Ca2؉ and cAMP are important second messengers that regulate multiple cellular processes. Although previous studies have suggested direct interactions between Ca 2؉ and cAMP signaling pathways, the underlying mechanisms remain unresolved. In particular, direct evidence for Ca 2؉ -regulated cAMP production in living cells is incomplete. Genetically encoded fluorescence resonance energy transfer-based biosensors have made possible real-time imaging of spatial and temporal gradients of intracellular cAMP concentration in single living cells. Here, we used confocal microscopy, fluorescence resonance energy transfer, and insulin-secreting MIN6 cells expressing Epac1-camps, a biosynthetic unimolecular cAMP indicator, to better understand the role of intracellular Ca 2؉ in cAMP production. We report that depolarization with high external K ؉ , tolbutamide, or glucose caused a rapid increase in cAMP that was dependent on extracellular Ca 2؉ and inhibited by nitrendipine, a Ca 2؉ channel blocker, or 2,5-dideoxyadenosine, a P-site antagonist of transmembrane adenylate cyclases. Stimulation of MIN6 cells with glucose in the presence of tetraethylammonium chloride generated concomitant Ca 2؉ and cAMP oscillations that were abolished in the absence of extracellular Ca 2؉ and blocked by 2,5-dideoxyadenosine or 3-isobutyl-1-methylxanthine, an inhibitor of phosphodiesterase. Simultaneous measurements of Ca 2؉ and cAMP concentrations with Fura-2 and Epac1-camps, respectively, revealed a close temporal and causal interrelationship between the increases in cytoplasmic Ca 2؉ and cAMP levels following membrane depolarization. These findings indicate highly coordinated interplay between Ca 2؉ and cAMP signaling in electrically excitable endocrine cells and suggest that Ca 2؉ -dependent cAMP oscillations are derived from an increase in adenylate cyclase activity and periodic activation and inactivation of cAMP-hydrolyzing phosphodiesterase.