Tph1−/− Mice Lack 5-HT in the Pancreas and Are Diabetic

Pancreatic 5-HT levels in Tph1−/− mice only reach 10% of the wild-type (wt) mean (Figure 1A) and neither pancreas mass (Tph1+/+: 150±30 mg, n = 27; Tph1−/−: 160±40 mg, n = 30) nor morphology, nor the number and size of islets differ between Tph1−/− and wt mice (Figure 1B and 1C). Concordant to the lack of peripheral 5-HT in Tph1−/− mice, they are hypersensitive to the satiety mediating effect of systemically applied 5-HT (Figure S1). In addition, the basal blood glucose concentrations in freely feeding mice are significantly elevated relative to those in wt mice (Figure 1D), while none of the other pancreatic markers in extensive serological screenings are altered in Tph1−/− mice (Table S1). The glucose levels are elevated as early as 14 d after birth in Tph1−/− mice and are maintained into young adulthood, indicating glucose intolerance. Concordantly, fasted Tph1−/− mice exhibited significantly higher blood glucose concentrations than wt animals in glucose tolerance tests (Figure 1E). Young adult Tph1−/− mice also present a mild insulin resistance (Figure 1F).

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Figure 1. Pancreata of Tph1−/− mice have a normal morphology but lack 5-HT, which results in hyperglycemia and insulin resistance.

(A) 5-HT contents in Tph1−/− and wt mice show, that Tph1−/− pancreata contain only around 10% of the wt mean. *p<0.05; n = 6. (B) Combined stacks of confocal images of pancreas slices spanning 10 µm with anti-insulin-stained islets (green) and anti-S100-stained ductal structures (red) at postnatal day 3 (P3) reveal no difference between the genotypes; scale bar = 70 µm. (C) Individual islets do not differ in morphometric analysis (Tph1−/−: n = 29; wt: n = 30). (D) Basal blood glucose concentration in freely feeding Tph1−/− mice are significantly reduced at P3 (Tph1−/−: n = 20; wt: n = 11) and elevated at P14 (n = 5) and in adulthood (n = 6) compared to wt littermates. *p<0.05. (E) Glucose tolerance tests with fasted wt and Tph1−/− mice show impaired glucose tolerance of the latter. *p<0.05; n = 6. (F) Insulin tolerance tests with Tph1−/− and wt mice. *p<0.05; n = 6. For (A) and (C–F), data are means ± SEM.

https://doi.org/10.1371/journal.pbio.1000229.g001

The glucose intolerance is comparable to the T2DM phenotype of 5-HT_2C receptor knockout mice [20] and occurs at a surprising young age between postnatal Days 3 and 14 (Figure 1D). Glucose tolerance tests with simultaneous glucose and insulin measurements then revealed a primary β-cell dysfunction in glucose-induced insulin secretion (Figure 2). The rise in blood glucose was significantly higher in the Tph1−/− mice 30 min after a glucose load (Figure 2A) and was not proportional to the initially elevated glucose level (difference significantly higher). The glucose load was also accompanied with a significantly shortened insulin secretion (Figure 2B), best seen at the difference. Therefore, glucose to insulin ratios (Figure 2C) were significantly increased in Tph1−/− before and after the glucose load, which indicates a β-cell dysfunction. This reaction was also observed in younger animals of both mixed and inbred genetic backgrounds (Figure S2). Moreover, the fasting glucose levels were increased by around 20% to 9.7 mM in the Tph1−/− aged 64–70 wk (Figure 2A). In conclusion, Tph1−/− mice are clearly diabetic, but the classification of the specific subtype of diabetes is difficult due to the lack of standardized mice-specific criteria. Nevertheless, such a phenotype, a primary β-cell dysfunction in glucose-induced insulin secretion with a monogenic inheritance and an early onset but with no loss of β-cell mass, would be classified as MODY in humans [21]. Therefore, one might speculate that TPH1 is a possible candidate gene for this metabolic disorder in humans, especially as a genetic diagnosis in at least 11% of European and as many as 70%–80% of Asian families with a diagnosis of MODY cannot be made, indicating that additional MODY-related genes need to be identified [22]–[24]. Nonetheless, follow-up screening of the TPH1 gene of unclassified MODY patients is to be performed in order to support this hypothesis.

