, Volume 53, Issue 7, pp 1428–1437

Beta cell coupling and connexin expression change during the functional maturation of rat pancreatic islets


  • C. P. F. Carvalho
    • Department of Histology and Embryology, Institute of BiologyUniversity of Campinas (UNICAMP)
  • H. C. L. Barbosa
    • Department of Physiology and Biophysics, Institute of BiologyUniversity of Campinas
  • A. Britan
    • Department of Cell Physiology and Metabolism, Medical SchoolUniversity of Geneva
  • J. C. R. Santos-Silva
    • Department of Histology and Embryology, Institute of BiologyUniversity of Campinas (UNICAMP)
  • A. C. Boschero
    • Department of Physiology and Biophysics, Institute of BiologyUniversity of Campinas
  • P. Meda
    • Department of Cell Physiology and Metabolism, Medical SchoolUniversity of Geneva
    • Department of Histology and Embryology, Institute of BiologyUniversity of Campinas (UNICAMP)

DOI: 10.1007/s00125-010-1726-8

Cite this article as:
Carvalho, C.P.F., Barbosa, H.C.L., Britan, A. et al. Diabetologia (2010) 53: 1428. doi:10.1007/s00125-010-1726-8



Cell–cell coupling mediated by gap junctions formed from connexin (CX) contributes to the control of insulin secretion in the endocrine pancreas. We investigated the cellular production and localisation of CX36 and CX43, and gap junction-mediated beta cell coupling in pancreatic islets from rats of different ages, displaying different degrees of maturation of insulin secretion.


The presence and distribution of islet connexins were assessed by immunoblotting and immunofluorescence. The expression of connexin genes was evaluated by RT-PCR and quantitative real-time PCR. The ultrastructure of gap junctions and the function of connexin channels were assessed by freeze–fracture electron microscopy and tracer microinjection, respectively.


Young and adult beta cells, which respond to glucose, expressed significantly higher levels of Cx36 (also known as Gjd2) than fetal and newborn beta cells, which respond poorly to the sugar. Accordingly, adult beta cells also showed a significantly higher membrane density of gap junctions and greater intercellular exchange of ethidium bromide than newborn beta cells. Cx43 (also known as Gja1) was not expressed by beta cells, but was located in various cell types at the periphery of fetal and newborn islets.


These findings show that the pattern of connexins, gap junction membrane density and coupling changes in islets during the functional maturation of beta cells.


Beta cellsCell–cell couplingConnexinsGene expressionDevelopmentGap junctionInsulin secretionMaturationPancreatic islet





Lucifer Yellow


When compared with adult islets, fetal and neonatal islets from different species exhibit a reduced secretory response to glucose and other secretagogues [18]. The nature of this poor responsiveness is not fully understood, and has been variably attributed to many factors, including fuel metabolites, intracellular signals, hormones and other environmental conditions [13, 811].

Cell–cell contacts mediated by gap junctions are crucial for a proper secretory response of the endocrine pancreas. The synthesis and release of insulin are markedly altered after dispersion of beta cells in vitro, but rapidly recover after cell reaggregation, indicating that the secretory mechanism depends on intercellular interactions within the pancreatic islet [12, 13]. Several in vivo and in vitro studies have demonstrated that insulin secretion stimulated by glucose and other secretagogues is associated with increased gap junction coupling of beta cells, whereas the pharmacological blockage of gap junction channels impairs the secretory function of beta cells [9, 1416]. Thus, loss of connexin 36 after treatment of beta cell lines with antisense oligonucleotides or knocking out the gene (Cx36 [also known as Gjd2]) in mice resulted in loss of beta cell coupling, associated with a loss of synchronisation of intracellular calcium oscillations, as well as altered basal and glucose-stimulated insulin secretion [1720]. Together, these findings point to the importance of gap junction-mediated cell coupling in beta cell physiology.

