Myogenic mechanobiology governs how mechanical cues regulate myocyte organization, alignment, and functional maturation; however, in vitro platforms that enable quantitative control and real-time readout of myogenic mechanical microenvironments remain limited. Here, we engineered a pneumatic-driven organ-on-a-chip platform integrating six parallel culture units and a bead-embedded flexible PDMS membrane to deliver cyclic mechanical strain and enable quantitative stress–strain mapping in cardiomyocytes and skeletal muscle cells. Finite element-guided optimization ensured effective membrane deformation, and the platform generated stable and tunable cyclic strain with a strong linear relationship between applied negative pressure (50–700 mbar) and membrane stress and strain. Plasma treatment combined with type I collagen coating restored myogenic cell adhesion and growth on PDMS to levels comparable to standard culture conditions. Under 13% cyclic strain, both cardiomyocytes and skeletal muscle cells exhibited pronounced and highly uniform alignment, with cellular polarity oriented perpendicular to the stretch axis. Moreover, cyclic loading significantly enhanced the expression of contractile maturation markers, including MYH7 in cardiomyocytes and MYH6 in skeletal muscle cells (all p < 0.05), whereas expression of the differentiation regulator MyoG remained unchanged, indicating that mechanical stimulation preferentially promotes structural organization and contractile maturation rather than lineage commitment. Collectively, this quantitatively programmable organ-on-a-chip represents a bioengineered microdevice for studying myogenic mechanobiology, revealing conserved mechanosensitive alignment and maturation responses across myogenic lineages and providing a versatile framework for biomedical engineering research, disease modeling, and mechanotherapeutic screening.

Helicobacter pylori (H. pylori) infection is closely associated with the development of chronic gastritis, peptic ulcers, and gastric cancer, highlighting the importance of rapid and accurate detection for disease prevention and clinical management. In this study, a one-pot LAMP-CRISPR/Cas12b assay targeting the CagA gene was developed for H. pylori detection. First, the LAMP system was optimized by systematically screening key reaction components. Subsequently, a one-step LAMP-CRISPR/Cas12b detection platform was established through optimization of the ratio between the LAMP premix and CRISPR buffer, reaction temperature, Cas12b concentration, and ssDNA reporter concentration. Under optimal conditions, the assay achieved a detection limit of 3.14 × 10¹ copies/µL, representing a tenfold improvement in sensitivity compared with conventional LAMP and PCR assays (3.14 × 10² copies/µL). In addition, the entire detection process could be completed within 1 h. Validation using 17 culture-positive and 17 culture-negative samples demonstrated complete concordance with culture-based results, with no false-positive or false-negative detections observed. These findings indicate that the proposed platform possesses high sensitivity, excellent specificity, rapid turnaround, and operational simplicity, demonstrating strong potential for point-of-care testing and applications in resource-limited settings.