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Figure 2. Intra- and extracellular 5-HT modulates insulin secretion in opposing directions.

(A–C) Diabetes mellitus and β-cell dysfunction in Tph1−/− mice aged 64 to 70 wk and rescue with 5-HTP. Glucose tolerance test with simultaneous blood glucose (A) and serum insulin (B) measurements. Glucose to insulin ratios (C) are significantly increased in Tph1−/− without 5-HTP treatment before and after the glucose load. *p<0.05; n = 8 (wt and Tph1−/− + 5-HTP) and n = 6 (Tph1−/−). (D) Pargyline induces hyperglycemia in wt mice. After a meal of 60 min, mice were treated with pargyline (75 mg kg⁻¹) and blood glucose was measured immediately and after additional 60 min. *p<0.05; n = 6. (E) Pargyline treatment substantially elevated insulin secretion in wt mice. Mice were treated as described in (D). *p<0.05; n = 6. (F) Glucose tolerance test of Tph1−/− and wt mice with systemic 5-HT pre-treatment. *p<0.05; n = 6. (G) Extracellular 5-HT inhibits insulin secretion in MIN-6, INS-1, and RINm5F insulinoma cells. Cells were treated with 5-HT (500 µM) at the beginning of a 60 min secretion period. Insulin secretion is normalized to glucose-induced control cells. *p<0.05; n = 4. (H) Insulin secretion of RINm5F cells with or without glucose and 5-HTP (500 µM; 3 h) or pargyline (20 µM; 3 h). *p<0.05; n = 3. All data are presented as means ± SEM.

https://doi.org/10.1371/journal.pbio.1000229.g002

Interestingly, Tph1−/− mice thrive normally [13],[25], and they live as long as their wt littermates (mean life expectancy: 113 wk; n = 37; χ² = 0.98). We consider these findings to be particularly important, since diabetes mellitus, if left untreated, significantly curtails life expectancy [21],[26]. Especially the development of secondary damage like cardiovascular disease is the major cause for morbidity and mortality in diabetes. We have previously demonstrated that Tph1−/− mice are less prone to succumb to vessel occlusion in experimental thromboembolism and thrombosis due to a reduced primary haemostatic response [13]. This beneficial protective side effect of the lack of 5-HT decreases cardiovascular complications in Tph1−/− mice and seems to mild the severity of their diabetes. The general differences between mouse and man hamper a direct translation of findings between these species. Nevertheless, one might speculate that therapeutic peripheral 5-HT reduction specifically in thrombocytes [13],[27], together with blood glucose management, can also ameliorate vascular disease and its complications in diabetic patients. This concept for future work could possibly open new avenues to improve quality of life and to prolong life expectancy of diabetic patients.

Extra- and Intracellular 5-HT Modulates Insulin Secretion in Opposing Directions

To further elucidate the role of 5-HT in diabetes, we took advantage of well-established pharmacological possibilities for manipulating intracellular 5-HT levels (Figure S3). Application of 5-hydroxytryptophan (5-HTP), the immediate precursor of 5-HT (Figure S3A), increases the intracellular 5-HT level, bypassing the rate-limiting biosynthesis step [6],[11],[28]. Indeed, this treatment normalized the blood glucose levels and largely rescued the deficient insulin secretion in the Tph1−/− mice (Figure 2A and 2B).

In addition to the use of 5-HTP to increase intracellular 5-HT, pargyline, which blocks the 5-HT catabolism [6], can also be used for this purpose (Figure S3A). Systemic application of pargyline leads to a rapid hypoglycemic and hyperinsulinemic response in mice [29], suggesting that intracellular 5-HT enhances insulin secretion. If intracellular 5-HT plays such an enhancing role in insulin secretion, then pargyline application should have no effects in Tph1−/− mice, which lack 5-HT. Concordantly, pargyline induced hypoglycemia (Figure 2D) and an acute rise in plasma insulin (Figure 2E) exclusively in wt but not in Tph1−/− mice.