The role of gap junctions in the developmental maturation process of beta cell function has not been evaluated. In this work we investigated the expression and localisation of the gap junction-associated connexins CX36 and CX43 and the ultrastructural and functional aspects of the intercellular channels which connexins form in pancreatic islets of rats of different ages. Our findings reveal a close relationship between the degree of maturation of the insulin secretory machinery, notably insulin expression and glucose-induced insulin secretion, and CX36-dependent coupling in rat pancreatic islets.



Fetuses (embryonic day 20) and neonatal (1–2 days old) male and female Wistar rats and young (21 days old) and adult male (3–4 months old) Wistar rats were obtained from the breeding colony of the University of Campinas (Campinas, Brazil) or from the University of Geneva (Geneva, Switzerland). The animals were used in accordance with the guidelines of the Institutional Committee for Ethics in Animal Experimentation of the University of Campinas and the University of Geneva.


The cellular locations of connexins, insulin, glucagon and vimentin were determined by immunofluorescence staining of sections of pancreas frozen in n-hexane with liquid nitrogen, and cryosectioned (8 μm). For the detection of CX36, insulin, glucagon and vimentin, the sections were fixed with acetone at −20°C for 3 min. For CX43 detection, the sections were fixed with 2% paraformaldehyde (wt/vol. in PBS, pH 7.4) for 8 min and permeabilised with 0.1% Triton X-100 (vol./vol. in 0.05 mol/l Tris-buffered saline [TBS], pH 7.4) for 5 min. All sections were then incubated for 1 h with 5% dry skimmed milk (wt/vol. in TBS, pH 7.4) and then with the primary antibodies under the conditions listed in Table 1 of the Electronic supplementary material (ESM). Following incubation with the corresponding fluorochrome-labelled secondary antibody (ESM Table 1), the sections were mounted with Vectashield (Vector Laboratories, Burlingame, CA, USA) and observed using a confocal laser-scanning microscope (MRC 1024 UV; Bio-Rad Laboratories, Hercules, CA, USA; or LSM 510 META; Zeiss, Hamburg, Germany). To compare the different animal groups, islets from fetal, neonatal, young and adult animals were analysed during the same session using identical confocal parameters. The specificity of the primary antibodies was tested by omitting them and by incubating the sections in 3% dry skimmed milk (wt/vol. in TBS). These negative controls did not result in consistent labelling of islet cells (data not shown).

Islet isolation

Islets were isolated by type V collagenase digestion (EC; Sigma) of fetal, neonatal, young and adult pancreas in Hanks’ balanced salt solution and, after separation with Ficoll gradients or Histopaque 1077 (Sigma, St Louis, MO, USA), were collected under a dissecting microscope. To minimise contamination by exocrine tissue, fetal and newborn islets were cultured for 24 h in RPMI-1640 medium supplemented with 5% fetal bovine serum (vol./vol.), 10 mmol/l glucose, 100 IU penicillin/ml and 100 μg streptomycin/ml at 37°C in a 5% CO2/air atmosphere. Most experiments tested freshly isolated young and adult islets. However, for comparison with fetal and neonatal islets, some freeze–fracture and quantitative real-time PCR experiments also investigated adult islets after culture. No marked difference in terms of Cx36 expression and gap junction numbers was observed between freshly isolated and cultured adult islets (data not shown).

Insulin secretion

Five to 15 overnight-cultured islets from fetal, neonatal, young and adult rats were placed in 1 ml Eppendorf tubes and preincubated for 30 min at 37°C in 0.5 ml bicarbonate-buffered Krebs solution containing 3 mg/ml bovine serum albumin/ml and equilibrated to pH 7.4 with a mixture of 95% O2 and 5% CO2 (BBKS) [9] supplemented with 5.6 mmol/l glucose. The islets were then incubated for 1 h at 37°C in 0.5 ml BBKS supplemented with either 2.8 or 16.7 mmol/l glucose. Aliquots of the supernatant fraction were stored at −20°C. Secreted insulin was determined by RIA and expressed as ng islet−1 h−1 [9].

