the native substrates (Petersen and DeFelice, 1999; Kahlig et al., 2005). A recent report described an (S+)-amphetamine-specific leak current observed in Xenopus laevis oocytes expressing DAT (Rodriguez-Menchaca et al., 2012). This current displayed peculiar features: it was induced by extracellular (S+)-amphetamine, but it did not require its continuous presence. In fact, it stayed activated long after (S+)-amphetamine had been removed from the solution, implying a long-lasting conformational change induced by amphetamine. DeFelice and coworkers termed this current a ‘shelf current’ and proposed a molecular stent hypothesis for amphetamine action, which invoked this persistent conductance as the pathway for efflux of accumulated substrate. Here, we observed that p-chloroamphetamine (pCA) induces SERT currents similar to the ‘shelf currents’ of (S+)-amphetamine-stimulated DAT. However, we showed that novel activities or conformational states of SERT are not required for these pCA-induced ‘shelf currents’ and that a recently established alternative access model (Schicker et al., 2011; Bulling et al., 2012) can adequately describe the action of pCA. Our observations suggest that pCA-induced ‘shelf currents’ are substrate-induced currents similar to those observed and described by other groups (Mager et al., 1994; Quick, 2003; Erreger et al., 2008). The reason that pCA-induced currents can appear to differ from currents triggered by 5-HT can be accounted for by the lipophilic nature of pCA.
Plasmids encoding hSERT were linearized and transcribed into RNA with a T7 RNA polymerase Kit mMessage mMachine (Ambion, Foster City, CA, USA). A total of 5 ng cRNA was microinjected into each oocyte. Electrophysiological recordings were performed 6–9 days following injection.
Xenopus laevis frogs (Nasco, Fort Atkinson, WI, USA) were anaesthetized with ethyl 3-aminobenzoate methanesulfonate (FLUKA A5040, Sigma Aldrich, Seelze, Germany) 2 mg mL−1 in H2O before the frogs were decapitated and the ovarian lobes removed and transferred to sterile Ca2+-free OR2 solution (82.5 mM NaCl, 2.5 mM KCl, 2 mM MgCl2, 10 mM HEPES, pH adjusted to 7.4 with NaOH). The lobes were manually dissected to produce groups of 5–10 oocytes and incubated in OR2, containing 1 mg mL−1 collagenase from Clostridium histolyticum (SIGMA, Sigma Aldrich). Forty-five to 60 min of incubation at 18°C were sufficient to digest and remove the follicular layer. Oocytes were then selected and transferred to a Ringer solution (100 mM NaCl, 2 mM KCl, 1.8 mM CaCl2, 1 mM MgCl2, 5 mM HEPES, pH adjusted to 7.6 with NaOH). Oocytes were kept at 18°C for a minimum of 2 h prior to injection. Injected oocytes were kept for 6–9 days at 18°C in a Ringer solution containing 2.5 mM Na+ pyruvate, 100 μg mL−1 penicillin, 100 μg mL−1 streptomycin. Solutions were changed daily.
Electrophysiological recordings in Xenopus laevis oocytes
A CA-1B high performance oocyte clamp (Dagan Corporation, Minneapolis, MN, USA) was employed for the measurements. The recorded signal was digitized with a Digidata 13222A (Axon Instruments, Sunnyvale, CA, USA). An Intel personal computer running pCLAMP 9.2 (Axon Instruments) was used for acquisition. Borosilicate glass capillaries were pulled to a final resistance of 0.4–1.2 MΩ and filled with 3 M KCl. Oocytes were impaled and the membrane potential was clamped to a holding potential of −60 mV. For continuous superfusion with ND100 solution (100 mM NaCl, 2 mM KCl, 1 mm CaCl2, 1 mM MgCl2, 10 mM HEPES, pH adjusted to 7.4 with NaOH), a gravity-driven superfusion system [Warner Instruments (Hamden, CT, USA), Eight Channel Perfusion Valve Control System (VC-8)] was used. Recordings were started after a stable current baseline had been established. The current was sampled with 100 Hz and low pass filtered with 20 Hz.