We then investigated glucose homeostasis after a systemic 5-HT application 30 min prior to the glucose load in fasted mice, in order to explore the extracellular role of 5-HT. In these tests, mice of both genotypes had largely elevated blood glucose levels (Figure 2F) compared to mice without pre-treatment (Figure 1E). This suggests that extracellular 5-HT has an inhibitory influence on insulin secretion as noted previously [30], most likely acting via the sole known 5-HT receptor of β-cells, the 5-HT_1A receptor.

The effect of extracellular 5-HT on insulin secretion of β-cells was further investigated using the insulin-secreting cell lines MIN-6, INS-1, and RINm5F [31],[32], which all exhibit responsiveness to glucose-stimulation (Figure 2G). Indeed, extracellular 5-HT inhibited glucose-induced insulin secretion in all three β-cell lines. One has to take into account that β-cells take up 5-HT via the plasma membrane SERT into the cytoplasm [7],[9],[10]. Therefore, 5-HT might also partially act intracellularly in this experiment. But since the incubation with 5-HT was short, its action can be attributed mostly to extracellular mechanisms.

Moreover, elevated levels of intracellular 5-HT would rather not inhibit but enhance the glucose-mediated insulin secretion, as seen by 5-HTP and pargyline treatment of insulinoma cells (Figure 2H). The stronger effect of 5-HTP found in these tests is supported by our finding that 5-HTP rises the intracellular 5-HT concentration to a higher extent than pargyline treatment (Figure S4). High intracellular 5-HT levels seem to be involved in the control of basal secretion as well, as 5-HTP slightly enhances insulin secretion from RINm5F cells also under non-stimulatory conditions (Figure 2H). The hyperinsulinemic effect of the above-mentioned compounds that increase intracellular 5-HT levels is in accordance with the results in vivo (Figure 2B and 2E), further supporting a crucial role for intracellular 5-HT as a modifier of insulin secretion.

Impaired Secretory Activity from β-Cells in Adult Tph1−/− Mice

To directly test the hyposecretory phenotype, we monitored secretion from Tph1−/− and wt β-cells by whole-cell patch-clamp measurements of membrane capacitance in fresh pancreas slices, taking advantage of the fast time resolution of electrophysiological techniques [33]. The resting membrane capacitance, electrical coupling between neighboring cells, and the amplitude of high voltage-activated Ca²⁺ channels (VACC) did not differ significantly between the Tph1−/− and wt β-cells (Figure S5). Nevertheless, the secretory response in Tph1−/− β-cells was significantly impaired when triggered by depolarization trains and measured as a cumulative increase in membrane capacitance (Figure 3A). Impaired secretion can also be due to impaired function of high VACC, but we found that peak amplitude of high voltage-activated (HVA) Ca²⁺ currents were not significantly different (Figure S5A). However the amplitude of low voltage-activated (LVA) Ca²⁺ currents was prominently increased in Tph1−/− compared to wt β-cells (Figure S5B). The β-cell electrical activity in Tph1−/− cells seems to be activating at lower glucose concentration (Figure 3B), which likely results from the increased LVA Ca²⁺ current amplitudes we observe in these mice (Figure S5B), because increased T-type currents are known to lower the threshold for action potential firing in insulinoma cells (INS-1) and non-obese diabetic mice [34],[35]. As the HVA current amplitudes were not significantly impaired, we conclude that the secretory impairment is not due to lower Ca²⁺ influx. Next we tested the impairment of the secretory response downstream of the Ca²⁺ influx. Slow UV photo-release of caged Ca²⁺ increased intracellular Ca²⁺, which peaked after about 5 s and reached a steady state value after 10 s (Figure 3C, lower panel). When free Ca²⁺ exceeded about 2 mM, a biphasic response in membrane capacitance was triggered. The amplitude of the fast component was comparable in both phenotypes, whereas the amplitude of the slow component was significantly reduced in Tph1−/− (Figure 3C, upper panel; for statistics see Figure S6). To test the direct role of 5-HT, we either incubated isolated β-cells with 5-HTP for 24 h or infused 5-HT through the patch pipette. While 5-HTP treatment partially restores the capacitance response, infusion of 5-HT completely rescued the reduced secretory phenotype (Figure 3C, upper panel). We conclude that the secretory lesion does not involve the coupling of the secretory machinery to either VACCs or Ca²⁺ sensors but interferes with the recruitment and exocytosis of the dense-core vesicles. The process is fast since the cell dialysis with 5-HT rescues the phenotype within a few minutes.