Western blotting

Pools of at least 1,000 islets isolated from each animal group were homogenised by sonication in an antiprotease cocktail [9]. The total protein content of the lysates was determined using a DC protein assay kit (Bio-Rad). Aliquots (70 μg) of each group were incubated for 1 h at 37°C with 30% of the total volume made with 5× concentrated Laemmli sample buffer [9]. The samples were then fractionated by electrophoresis in 10% polyacrylamide gels and the proteins were electrotransferred to nitrocellulose membranes (Bio-Rad). The membranes were stained with Ponceau S solution (Sigma) and immunoblotted only when showing comparable staining of corresponding bands. Selected membranes were blocked overnight at 4°C with TBS containing 0.05% (vol./vol.) Tween 20 plus 5% (wt/vol.) dry skimmed milk. They were then incubated with the primary antibodies followed by incubation with their respective specific secondary antibody conjugated with horseradish peroxidase (HRP) [9] under the conditions given in ESM Table 2. After washing the membranes, the membranes were revealed using an enhanced chemiluminescence kit (SuperSignal West Pico Chemiluminescent Substrate; Pierce, Rockford, IL, USA) and autoradiography film (Amersham, Cleveland, OH, USA). Band intensities were quantified by optical densitometry using Image software (Scion, Frederick, MD, USA). The densitometric values of connexin signals were expressed relative to those of all proteins stained with Ponceau S, which were taken as 100%. The specificity of antibodies was confirmed in brain and heart homogenates, used as positive controls for CX36 and CX43, respectively. Liver tissue, which was used as a negative control, showed, as expected, no signal for CX36 and a relatively weak band for CX43 (data not shown).


Pools of approximately 1,000 islets were lysed in 1 ml Trizol solution (Invitrogen, Carlsbad, CA, USA), and total RNA was extracted as described by the manufacturer. RNA concentrations were determined by measuring the optical absorbance at 260 nm. cDNA was synthesised from 3 μg islet RNA in a volume of 20 μl, using the reverse transcriptase SuperScript II and random hexamer primers (Invitrogen, USA). The primer sets used in RT-PCR analysis are shown in ESM Table 3. The number of amplification cycles was defined for each gene after titration between 18 and 42 cycles, using RNA islet samples from all animal groups in a PCR Thermal Cycler 9600 (PerkinElmer Cetus, Waltham, MA, USA). In all cases, negative controls were provided by submitting a sample of water to amplification (data not shown). PCR products were separated on 2% ethidium bromide–agarose gels, and band intensities were determined by digital scanning (GelDoc 2000; Bio-Rad) followed by quantification using Scion Image software. The Cx43 and Cx36 transcript levels were normalised to those of ribosomal protein S29 (Rps29).

Quantitative PCR

Pools of 200–400 isolated neonatal and adult islets were lysed in a guanidinium thiocyanate solution and total RNA was extracted using the RNAqueous-Micro kit (Ambion, Austin, TX, USA). mRNAs (0.5 µg) were reverse-transcribed using ImProm-2 Reverse transcription system (Promega, Madison, WI, USA). RNA integrity was checked using a 2100 Bioanalyzer (Agilent, Santa Clara, CA, USA), and quantitative PCR was performed with a 7900H Sequence Detection System (Applied Biosystems, Foster City, CA, USA). The primers are listed in EMS Table 4. Each transcript was evaluated in triplicate. Mean values were normalised to the mean geometric value of the housekeeping genes Rps29, Gapdh and Eef1a1.