Whole-cell patch clamp
For patch clamp recordings, HEK293 cells stably expressing hSERT (Hilber et al., 2005) were seeded at low density for 24 h before measuring currents. To measure substrate-induced hSERT currents, cells were voltage clamped using the whole-cell patch clamp technique. Briefly, glass pipettes were filled with a solution consisting of 133 mM K-gluconate, 5.9 mM NaCl, 1 mM CaCl2, 0.7 mM MgCl2, 10 mM EGTA and 10 mM HEPES adjusted to pH 7.2 with KOH. For some experiments, the internal K+ concentration had to be reduced. In these instances, the pipette solution consisted of (mM) NMDG (163), MES (137), NaCl (5.9), CaCl2 (1), MgCl2 (0.7), HEPES (10), EGTA (10) pH 7.2.
The cells were continuously superfused with external solution 140 mM NaCl, 3 mM KCl, 2.5 mM CaCl2, 2 mM MgCl2, 20 mM glucose and 10 mM HEPES adjusted to pH 7.4 with NaOH. Currents were recorded at room temperature (20–24°C) using an Axopatch 200B amplifier and pClamp 10.2 software (MDS Analytical Technologies, Sunnyvale, CA, USA). Unless otherwise stated, cells were voltage clamped to a holding potential of −70 mV and 5-HT or pCA was applied for 5 s once every 60 s. Current traces were filtered at 1 kHz and digitized at 2 kHz using a Digidata 1320A (MDS Analytical Technologies). The liquid junction potential was calculated to be +16 mV and measurements were accordingly compensated. Drugs were applied using a DAD- 12 (Adams & List, Westbury, NY, USA), which permits complete solution exchange around the cells within 100 ms (Boehm, 1999). Current amplitudes in response to 5-HT application were quantified using Clampfit 10.2 software (Axon Instruments). Passive holding currents were subtracted and the traces were filtered using a 100 Hz digital Gaussian low pass filter.
Quantitative pCA measurements
Diffusion of pCA into uninjected Xenopus laevis oocytes was determined by adapting the method developed from measuring uptake of amphetamines into HEK293 cells (Seidel et al., 2005) as follows: single oocytes were incubated at room temperature in 1 mL ND100 solution containing 100 μM pCA. The respective incubation periods were 8, 16, 32, 64 128, 256 or 600 s. After incubation in pCA, the cells were transferred into 10 mL of a pCA free ND-100 solution and washed for 3 to 5 s. The oocytes were then transferred to an Eppendorf reaction tube. The carry-over of wash solution was about 20 μL. The sample was spiked with internal standard (50 ng of amphetamine) and pCA was extracted from the cell by addition of acetonitrile (0.25 mL). After centrifugation, the supernatant (0.15 mL) was mixed with an equal volume of aqueous solution (pH 9.2; final concentration, 15 mM Na2HPO4) containing dansyl chloride (6.25 μg, Serva Feinbiochemika, Heidelberg, Germany). After 20 min at 65°C, the samples were centrifuged to remove precipitated material; 0.15 mL were injected into an HPLC system and resolved at a flow rate of 1 mL min−1 at 50°C (mobile phase, 1:1; 30 mM KH2PO4, pH 6;.acetonitrile; column, Hewlett-Packard Hypersil MOS 200 _ 2.1 mm (Thermo Fisher Scientific Inc., Waltham, MA, USA); fluorescence detection, Shimadzu RF-551 Shimadzu, Kyōto, Japan; excitation and emission wavelength, 318 and 510 nm respectively).
We modelled the recorded currents utilizing a previously published kinetic model of the transport cycle of SERT. The time-dependent changes in state occupancies were evaluated by numerical integration of the resulting system of differential equations using Systems Biology Toolbox (Schmidt and Jirstrand, 2006) and MATLAB 2012a (Mathworks, Natick, MA, USA).
The voltage-dependence of individual rates was modelled according to Laeuger (1991) assuming a symmetric barrier as kij = k0ijexp(-zQijFV/2RT), with F = 96 485 Cmol−1, R = 8.314 JK−1 mol−1 and V the membrane voltage in volts and T = 293 K. The uncoupled current was modelled as a current through a Na+ permeable channel with I = PcγNC(V-Vrev), with Pc being the occupancy of the channel state, γ the single channel conductance of 2.4 pS (Lin et al., 1996), NC the number of channels, V the membrane voltage and Vrev the reversal potential of Na+ being +80 mV. The extra- and intracellular ion concentrations were set to the values used in the experiments. Extra- and intracellular substrate concentrations at the membrane interfaces – Sout (t) and Sin (t) – were modelled as described in the supplement.