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Figure 3. Impaired exocytosis of Tph1−/− β-cells and rescue with 5-HT.

(A) A train of 50 depolarizing pulses from −80 to +10 mV for 40 ms at 10 Hz induced changes in the membrane capacitance of wt (n = 24) and Tph1−/− (n = 19) β-cells. Data are shown as means ± SEM. (B) Representative current-clamp recordings of the electrical activity of wt and Tph1−/− β-cells in pancreas tissue slices. The slices were perfused with solutions containing different glucose concentrations as indicated in the bar below the traces. (C) Representative membrane capacitance response of isolated wt and Tph1−/− β-cells (top panel) stimulated by ramp [Ca²⁺]_i change induced by slow photo-release of caged Ca²⁺ (bottom panel). The impaired component exocytosis has been partially rescued by extracellular 5-HTP (500 µM, 24 h) and completely restored by pipette intracellular dialysis with 5-HT.

https://doi.org/10.1371/journal.pbio.1000229.g003

Serotonylation Modulates Insulin Secretion

In thrombocytes, intracellular 5-HT serves as a substrate for protein serotonylation (Figure 4A), which modifies the trafficking of proaggregatory α-granules and results in their exocytosis [13]. Thus, we asked whether serotonylation is also involved in the β-granule transport and exocytosis. We first confirmed that RINm5F and β-TC3 cells readily take up [³H]-5-HT (Figure 4B and 4C), as previously described for other insulinoma cell lines and islets [7],[9],[10]. The uptake has a similar kinetic in both cell lines, leveling off approximately 90 min after addition of [³H]-5-HT. Under these conditions, we detected covalent [³H]-5-HT incorporation into the protein fraction in both cell lines, revealing a massive serotonylation of proteins. This serotonylation was sensitive to the potent TGase inhibitor cysteamine in both cell lines, demonstrating that the reaction is TGase-dependent. More importantly, cysteamine also curtailed the glucose-stimulated insulin secretion in MIN-6 insulinoma cells (Figure 4D), as well as in INS-1 and RINm5F cells (Figure S7). These results are in line with the reduced insulin secretion of primary β-cells from rat treated with either the TGase inhibitor monodansylcadaverin (MDC) [36] or cysteamine [37] and the reduced insulin release and the MODY phenotype of TGase2−/− mice [16]. Thus, protein serotonylation is unequivocally detectable in β-cells and it modulates insulin secretion. Nonetheless, the further elucidation of signaling cascades regulating or interfering with this novel mechanism is an obvious issue that has to be clarified in follow-up studies.

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Figure 4. Inhibition of protein serotonylation reduces insulin secretion.