Freeze–fracture electron microscopy

Isolated neonatal and adult islets were fixed for 60 min in 2.5% glutaraldehyde solution (vol./vol.) and processed for freeze–fracturing [16, 21] using a BAF 60 Freeze Etching System (Balzers High Vacuum, Balzers, Liechtenstein). Replicas were examined with a Philips CM10 electron microscope. To evaluate beta cells, we only considered membrane profiles located in the islet centre and surrounded by cytoplasm displaying secretory granules [21]. Gap junctions and tight junctions were identified by their characteristic appearance [16]. Membrane and junction areas were photographed and measured using UTHSCSA Image Tool software (http://ddsdx.uthscsa.edu/dig/itdesc.html, version 3.0).

Tracer microinjection

Neonatal and adult islets were attached to Sylgard- (Dow Corning, Midland, MI, USA) and poly-l-lysine-coated dishes as previously described [22], transferred to the heated stage (37°C) of a Universal Zeiss microscope and kept in Krebs Ringer bicarbonate HEPES buffer (117 mmol/l NaCl, 4.7 mmol/l KCl, 2.5 mmol/l CaCl2, 1.2 mmol/l MgSO4, 1.2 mmol/l KH2PO4, 5.0 mmol/l NaHCO3, 10 mmol/l HEPES), 0.5% (wt/vol.) BSA and 10 mmol/l glucose, pH 7.3–7.4, after equilibration with O2/CO2 (95:5, vol./vol.). Individual cells located in the islet centre were impaled using glass microelectrodes filled with a 4% solution (wt/vol.) in 150 mmol/l LiCl (pH 7.2) of either Lucifer Yellow (LY; mol. wt 457, two negative charges) or ethidium bromide (mol. wt 394, one positive charge; wt/vol.), without altering the islet shape. After cell penetration, the tracers were injected iontophoretically for 5 min by applying 0.1 nA square pulses of 900 ms duration and 0.5 Hz frequency. Pulses were negative for injection of LY and positive for ethidium bromide. In all cases, the extent of diffusion was captured with an Axiocam camera (Carl Zeiss, Oberkochen, Germany) coupled to the fluorescence microscope. The extent of coupling was determined by measuring the area labelled by each tracer on digitised photographs of the intact islets, using Image Tool software. The islets were then fixed in 4% paraformaldehyde (wt/vol. in 0.1 mol/l phosphate buffer). Some of them were embedded in Epon (EMS, Hatfield, PA, USA), serially sectioned (1 μm) and processed for checking the location of the injection site [22].

Statistical analysis

Results are expressed as mean ± SEM. For comparison between groups, statistical significance was assessed using Student’s t test. For multiple comparisons, statistical significance was assessed by ANOVA followed by the Bonferroni test. The χ2 test was used to compare the coupling incidence in adult and neonatal islets. The significance level was set at p < 0.05. Statistical analyses were performed using the GraphPad Prism Version 4.00 for Windows (GraphPad Software, La Jolla, CA, USA).


Fetal, neonatal and young islets had a similar basal release of insulin in the presence of 2.8 mmol/l glucose (0.3 ± 0.1 [n = 10], 0.1 ± 0.02 [n = 22] and 0.2 ± 0.05 [n = 10] ng islet−1 h−1 respectively), which was lower (p < 0.001) than that of adult islets (1.1 ± 0.2 ng islet−1 h−1, n = 24). When stimulated with 16.7 mmol/l glucose, fetal and neonatal islets did not significantly increase their insulin release (0.5 ± 0.5 [n = 10] and 0.3 ± 0.1 [n = 24] ng islet−1 h−1, respectively), whereas young and adult islets increased it (1.9 ± 0.4 [n = 10] and 9.5 ± 0.8 [n = 22] ng islet−1 h−1 respectively; p < 0.001). As a result, the fold increase in insulin release was significantly greater in young and adult islets compared with fetal and neonatal islets (Fig. 1).
Fig. 1