All values are given as mean ± SD. The statistical significance of differences between groups was analysed using Mann–Whitney U-test. P-values <0.05 were considered to indicate statistical significance.
Assessment of pCA-induced currents in Xenopus laevis oocytes expressing hSERT
The deactivation of pCA-induced currents occurs more slowly than the deactivation of currents induced by the native substrate (5-HT)
Figure 1A and B show representative current traces recorded in Xenopus laevis oocytes expressing hSERT, measured using the two-electrode voltage clamp technique. The membrane voltage was clamped to −60 mV and 3 μM 5-HT was applied to the cell (Figure 1A); 5-HT provoked an inwardly directed current that reached a steady amplitude during the exposure time (10 s). Upon 5-HT removal, the current decayed exponentially to the initial level with a time constant of 5 s (this process is referred to as deactivation throughout the subsequent description). A current of similar size was induced when the same cell was challenged with 3 μM pCA (Figure 1B). However, after removal of pCA, the current deactivated about four times slower with a time constant of ∼20 s (Figure 1C).
The current amplitudes as a function of increasing 5-HT/pCA concentrations
Xenopus laevis oocytes clamped to a holding potential of −60 mV were challenged with increasing concentrations of pCA (Figure 2B). Application of lower concentrations (up to 10 μM) led to an increase in the measured current while higher concentrations led to inhibition. This is reflected in the bell-shaped concentration-response curve plotted in Figure 2A (closed circles). A concentration ramp of 5-HT (Figure 2A, open circles) was also associated with a reduction in current at higher concentrations; however, the inhibitory effect was less pronounced in the concentration range from 100 μM to 1 mM. These data show that pCA and 5-HT exert two effects on SERT: activation of a current at low and inhibition at higher concentrations. However, pCA was more potent at inhibiting the current.
‘Persistent’ current after removal of high pCA concentrations
DeFelice and coworkers observed a persistent current through DAT expressed in Xenopus laevis oocytes, when they challenged the transporter with (S+)-amphetamine and then removed (S+)-amphetamine from the solution. (S+)-amphetamine concentrations above 10 μM had to be applied to evoke this current. Here, we tested if SERT would also conduct a persistent current when challenged with pCA in a similar concentration range. A representative current trace is depicted in Figure 2C: The maximal current amplitude was induced by 10 μM pCA, followed by the application of 100 μM pCA. The current amplitude decreased in agreement with the concentration-response relation shown in Figure 2A. Upon removal of pCA, the current amplitude increased again, reaching a level comparable to that seen in the presence of 10 μM pCA. Thereafter, the current decayed slowly over 30 to 40 min. We stress that this decay was not observed when currents were monitored within a narrower time window, that is over a time scale of 10 to 100 s as is commonly used in most other studies of transporter-associated currents (Mager et al., 1994; Adams and DeFelice, 2003; Quick, 2003). In this narrower time range, the current appears to be persistent (Figure 2C, inset). DeFelice and coworkers showed that the ‘persistent’ current invoked by the removal of (S+)-amphetamine in DAT increased upon prolongation of the exposure to (S+)-amphetamine. In SERT, similar to DAT, the current contingent on pCA removal also changed in a time-dependent manner (Rodriguez-Menchaca et al., 2012). Figure 2D shows representative current traces that were recorded after different exposure times (i.e. after 4, 8 and 16 s). The applied pCA concentration was 100 μM in all instances. However, upon prolonged administration, pCA gave rise to currents that lasted longer.