(A) Scheme of protein serotonylation of glutamine residues by TGase. Cysteamine (CTA) and monodansylcadaverin (MDC) are potent inhibitors of TGases. (B and C) Uptake and protein incorporation of [³H]-5-HT in β-TC3 (B) and RINm5F cells (C) in the presence of CTA (500 µM; 3 h). *p<0.05; n = 3. (D) Insulin secretion from MIN-6 cells in the presence of CTA (500 µM; 3 h). *p<0.05; n = 4. (E) Proteasomal degradation of serotonylated proteins in RINm5F cells at different glucose concentrations in the presence or absence of the proteasomal inhibitor LLnL (50 µM; 3 h).*p<0.05; n = 4. (F) Immunoblot of serotonylated (5-HT) and total (5xHis) 6xH-Rab3a (white arrowhead) and 6xH-Rab27a (black arrowhead) prepared from glucose-stimulated RINm5F cells treated with 100 µM MDC, 200 µM CTA, or vehicle. Shown is one representative experiment out of three repetitions. (G) Quantification by Ni-NTA pull-downs of 6xH-Rab3a and 6xH-Rab27a from glucose-stimulated RINm5F cells incubated with [³H]-5-HT and either 50 µM LLnL or vehicle. *p<0.05; n = 3. Vector, vector-transfected control. For (B–E) and (G), data are means ± SEM.

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Unexpectedly, the [³H]-5-HT incorporation rates in glucose-stimulated and non-stimulated RIN5mF cells did not differ (Figure 4E). However, it is now well-established that small GTPases constitutively activated by TGases are marked for proteasomal degradation by ubiquitination [14]. Concordantly, inhibition of the proteasome with calpain inhibitor I (LLnL) significantly accumulated serotonylated proteins only in the presence of glucose (Figure 4E), suggesting that with an increased insulin secretion, there is a faster cycling between activation by serotonylation and inactivation by proteasomal degradation.

Rab3a and Rab27a Become Serotonylated during Glucose-Mediated Insulin Secretion

Previously, GTPases have been found to be targets for serotonylation in other tissues [13],[14], prompting us to test two GTPases crucially involved in insulin secretion as putative targets in β-cells; Rab3a regulates replenishment of the ready releasable pool of β-granules by recruiting calmodulin to the resting pool at early stages of vesicle transport [38]. Rab27a acts directly in the targeting of β-granules from the resting pool to the ready releasable pool at the plasma membrane [19]. To confirm their serotonylation during insulin secretion, we expressed 6xHis-tagged Rab3a and Rab27a in RINm5F cells (Figure S8), which express all components for serotonylation (Figure S9). Indeed, both GTPases become serotonylated within these cells in a TGase-dependent manner, as the TGase inhibitors MDC and cysteamine both blocked this reaction (Figure 4F). In addition, using radiolabeled [³H]-5-HT, we quantified the serotonylation of these GTPases (Figure 4G). LLnL enriched serotonylated Rab3a but not Rab27a, showing that proteasomal degradation is the mechanism of inactivation of Rab3a, at least at the selected time point, as shown for serotonylated RhoA [14]. The difference between the two GTPases could reflect different kinetics of inactivation by proteasomal degradation, suggesting a high selectivity of this process. While Rab3a-deficient mice present with glucose intolerance, transfection of insulinoma cells with constitutively active Rab3a was shown to inhibit insulin release by accumulating and retaining the vesicles in the ready releasable pool [17]. Hence, the continuous secretion seems to demand a rapid cycling of Rab3a between an active and inactive state. In contrast, constitutively active Rab27a has been shown to increase insulin release [39]. Thus, it could be of physiological relevance to serotonylate Rab27a to a higher extent and stability than Rab3a in order to promote continuous β-granule exocytosis.

The data presented here suggest a model in which TGase is activated by the increase of intracellular Ca²⁺ that occurs upon glucose stimulation (Figure 5). TGases then use intracellular 5-HT to serotonylate Rab3a and Rab27a, likely amongst a set of diverse other yet to be identified target proteins, as suggested by the massive serotonylation observed in β-cells (Figure 4B and 4C). This renders them constitutively active and promotes insulin secretion. The serotonylated GTPases become inactivated by ubiquitin-dependent proteasomal degradation at different rates, which is analogous to the recently described inactivation of serotonylated RhoA [14].

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Figure 5. Proposed model of 5-HT-induced exocytosis of β-granules from glucose-stimulated β-cells.