Beta cells acquire glucose responsiveness after birth. Fetal and neonatal islets did not show significantly higher insulin secretion compared with the basal value observed in the presence of 2.8 mmol/l glucose (white bars) when exposed to 16.7 mmol/l glucose (black bars), whereas young and adult islets did. Values are mean + SEM fold increase over basal mean value (set to 1) of ten (fetal and young islets) to 24 experiments (neonatal and adult islets). p < 0.0001 vs basal value (2.8 mmol/l glucose) within each group

The beta cells of young and adult islets showed substantial punctate staining for CX36, which was much less evident in fetal and neonatal islets (Fig. 2). Blots confirmed that young and adult islets has higher levels of CX36 compared with fetal and neonatal islets (Fig. 2). A different pattern was observed for CX43. Thus, beta cells were not immunostained for this CX, whereas the same antibodies labelled vimentin-positive, duct and alpha cells at the periphery of fetal and neonatal islets (Fig. 3). Blots showed that whereas fetal and neonatal islets produced two forms of CX43, the form of lower electrophoretic mobility was preferentially detected in young and adult islets (Fig. 3).
Fig. 2

CX36 production increases during development of rat pancreatic islets. a–h Confocal views of immunolabelled CX36 (green, a–d) and insulin (red, e–h) in fetal (a, e), neonatal (b, f), young (c, g) and adult (d, h) islets. The punctate CX36 distribution in beta cells is evident in young and adult islets, but much less in fetal and neonatal islets. Scale bar, 50 µm. i–k Sonicates of isolated islets (i) were immunoblotted for CX36 (j). The protein was mostly detected in its dimeric (66 kDa) form (j). k Densitometric evaluation revealed a marked postnatal increase in CX36 relative to all proteins stained by Ponceau S (i). Values are mean + SEM of seven membranes from four independent experiments. M, molecular weight markers; F, fetus; N, neonatal; Y, young; A, adult. *p < 0.05 vs neonatal and fetal values

Fig. 3

Beta cells do not produce CX43 throughout the development of rat pancreatic islets. a–h Confocal views of immunolabelled CX43 (green, a–d) and insulin (red, e–h) in fetal (a, e), neonatal (b, f), young (c, g) and adult islets (d, h). No CX43 was immunodetected in beta cells throughout islet development. In contrast, antibodies to CX43 immunostained some cells (arrows) at the periphery of fetal (a, e) and neonatal islets (b, f). i–k Triple labelling for CX43 (green), insulin (blue) and either vimentin (red in i, j) or glucagon (red in k) confirmed that the antibodies to CX43 did not stain beta cells (i), but appeared to stain vimentin-positive (i, arrow), duct (j, arrow) and alpha (k) cells at the periphery of a neonatal islet. Scale bars, 50 µm (a–h); 25 µm (i–k). l, m Islet sonicates (l) were immunoblotted for CX43. The protein was detected as two bands in fetal and neonatal islets, whereas the lower mobility form was detected in young and adult islets (l). m Densitometric evaluation revealed a marked postnatal decrease in CX43 relative to all proteins stained by Ponceau S (l). The difference in CX43 levels between fetal and neonatal islets did not reach statistical significance. Values are mean + SEM of five membranes from three independent experiments. M, molecular weight markers; F, fetus; N, neonatal; Y, young; A, adult. **p < 0.01 vs neonatal value

RT-PCR showed that the levels of Cx36 mRNA increased (p < 0.001) with islet development, whereas those of Cx43 decreased (p < 0.05) in parallel (Fig. 4). Quantitative PCR confirmed the opposite changes in the two connexins, and further showed that the levels of Cx36 mRNA increased in parallel with those of mRNAs for both the insulin 1 and the insulin 2 gene (Cx36 vs insulin 1, r2 = 0.9232, p < 0.0001; Cx36 vs insulin 2, r2 = 0.9748, p < 0.0001; Fig. 5).
Fig. 4