Assessment of pCA-induced current properties in HEK293 cells expressing SERT
The data shown in Figures 1 and 2 were recorded from Xenopus laevis oocytes injected with SERT cRNA. We also recorded pCA- and 5-HT-induced currents in HEK293 cells stably expressing hSERT using patch clamp recordings in the whole cell configuration. As shown in Figure 3A (lower trace) 3 μM pCA induced an inwardly directed current in HEK293 cells clamped to −70 mV. Similar to the observation in oocytes, removal of pCA led to slow deactivation of the current. In further agreement with the recordings in oocytes, the time constant for 3 μM pCA was about five times slower than for 3 μM 5-HT (Figure 3A, upper trace). However, we also identified important differences. The most notable was found for the time course of current deactivation upon pCA removal: while the current decays were well described by a mono-exponential function in both HEK293 cells and Xenopus laevis oocytes, the absolute values of the time constants differed by ∼10-fold (compare Figures 1C and 3B).
Lack of ‘persistent currents’ upon removal of high concentrations of pCA in HEK293 cells
The kinetics of currents measured in HEK293 cells upon application of high pCA concentrations (>10 μM) differed substantially from those recorded in Xenopus laevis oocytes. While the latter exhibited only a steady current partially reduced by concentrations above 10 μM pCA (Figure 2B,C), currents measured in HEK293 cells upon application of high pCA concentrations were transient, as depicted in Figure 4A. After a brief initial peak, the current inactivated during a 5 s application of pCA and reached baseline values in the case of 100 μM. The time course of inactivation was fitted to a mono-exponential function, which yielded a time constant of about 230 ms at 100 μM pCA. It is important to note and it will be shown later that this transient component is different from the capacitive current previously described (Schicker et al., 2011). When current amplitudes were measured at the end of a 5 s exposure to different pCA concentrations, the resulting plots recapitulated the bell-shaped concentration-response curves found in Xenopus laevis oocytes (Figure 2A). We surmise that the lack of the transient component in Xenopus laevis oocytes was due to the slow solution exchange rates that can be achieved upon superfusion of oocytes; because of the large volume, wash-in of compounds is slow and rate-limiting. In contrast, solution exchange is rapid in patch clamp experiments with HEK293 cells allowing for superior time-resolved recordings. Recapitulating the findings in Xenopus laevis oocytes, the current showed an initial increase in amplitude upon removal of 30 μM or 100 μM pCA. However, following the initial peak, the current deactivated with a time constant of about 13 s after removal of 100 μM pCA. In contrast, as shown above, in oocytes the current decayed fully only after 30 to 40 min. This discrepancy is too large to be attributed to different solution exchange times. These data show that pCA did not induce persistent currents in HEK293 cells.
pCA-induced currents require internal K+
In a recent study, we demonstrated that 5-HT-induced currents through SERT are comprised of two components: utilizing a fast perfusion device, we observed an inwardly directed current peak followed by a steady current when SERT was challenged with 5-HT (Schicker et al., 2011). In the same study, we showed that removal of internal K+ suppressed the steady current but left the peak current unchanged. In the current study, we determined whether pCA-induced currents are similarly affected by the absence of internal K+. Figure 5 shows a representative current trace from a HEK293 cell clamped to −70 mV. At 100 μM, pCA elicited a peak current very similar to that previously observed with 5-HT (Schicker et al., 2011). This contrasts with the recording shown in Figure 4A (lower trace) where the same pCA concentration was applied but the intracellular solution in the patch electrode contained 164 mM K+. The comparison shows that pCA-induced currents were fully suppressed in the absence of K+, including the slowly deactivating current that had followed pCA removal. The peak current decayed with a time constant of about 70 ms (see inset Figure 5). This is considerably faster than the transient current shown in Figure 4A. Taken together, these data are consistent with the hypothesis that pCA- and 5-HT-induced currents are carried by the same conducting state.
Current inhibition at higher substrate concentrations is a consequence of internal substrate accumulation
In the original description of SERT-associated currents, Lester and coworkers observed current inhibition at external 5-HT concentrations exceeding 3 μM, but the underlying mechanism has remained elusive. In the present study, we addressed the mechanistic basis for this action of 5-HT. In principle, two mechanisms can be envisaged that result in decrease in current amplitude. The first encompasses a direct block of the conducting state by the substrate. This mechanism implies the presence of a second substrate-binding site of low affinity within the conduction pathway. The model posits that occupation of this site with substrate causes the current block. An alternative model assumes a change in the conformational equilibrium by internally accumulating substrate. This results in a reduced dwell time of SERT in the conducting state, because high internal substrate concentrations favour re-association of substrate to the internal substrate-binding site and thus impede progression through the transport cycle. Thus, by definition, high internal substrate alters the conformational equilibrium.