The classic sequel of glucose transport, glucose oxidation and ATP generation, ATP-gated potassium channel closure, membrane depolarisation, and Ca²⁺ influx via voltage-dependent calcium channels is represented in the upper part of the scheme. Amongst other functions, Ca²⁺ activates TGases that serotonylate a variety of proteins. In the β-cell, Rab3a, and Rab27a, which are crucially involved in the exocytosis of insulin, are target signaling proteins that become activated by this mechanism. Insulin and 5-HT co-secretion is the consequence. While insulin then exerts its endocrine function, 5-HT acts via an autocrine/paracrine loop. Initially, high extracellular 5-HT concentrations [5-HT]_e attenuate further insulin secretion through 5-HT_1A receptors, with progressive weakening of this effect by the clearance of [5-HT]_e via uptake through the plasma membrane SERT. Eventually, [5-HT]_i reaches much higher levels than [5-HT]_e, promoting another event of insulin secretion by serotonylation. This 5-HT-dependent cycling between inhibition and induction might contribute to the well-known oscillating nature of insulin exocytosis from glucose-stimulated β-cells.

https://doi.org/10.1371/journal.pbio.1000229.g005

This model is in line with the well-known pulsatile insulin secretion with a frequency of about one to five per minute, which is accompanied by synchronous intracellular Ca²⁺ oscillations [40]. These Ca²⁺ oscillations that are likely paralleled by intracellular 5-HT oscillations fulfill the conditions required for serotonylation of GTPases [13]. Furthermore, our data are in accordance with the phenotype of TGase2−/− mice, which also present a reduced β-cell function [16]. Thus, inactivation of the catalyzing enzyme TGase2 [16], a lack of the monoamine substrate for serotonylation (Tph1−/−), and the absence of the protein substrates Rab3a and Rab27a [18],[19] all lead to defective insulin secretion independently. These findings support an essential function of serotonylation for insulin exocytosis.

The data presented here assign a mechanistic role to the 5-HT contained in β-granules as a substrate for the serotonylation of proteins involved in insulin secretion. Our model, in which signaling protein serotonylation strengthens the function of the exocytotic machinery, shows striking resemblance to the process in thrombocytes [13]. Our findings suggest that serotonylation is a modifier mechanism in the high clinical variability of diabetes and may have an impact on future therapeutic concepts. If confirmed in other monoamine-rich cells, such as histaminergic or catecholaminergic neurons, this study has not only elucidated a key role of 5-HT in β-cells but also may contribute to change more general concepts about monoamine functions, adding another posttranslational modification to the repertoire of signaling.

Animal Experiments

Animals were held under standardized conditions on a mixed genetic 129/SvEvBrd × C57BL/6 background as previously described [13],[25]. In order to ensure that Tph1−/− and Tph1+/+ do not genetically drift away from each other, they were periodically interbred to obtain Tph1+/−, which were then used to re-establish Tph1−/− and Tph1+/+ to refresh the breeding colony, as generally recommended for mixed genetic backgrounds [41]. At the beginning of physiological experiments, the mice were at the F₁₁-generation of interbreeding. In addition, Tph1−/− were backcrossed to the inbred strain C57BL/6 until the F₈-generation and compared with the mixed genetic background. All phenotypical aspects were the same in the 129/SvEvBrd × C57BL/6 and the inbred C57BL/6 Tph1−/−. Pancreas extracts and whole blood samples for the determination of 5-HT contents were obtained and analyzed as described [25],[42]. For glucose and insulin measurements, blood of barbital sodium-anaesthetized animals was obtained from the vena cava inferior, the retrobulbar plexus, or by severing the tail tips. Glucose was immediately measured using a B-glucose analyzer (HemoCue) and insulin in serum or cell culture supernatants was quantified by insulin ELISA (Mercodia). Mice were fasted for 24 h prior to tolerance tests. Glucose (2 g kg⁻¹), insulin (0.75 U kg⁻¹), 5-HT (4 mg kg⁻¹) or pargyline (75 mg kg⁻¹) was injected intraperitoneally. Blood for serum preparation was collected from the vena cava inferior as described [13]. The serological analysis was performed at the animal clinic laboratory VetMedLab GmbH, Division of IDEXX Laboratories Inc. (Ludwigsburg, Germany). Peripheral 5-HT levels for rescue experiments were replenished by subcutaneous injections with 5-HTP as described [11].