Transcription of Cx36 and Cx43 genes changed inversely during islet development. a, b Amplicons detected at different cycles in fetal, neonatal, young and adult islets, using primers for Cx36 (a) and Cx43 (b). c, d Quantitative evaluation of these amplicons showed that the levels of Cx36 mRNA increased with islet development, whereas those of Cx43 mRNA decreased in parallel. Data are mean+SEM normalised to the levels of Rps29 mRNA for three independent experiments. ***p < 0.001 (c); *p < 0.05 (d) vs fetal and neonatal values

Fig. 5

Cx36 and insulin gene expression were correlated in neonatal and adult rat islets. a, b Quantitative PCR confirmed that the levels of Cx36 mRNA were higher in adult than neonatal islets, whereas those of Cx43 mRNA were lower. Data are mean + SEM normalised to the levels of Rps29, Gadph and Eef1a1 mRNAs for three independent experiments. e, f When related to the levels of mRNA expression of both the insulin 1 (Ins1) and the insulin 2 (Ins2) gene, which also increased with islet development (c, d), a significant (p < 0.0001) correlation was found between the expression of Cx36 and insulin mRNAs in neonatal (triangles) and adult (squares) islets. ***p < 0.001 vs neonatal value

Freeze–fracture electron microscopy showed that beta cells of both adult and neonatal islets displayed typical gap junctions, often associated with tight junctions (Fig. 6). However, the proportion of beta cell membranes showing gap junctions was higher (p < 0.0001) in adult than in neonatal islets, because of a 3.5-fold increase in the numerical density of gap junctions (Table 1).
Fig. 6

Gap junctions connected beta cell membranes within neonatal and adult rat islets. Freeze–fracture electron microscopy revealed gap junction plaques in the beta cell membranes of both adult (a, b) and neonatal (c, d) islets. Gap junctions were often found associated with tight junction fibrils (a, c). Scale bar, 120 nm

Table 1

Morphometric analysis of junctions in neonatal and adult rat pancreatic islets


No. of membranes examined (μm2)

No. of membranesa

Type of junction

No. of gap junctions per 100 μm2

With gap junctions

Without gap junctions

Gap junction

Gap + tight junction

Tight junction


78 (976)



4 (8.9%)

22 (48.9%)

19 (42.2%)



72 (1000)



23 (13.8%)

70 (42.2%)

73 (44.0%)


Ten replicates from two independent pools of about 100 islets were analysed per group

ap < 0.0001 for the distribution of junctions between neonatal and adult islets, as evaluated by the χ2 test

Microinjection of islets with either LY or ethidium bromide revealed coupling of beta cells in both neonatal and adult islets (Fig. 7). The extent of LY diffusion did not change significantly with islet development, whereas that of ethidium bromide was greater (p < 0.01) in adult than in neonatal islets. Under these conditions, adult islets less frequently displayed uncoupled beta cells and more frequently (p < 0.01) displayed territories comprising at least seven coupled beta cells compared with neonatal islets (Fig. 7). Fetal and neonatal islets showed a similar coupling pattern (LY diffusion, neonatal 619.2 ± 78.48 μm2 [n = 43], fetal 504.4 ± 137.2 μm2 [n = 7]; ethidium bromide diffusion, neonatal 847.1 ± 42.6 μm2 [n = 34], fetal 842.0 ± 131.0 μm2 [n = 10]).
Fig. 7

Beta cell coupling changed with development of rat pancreatic islets. ad Microinjection of neonatal (a, c) and adult intact islets (b, d) with either LY (a, b) or ethidium bromide (c, d) resulted in variable transfer of tracers into adjacent beta cells. In both islet types, the extent of ethidium bromide transfer was greater than that of LY, consistent with the presence of CX36 but not CX43 channels. Scale bar, 50 μm. e Quantitative analysis showed that whereas LY transfer (white bars) did not change significantly with islet development, the exchange of ethidium bromide (black bars) was greater (p < 0.01) in adult than neonatal islets. f Comparison of the coupling rank order between LY (white columns) and ethidium bromide (black columns), i.e. the number of beta cell diameters labelled by ethidium bromide, revealed that adult islets had fewer uncoupled cells (one cell) and more frequent territories comprising more than seven coupled beta cells than neonatal islets. Data in e are mean + SEM of the number of islets indicated above the columns. **p < 0.01 vs neonatal, LY; ***p < 0.001 vs adult, LY