Figure 6A shows original traces of substrate currents induced at −70 mV by 30 and 100 μM methylenedioxyamphetamine (MDMA) respectively. MDMA induced a current that resembled the pCA current shown in Figure 4A. Similar to the pCA-induced current, the MDMA current first increased and then decreased rapidly reaching a new steady state within the application time (5 s). Similarly, application of 100 μM 5-HT also resulted in a current run-down, which, however, emerged more slowly and hence required a longer application period to reach steady state (Figure 6B-lower trace). Figure 6C shows a semi-logarithmic plot of the time constant of current inactivation (at 100 μM) as a function of the polar surface area (PSA) of each compound. The PSA, a good predictor of membrane permeability, is proportional to the energy term in the exponential of the rate constant (Reynolds et al., 1974; Baldwin, 2013). Thus, the observed linear relation in the semi-logarithmic presentation is consistent with the hypothesis that the current inactivation occurs as a consequence of substrate permeation into the cell. Figure 6D shows the unblocked fraction of 5-HT current at steady state for increasing concentrations of 5-HT. The extracted IC50 value around 100 μM are in good agreement with the IC50 value for internal substrate block determined by DeFelice and coworkers and the KM of 5-HT for the internal site (Sitte et al., 2001; Adams and DeFelice, 2003). This again suggests that the observed current inhibition at high substrate concentrations is caused by internal substrate accumulation. The rapid onset of current inactivation in the case of amphetamines suggested that there was substantial diffusion-driven uptake of pCA into oocytes. We tested this conjecture by assessing pCA diffusion directly: we measured uptake of pCA by uninjected Xenopus laevis oocytes. Single Xenopus laevis oocytes were exposed to 100 μM pCA, after a brief wash, the pCA level that remained in the oocyte was determined (see methods). Figure 6E shows the plot of pCA accumulated per oocyte as a function of the exposure time. These data were adequately described by an equation for a mono-exponential rise to equilibrium. Based on the parameter estimates, we calculated an equilibration time constant of about 135 s. It is worth noting that the calculated diffusion time of freely diffusing pCA is around 170 s 500 μm-1. Thus, given the diameter of an oocyte (500 to 1000 μm), the observations are consistent with the interpretation that the speed of equilibration is only limited by the velocity of free diffusion. Conversely, the findings also imply that the cell membrane does not impose a major diffusion barrier for pCA. These data are therefore again in agreement with the hypothesis that the rapid inactivation observed with pCA (see Figure 4A) is a consequence of amphetamine accumulation within the cell.
A model of SERT function in the presence of amphetamines
Recently, we established an alternative access model of SERT function that links transporter-associated currents to substrate translocation (Schicker et al., 2011). In this model, activation of currents by external substrates is associated with the formation of a K+ bound inward-facing conformation in equilibrium with the conducting state. The results of the present study suggest that, at high concentrations, external substrates exert inhibitory effects on the currents (Figures 2A, 4B). Although inhibition by extracellular substrates is not a feature of our model, current inhibition is predicted to occur at high internal substrate levels.
Upon inward transport, the internal substrate concentration is expected to rise over time. In previous studies (Schicker et al., 2011; Bulling et al., 2012), substrate application was modelled as a step function and the effect of internal substrate accumulation was ignored. However, in the case of amphetamines, concentrations of substrate on the cytoplasmic (Sin) and external (Sout) faces of the transporter are both expected to follow a complex time course, if passive diffusion through the membrane is taken into account. The respective substrate concentrations as a function of time [Sin(t) and Sout(t)] are critical factors for emulating current responses in our SERT model.