Pancreas Slices, Immunostaining, and Electrophysiology

The agarose embedded tissue (Seaplaque GTG agarose, BMA, Walkersville) was cut to 140 µm thick slices. During slicing and after the preparation, the tissue was kept in an ice-cold extracellular solution (125 mM NaCl, 2.5 mM KCl, 26 mM NaHCO₃, 1.25 mM Na₂HPO₄, 2 mM sodiumpyruvate, 0.25 mM ascorbic acid, 3 mM myo-inositol, 6 mM lactic acid, 1 mM MgCl₂, 2 mM CaCl₂ and 3 mM glucose) adjusted to pH 7.3 by gassing with carbogen (95% O₂, 5% CO₂) for at least 30 min. The slices were transferred to carbogen-bubbled extracellular solution at 32°C 30 min before experiments. For primary β-cell culture, liberase (0.3 g L⁻¹) (Roche) was dissolved in HBSS (Invitrogen) and injected into pancreas via the bile duct. The pancreas was removed and digested for 10–15 min at 37°C, centrifuged, and then hand picked [43]. Isolated islets were trypsinized into single cells, plated onto coverslips, and cultured in RPMI 1640 medium supplemented with 10% fetal bovine serum (Invitrogen) and antibiotics. The cultured β-cells were used within 3 d. For immunostaining, cells were incubated overnight at 4°C with anti-insulin and anti-S100 antibodies followed by anti-mouse Alexa 488 and anti-rabbit Alexa 647 for 1 h at room temperature. The fluorescence was acquired using a confocal microscope (Leica TCS SP2 AOBS) at 488 and 633 nm. The images were processed for morphometrical analysis using Leica confocal software. Pancreatic β-cells were identified by the characteristic half maximal inactivation of voltage-activated Na⁺ currents (approx. −100 mV) [44]. The pipette filling solution used in depolarization protocols, isolation of Ca²⁺ currents and current-clamp experiments on β-cells in slices contained 127 mM Cs-methanesulfonate, 8 mM CsCl, 10 mM Hepes (pH 7.2; CsOH), 2 mM MgCl₂, 0.05 mM EGTA, 20 mM TEACl, and 4 mM ATP-Na₂ (see [44] for details of the analysis). The pipette filling solution used in photo-release experiments on isolated β-cells contained 125 mM CsCl, 40 mM Hepes (pH 7.2; CsOH), 2 mM MgCl₂, 0.05 mM EGTA, 20 mM TEACl, 2 mM ATP-Na₂, 5 mM NP-EGTA (Molecular Probes), 4.5 mM CaCl₂, and 0.1 mM Fura-6 (Molecular Probes). The perfusion chamber was mounted on an upright microscope (×60 water, NA 0.9, Eclipse E600FN, Nikon, Japan). All experiments were performed on a SWAM II C dual-phase lock-in patch-clamp amplifier (Celica, Ljubljana). Data were filtered at 3 kHz by an A/D converter (National Instruments). Recording, stimulation, and preliminary analysis were performed using the WinWcp software (v3.52, John Dempster, University of Strathclyde, UK). Patch pipettes were pulled (P-97; Sutter Instruments, USA) from borosilicate glass capillaries (GC150F-15; WPI, USA) to a resistance of 2–5 MΩ in pipette solution as reported previously. All currents were analyzed and presented after p/n leak subtraction. To estimate changes in membrane capacitance, the piecewise linear technique was used (1.6 kHz sine-wave frequency, 11 mV RMS amplitude). Secretory activity was triggered by elevations of cytosolic Ca²⁺. To manipulate Ca²⁺, we used depolarizing trains or continuous photo-release (Polychrome IV, Till Photonics) of caged Ca²⁺ (NP-EGTA). For data analysis and figure preparation, we used Matlab, Matview (Matlab WinWCP extension, Wise Technologies, Ljubljana), Sigmaplot, and Sigmastat (SPSS, Chicago, IL, USA).