The ability to recognise increasing concentrations of glucose as a graded stimulus for acute insulin release is a unique and major characteristic of pancreatic beta cells. It has long been known that this glucose responsiveness is normally established in the few days that follow birth, even though beta cells are already equipped in the late prenatal period with most of their adult features [38]. Several events occurring during the early neonatal period, including changes in K+ membrane permeability, production of GLUT2, protein kinase C-alpha, Ca2+ channels and key enzymes of the NADH shuttles, are implicated in the maturation of beta cell function [1, 2, 48, 2325]. We now show that gap junction/CX36 signalling, which contributes significantly to the proper function of adult beta cells [17, 18, 26, 27], is another key event in the final maturation of this function.

Here we provide the first evidence that structural and functional changes in gap junctions take place between beta cells in parallel with their developmental secretory maturation. Specifically, we have found that fetal and newborn rat beta cells express a similar pattern of gap junctions and coupling that is quite different from that observed in both young and adult animals. Thus, fetal and newborn beta cells, which respond poorly to glucose stimulation, produced little CX36, the native gap junction protein of adult beta cells [18, 22, 28], and were modestly coupled to each other. These features changed after birth. Thus, glucose-responsive young and adult rat islets featured increased levels of CX36 as a result of transcriptional activation of the cognate gene, and greater functional beta cell coupling, particularly when tested with positively charged tracers that preferentially permeate CX36 channels [22, 29].

Increasing evidence points to a requirement for adequate levels of CX36 and of the cell-to-cell channels this protein makes, to establish/retain appropriate insulin secretory in response to glucose stimulation [1820]. Thus, loss of Cx36 results in increased basal insulin secretion and decreased or abolished glucose-stimulated insulin release in vitro and in vivo [1720], as well as increased sensitivity of beta cells to conditions triggering apoptosis [30]. In vitro, most of these changes are also observed after pharmacological blockade of CX36 channels [15]. In vivo, beta cells lacking Cx36 also feature a delayed off response, i.e. they are slower than controls in turning off their insulin output when taken from a stimulatory to a basal condition [17]. The mechanisms involved in these changes are multifold, and may include the downregulation or loss of several CX36-dependent mechanisms, including the intercellular synchronisation of the glucose-induced Ca2+ transients [17, 19, 31], the intercellular transfer of electrotonic currents [32], the recruitment of intrinsically heterogeneous beta cells into secretory function [33], and the cross-talk with insulin regulatory pathways activated by ephrins [34]. Given that fetal and newborn beta cells feature defects in membrane depolarisation and Ca+2 handling [1, 2, 4, 7, 8, 24], it is conceivable that their modest expression of Cx36, gap junctions and beta cell coupling could account for their poor glucose-induced insulin secretion. Consistent with this view, we now show that a postnatal increase in the levels of the CX36 protein, the abundance of gap junctions and the extent of beta cell coupling accompanies the in vivo acquisition of glucose responsiveness, as previously suggested by preliminary in vitro experiments [9]. We further document that, during development, the levels of Cx36 expression correlate with those of the insulin gene, as recently reported in humans [29]. Beta cells of neonatal islets express significantly less insulin mRNA than those of adult rats [8], a difference that cannot be explained merely by developmental changes in beta cell number/volume [3]. Our data indicate that increased CX36 signalling may be required to achieve proper insulin expression, an essential landmark of beta cell maturation, a consideration which, in turn, raises the intriguing possibility that the CX36 and beta cell maturation events may not only be coincidental but possibly also causally linked. Further experiments investigating the underlying molecular mechanism and/or mice featuring a beta cell-specific loss of CX36 [18] are now required to test this hypothesis.