Here, we tested the hypothesis that 5-HT and pCA interact with SERT in an identical fashion (all parameters of the transport model kept unchanged) and that the observed differences between substrates (5-HT and pCA) and between HEK293 cells and Xenopus laevis oocytes can be attributed to internal reservoirs of accumulated amphetamine. Addressing this hypothesis requires a plausible model to predict Sin(t) and Sout(t). Accordingly, we formulated a model that included the following elements: (i) substrate fluxes through transporters and membranes, (ii) an external compartment subject to diffusion (unstirred layer), (iii) a stirred external compartment with infinite volume, and (iv) internal reservoir compartments with a plausible volume. We arranged all these elements as depicted in the scheme shown in Figure 7A. Realistic parameters (see Supplement) were extracted from the literature and the resulting system of differential equations was solved numerically. Two examples are shown in Figure 7B and C. In Figure 7B, 100 μM 5-HT was applied in silico for 5 s to an assumed HEK293 cell expressing SERT. The respective concentrations – Sout(t) and Sin(t) – predicted by our model are displayed. Sout(t) and Sin(t), give rise to the simulated current response I(t). The second example (Figure 7C) assumes a 5 s application of 100 μM pCA. Here, the respective concentrations over time differ, because Sin(t) ramps up faster to higher concentrations; this occurs as a consequence of passive diffusion through the membrane. The time course of Sout(t) and Sin(t) depicted gives rise to the calculated response I(t). Emulated current responses predicted by the model are shown in Figure 7D, E, F, H and I. Figure 7G displays the predicted pCA uptake into an uninjected Xenopus laevis oocyte. It is evident that the simulations match the corresponding currents determined in oocytes and cells respectively (compare Figure 1A, Figure 1B, Figure 2C, Figure 4A and Figure 4C).
Discussion and conclusions
Various hypotheses have been put forward to account for the ability of amphetamines to trigger efflux through monoamine transporters. These models fall into two categories: the first is based on the original concept of exchange diffusion (Fischer and Cho, 1979) and include variations that focus on the oligomeric arrangement of the transporter to explain transporter-mediated efflux (Seidel et al., 2005; Sitte and Freissmuth, 2010; Sucic et al., 2010). The alternative approach focuses on the capacity of amphetamines to induce channel-like activity in transporters (Sonders et al., 1997; Sitte et al., 1998; Kahlig et al., 2005). The recently proposed molecular stent hypothesis is an extension of the latter models (Rodriguez-Menchaca et al., 2012): it assumes the presence of a second binding site within the inner vestibule of the transporter. This site cannot be occupied by the cognate substrate but only by amphetamines, which were proposed to induce a long-lasting channel-like mode in the transporter. The principal argument in favour of this model was the observation of a long-lasting amphetamine-induced current (termed ‘shelf current’) through DAT that persisted after removal of extracellular amphetamine.
Here, we examined several predictions of these models on SERT. We also observed a long-lasting current through SERT that was seen only upon superfusion with pCA, but not with 5-HT. However, the decay kinetics depended on the nature of the cell in which the transporter was expressed. Upon removal of 100 μM pCA, the current disappeared 100 times more rapidly in HEK293 cells than in Xenopus laevis oocytes. The molecular stent hypothesis predicts that the deactivation kinetics are an intrinsic feature of the amphetamine binding site at the inner gate of the transporter rather than a property conferred onto the transporter by the cellular context.
In line with earlier observations (Gobbi et al., 2008), we observed a bell-shaped concentration-response curve: concentrations of pCA exceeding 10 μM resulted in progressively smaller currents. Furthermore, when pCA was completely removed from the bath solution, the current re-emerged. These observations are also difficult to reconcile with the core tenet of the molecular stent hypothesis, that is an amphetamine binding site at the inner gate. While our findings are not easily explained by the molecular stent hypothesis, they are consistent with an alternative access model.
Transporter-associated currents are a very sensitive readout because they allow for high temporal resolution. Accordingly, they monitor conformational changes in the transporter in real time. However, until recently, it was not clear how to understand the SERT-associated currents in the context of an alternative access model of substrate translocation. We identified the conformational state that gives rise to transport-associated currents and developed a mathematical model that provides a plausible kinetic description of SERT catalytic cycle (Schicker et al., 2011). In the inward-facing (K+-bound) conformation, SERT can apparently adopt a conducting state (TIKcond in Figure 7A). Monitoring the current thus allows for estimating the abundance of TIKcond.
