Kisspeptin-10 Reconstitution Protocol: Bacteriostatic Water & Aliquoting

To reconstitute Kisspeptin-10, prepare: a sealed vial of Kisspeptin-10, bacteriostatic water (0.9% benzyl alcohol), a sterile insulin or tuberculin syringe with appropriate needle gauge, an alcohol prep pad, and a clean laminar flow surface or comparable workspace. Quality Peptide USA stocks both bacteriostatic water and individually wrapped alcohol prep pads as companion lab supplies.

1. Allow the lyophilized Kisspeptin-10 vial to equilibrate to room temperature for 5–10 minutes. 2. Wipe both vial stoppers with an alcohol pad. 3. Draw the desired volume of bacteriostatic water (commonly 1–3 mL per vial depending on study concentration). 4. Slowly inject the water down the inside wall of the peptide vial — do not inject directly onto the powder. 5. Swirl gently to fully dissolve. Do not vortex or shake aggressively. 6. Inspect the solution: it should be clear, particulate-free, and free of color.

With 5mg per vial, common research dilutions include 1 mL bacteriostatic water (yielding 5mg/mL), 2 mL (5mg/2 mL), or 3 mL for finer titration. Match the dilution to the volumetric precision of the syringe used for downstream aliquoting. Use the molecular weight (≈ 1302.45 g/mol) on the certificate of analysis to convert to molar concentration when required.

For longer-term studies, aliquot reconstituted Kisspeptin-10 into low-protein-binding microcentrifuge tubes immediately after reconstitution, then store at −20°C in a frost-free freezer. Avoid repeat freeze/thaw cycles — each cycle increases the risk of aggregation and degradation. Working aliquots refrigerated at 2–8°C should be used within the window listed on the Kisspeptin-10 product page.