Cell Culture

Rat insulinoma cell line INS-1 was a generous gift from Claes B. Wollheim (University Medical Center, Geneva), and mouse MIN-6 cells were kindly provided by Franz Schaefer (University Heidelberg) and cultured as described [31],[32]. RINm5F cells were grown as previously described [45] in RPMI1640 (Invitrogen) containing 11.1 mM glucose supplemented with 10% fetal bovine serum (Biochrom) and antibiotics.

Insulin Secretion Assays

Insulinoma cells were cultured in Primaria plates (Falcon) 72 h before the experiment and pretreated with 5-HTP, pargyline, or cysteamine as indicated in the figure legends. The cells were washed twice in glucose-free growth medium supplemented with dialyzed serum to remove 5-HT and sensitized to glucose for 30 min in glucose-free medium and stimuli. Next, cells were stimulated for 60 min with or without 25 mM glucose in KRBH (136 mM NaCl, 4.7 mM KCl, 1.2 mM MgSO₄, 1 mM CaCl₂, 1.2 mM KH₂PO₄, 5 mM NaHCO₃, 10 mM HEPES, and 0.5% BSA, pH 7.4) in presence of indicated stimuli. We used KRBH to avoid any disturbances by compounds present in normal medium and/or serum (e.g., 5-HT). The supernatant was collected, centrifuged, and used for insulin ELISA as described above.

Molecular Biological and Analytical Methods

All cloning procedures, PCR, and immunoblotting were conducted according to standard protocols or to the manufacturer's instructions. 6xH-Rab constructs were generated using Rab3a and Rab27a cDNAs [13] that were reamplified with 5′-primers containing an ATG within a Kozak consensus sequence followed by six histidine codons and a stretch of 22 specific nucleotides for each cDNA. Stable transfection of RINm5F cells was conducted with linearized constructs and the transfectants were selected at 50 µg mL⁻¹ G418 for at least 4 wk.

Quantitative Serotonylation Assay

TGase-mediated 5-HT protein incorporation was assessed culturing confluent 12 well tissue culture plates for the indicated period in the presence of 1 µCi [³H]-5-HT. After harvesting and three extensive washing steps with PBS, the cells were homogenized in ice-cold 300 mM PCA. Protein was collected by centrifugation and the supernatant was measured in a scintillation counter (Beckman) in 5 mL ReadyProtein scintillation cocktail (Beckman) to assess for the total [³H]-5-HT uptake. The protein pellets were washed four times with 300 mM PCA, boiled in 200 µL 10% SDS, and sample radioactivity was determined as above. Quantitative affinity precipitations were performed with cells grown in glucose-stimulation medium for 4 h in the presence of 1 µCi [³H]-5-HT. Lysates were obtained with Ni-NTA lysis buffer pH 8.0 (50 mM NaH₂PO₄, 300 mM NaCl, 10 mM imidazole, protease inhibitors w/o EDTA, 1% NP40, 1% Triton X-100, and 0.1% SDS). After separation of the debris by centrifugation, binding of 6xH-tagged Rabs was conducted with an excess of Ni-NTA magnetic beads (Qiagen; 20 µL beads/cells harvested from a confluent 12 well tissue culture cavity) and overhead turning at 4°C overnight. The beads were then washed three times (50 mM NaH₂PO₄ pH 8.0, 300 mM NaCl, 8 mM imidazole, protease inhibitors w/o EDTA, and 0.05% Tween 20) and used for quantification as above.

Statistical Analyses

All data are presented as mean ± SEM and p values are from two-tailed Student's t tests type 3. Values of p<0.05 were considered as statistically significant.