Contrasting with most other cell types which co-produced several different connexin isoforms [35], adult beta cells produce only CX36 [18, 22, 28, 32, 36]. Still, the presence of different connexin transcripts, notably for CX43, has been reported repeatedly in the islets of different animal species [9, 14, 35, 37], presumably accounting for the connexin expressed by other cell types, including endothelial, connective and immune cells of islets [28]. Using available antibodies, we did not detect CX43 in the beta cells of all the islet groups we investigated and, accordingly, we could not record a large intercellular exchange of Lucifer Yellow, a tracer that readily permeates CX43 channels [22, 38]. Rather, we observed with development an increase in beta cell coupling attributable to channels that were preferentially permeable to positively charged tracers, a signature of CX36 [22]. These data clearly demonstrate that maturing beta cells are functionally connected by CX36, but not CX43 channels, as reported in adult animals [18, 22, 28, 32, 36] and humans [29]. Still, antibodies to CX43 labelled vimentin-positive, duct and alpha cells at the periphery of newborn islets. The specificity of these immunostainings is presently supported by their loss with islet development, but should be fully validated after deletion of Cx43 in specific cell types, e.g. using the Cre-lox strategy [18, 28]. Given that proliferating cells, some of which may be still undifferentiated progenitors of islet cells, are found at the periphery of fetal and neonatal islets [3, 3941], and that CX43 is usually produced in undifferentiated stem and progenitor cells [4244], further work should investigate whether these cells have any relevance for islet development or repair.

In summary, we have shown that the acquisition by rat islets of normal secretory function is tightly linked to selective changes in the production of gap junction proteins that result in increased assembly of gap junction plaques at beta cell membranes and in enhanced intercellular exchange of cationic molecules between cells of this type. As young islets reach full secretory maturation, their beta cells show CX36 coupling like that of adult beta cells. The close parallelism between these events and the close relationship between Cx36 and insulin levels raises the possibility that CX36 may be a useful target for inducing the maturation of beta cells in vitro [45], and for new approaches to the therapy of neonatal diabetes [46, 47].


The authors thank Marta Beatriz Leonardo, Léscio Domingos Teixeira (University of Campinas), Dorothée Caille, Anne Charollais, José Cancela and Pilar Ruga Fahy (University of Geneva) for excellent technical assistance. The authors thank Dr Hernandes F. Carvalho (University of Campinas) for the anti-vimentin and secondary antibodies. This work was funded by grants from FAPESP (99/06846-0, 02/11909-5, 02/13218-0, 06/50758-3) and CAPES/PROEX. C.P.F. Carvalho was a recipient of CAPES and CNPq fellowships (Brazil). C.B. Collares-Buzato was on sabbatical leave at the Department of Cell Physiology and Metabolism, University of Geneva, Switzerland, supported by CNPq (Brazil). The Meda team is supported by grants from the Swiss National Science Foundation (310000-109402), the Juvenile Diabetes Research Foundation International (1-2007-158) and the European Union (BETAIMAGE 222980, IMIDIA, C2008-T7).

Duality of interest

The authors declare that there is no duality of interest associated with this manuscript.

Supplementary material

125_2010_1726_MOESM1_ESM.pdf (10 kb)
ESM Table 1Antibodies used for immunofluorescence (PDF 10 kb)
125_2010_1726_MOESM2_ESM.pdf (7 kb)
ESM Table 2Antibodies used for western blots (PDF 7 kb)
125_2010_1726_MOESM3_ESM.pdf (33 kb)
ESM Table 3Specific primers for RT-PCR and predicted product sizes (PDF 33.4 KB)
125_2010_1726_MOESM4_ESM.pdf (32 kb)
ESM Table 4Specific primers for quantitative PCR and predicted product sizes (PDF 31.7 KB)

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© Springer-Verlag 2010