Both pCA and 5-HT can enter into cells by passive diffusion. However, because of its lipophilicity, pCA (PSA = 26.02 Å2) diffuses across the membrane much faster than the more hydrophilic 5-HT (PSA = 59.14 Å2). If passive diffusion and intracellular accumulation of pCA are taken into account, this model recapitulates all pCA mediated currents. Because there is considerable passive pCA flux through membranes, pCA can accumulate in the cell at a much faster rate than 5-HT. If pCA is removed from the external solution, the cell serves as a reservoir. This allows for a continuous outward leak of pCA, which results in concentrations sufficient to trigger pCA-induced currents. This analysis also explains the persistent current observed in Xenopus laevis oocytes. The large size of oocytes provides a large intracellular reservoir. Accordingly, upon removal of pCA from the external solution, there is a long-lasting diffusion of pCA into the extracellular medium. Despite continuous superfusion, the unstirred layer of fluid above the cell surface suffices to inhibit immediate removal of pCA (Hille, 1977). Passive cytoplasmic accumulation of pCA also accounts for the pronounced current inhibition in the presence of high external pCA concentrations (Figures 2A, 4B). Consistent with our model [(Schicker et al., 2011); see also Figure 7A], occupation of the inward-facing conformation with a transported ligand should block the transport-associated current by forcing the transporter into the TIS state (Figure 7) (Adams and DeFelice, 2003; Erreger et al., 2008). The resulting rapid rise in internal pCA was detected in HEK293 cells due to the fast solution exchange rate achieved by our superfusion device. At high pCA concentrations, the inhibition occurred with a delay (compare with Figure 4A). It was preceded by a short-lasting current activation (corresponding to concomitant inward transport of pCA by SERT). In our model, the current decay is due to pCA entering the cytoplasm where it competes with K+ for the transporter and thereby inhibits the K+-dependent current.
The molecular stent hypothesis implies that amphetamine binding causes an arrest of the transport cycle, because once the transporter converts from the outward facing to the inward-facing conformation, amphetamines are proposed to stabilize a channel-like mode by binding to a site at the internal gate. Consequently, as long as the amphetamine is bound, the transporter would not undergo a transition to the outward facing conformation (TIK to TOK in our model). However, this transition is facilitated by antiport of K+ (Rudnick and Nelson, 1978; Nelson and Rudnick, 1979). Moreover, we find that intracellular K+ is required for pCA to induce persistent SERT currents (Figure 4A vs. Figure 5), strongly suggesting that these currents, like steady-state 5-HT currents (Schicker et al., 2011), are properties of a transporter intermediate from which substrate (pCA) has already dissociated. This conclusion is in direct opposition to the molecular stent hypothesis, which assumes that amphetamine-induced currents are carried by an intermediate to which amphetamine remains bound.
The present study examined pCA action on SERT. DeFelice and coworkers proposed their hypothesis based on observations in DAT (Rodriguez-Menchaca et al., 2012). Therefore, we also assessed the action of (S+)amphetamine on DAT in HEK293 cells. When we recorded (S+)amphetamine-induced currents we found no evidence for the presence of a persistent current (see Supporting Information Figure S1). Conversely, we observed currents that resembled those from SERT challenged with pCA, suggesting that our conclusions can be extended to DAT.
In the model presented above, we assumed that 5-HT, pCA and MDMA interact with SERT in an identical manner. We are aware that this is an oversimplification because substrates and various amphetamines differ in their affinities for SERT; in addition and more importantly, structure-activity relations indicate that modest structural changes affect the capacity of substituted amphetamines to act as releasers and/or competitive inhibitors of uptake (Rothman and Baumann, 2003). This indicates that the compounds differ in their affinities for the conformational states through which SERT proceeds during the transport cycle (i.e. outward facing, occluded and inward-facing conformation). In our opinion, this does not limit the validity of the model: it provides a framework for refining our understanding on how amphetamine and its congeners elicit their effects on SERT. Finally, the model can be extended to the other monoamine transporters and thus allow for defining how amphetamines discriminate between the three closely related transporters.
This work was supported by the Austrian Science Fund/FWF, grants F3506 to HHS, F3510 to MF and P22893-B1 to HHS & SB. We thank Gary Rudnick and Thomas Stockner for their helpful comments. We also thank Karl Koppatz and Martin Witek for their technical assistance with HPLC measurements.
Conflict of interest
The authors of this article have no conflict of interest.