WPI Blog

Choosing the right hemostatic forceps is important, but technique plays an equally critical role in minimizing tissue trauma. Factors such as clamping pressure, instrument orientation, clamp duration, and release technique can all affect tissue viability and surgical outcomes. Excessive force, prolonged compression, and repeated tissue manipulation may contribute to unnecessary damage, even when using high-quality instruments. This article explores practical principles for atraumatic tissue handling, including how to apply hemostatic forceps effectively, avoid common mistakes, and preserve tissue integrity. By combining proper instrument selection with sound technique, researchers can improve consistency, support refinement principles, and achieve more reliable results.

WPI’s new 5 µL NanoFil™ syringe is designed for researchers who require exceptional precision when delivering ultra-low volumes in ophthalmic and neuroscience applications. Featuring a gas-tight, zero-dead-volume design and a compact format that supports comfortable single-handed operation, the syringe improves dosing accuracy, volume resolution, and reagent conservation. Researchers can maintain greater control during delicate procedures such as intravitreal, subretinal, and stereotaxic injections while minimizing tissue disruption and reducing operator fatigue. Ideal for gene therapy, optogenetics, CRISPR research, and ocular drug delivery, the 5 µL NanoFil™ syringe helps produce reliable, reproducible experimental results.

Vessel damage during small animal procedures can affect tissue viability, recovery, animal welfare, and experimental reproducibility. Fortunately, many vascular injuries are preventable through appropriate instrument selection and careful tissue handling. This article explores the most common causes of vessel damage, including excessive clamping force, repeated manipulation, poor visibility, and instrument mismatch. It also discusses how hemostatic forceps, thumb forceps, and microsurgical instruments can help preserve vascular integrity when properly selected and maintained. By combining thoughtful instrument choice with atraumatic technique, researchers can reduce tissue trauma, improve procedural consistency, and support more reliable research outcomes.

Microsurgery demands precise tissue handling, where even small technique variations can influence outcomes. This article explores four common causes of iatrogenic tissue damage: excessive clamping force, instrument-related thermal transfer, repeated tissue grasping, and poor instrument tip alignment. Readers will learn how these mechanisms contribute to endothelial injury, inflammation, tissue fragility, and compromised healing, often before visible signs of damage appear. The article also outlines practical strategies for recognizing and preventing tissue trauma through proper instrument maintenance, careful energy management, and atraumatic handling techniques. These principles help improve surgical consistency, tissue viability, and experimental reproducibility in microsurgical procedures.

WPI’s disposable scalpels come in many styles and are ideal for students, researchers, and crafters. Here we will describe some of the uses for these popular blades.

Choosing the right cell culture dish for microscopy involves four key decisions: material, objective compatibility, format, and surface coating. This guide provides a practical framework for matching dish selection to imaging technique — from widefield fluorescence and confocal to TIRF, super-resolution, and live cell time-lapse. It covers when glass bottom dishes are required versus when plastic is acceptable, how to match FluoroDish™ format to workflow requirements, and when the FD3510's unique geometry makes it the right choice for microinjection and reagent conservation. A format reference table and technique-by-technique recommendations make this a practical resource for researchers, CRO analysts, and pharma imaging scientists.

Tissue preservation is critical in research surgery, where excessive trauma can affect healing, animal welfare, and experimental outcomes. Hemostatic forceps help minimize tissue damage by providing controlled pressure, improving bleeding control, and reducing unnecessary tissue manipulation during procedures. From fine mosquito forceps used in small animal surgery to larger instruments designed for tissue bundles and vascular pedicles, selecting the appropriate hemostat can improve precision and consistency. This article explores how hemostatic forceps contribute to atraumatic tissue handling, common mistakes that increase tissue injury, and best practices for preserving tissue integrity during laboratory and research procedures.

Coverslip thickness is one of the most overlooked variables in fluorescence microscopy, and one of the most consequential. High-NA objectives are optically corrected for imaging through exactly 170 µm of borosilicate glass. When the substrate deviates from that specification in thickness or refractive index, spherical aberration reduces resolution, degrades signal, and shifts the focal plane. Plastic dishes fail this specification on both counts and cannot be corrected with adjustment collars. This article explains the optical engineering behind the 0.17mm standard, the consequences of deviating from it, and why glass bottom dishes are the only substrate that meets it fully.

Up to 10% of researchers are left-handed, yet most laboratory scissors and instruments are designed exclusively for right-handed use. This creates real consequences in the lab, including reduced precision, compromised visibility, compensatory fatigue, and increased technique variability. This article explains the mechanical reasons why standard scissors underperform in a left hand, covers related instruments such as needle holders and ratchet forceps, and presents two practical solutions, dedicated left-handed scissors that mirror the blade geometry for natural action, and spring scissors, which are fully ambidextrous and ideal for fine dissection work. Small differences in instrument design can have a measurable impact on research quality.

Disposable scalpels are essential precision tools used in surgical, histology, and laboratory environments where accuracy, sterility, and reproducibility are critical. Selecting the correct blade type directly impacts cutting performance, tissue integrity, and experimental outcomes. Common blade types include the #10 for broad incisions, the #11 for puncture and entry cuts, and the #15 for fine, controlled dissection. This guide helps users understand how blade geometry affects cutting behavior and how to match scalpel selection to specific research workflows. Proper technique, including controlled cutting and single-use adherence, improves consistency and reduces contamination risk in sensitive biological applications across modern laboratory settings.

Plastic cell culture dishes are a common but overlooked source of fluorescence imaging problems. Polystyrene introduces two compounding issues: optical distortion from refractive index inconsistencies and autofluorescence from the material itself. These degrade image clarity, reduce signal-to-noise ratio, and compromise quantitative measurements. These problems are most damaging in low-expression reporter assays, multiplexed panels, and live cell time-lapse experiments. This article explains the science behind both mechanisms, identifies which workflows are most vulnerable, and provides a practical troubleshooting checklist for confirming whether your dish is the source of the problem.

Scalpel injuries in research and teaching laboratories are often preventable with the right sharps handling procedures and instrument choices. This article explores the most common causes of laboratory scalpel injuries, including blade changes, improper disposal, and unsafe instrument passing. It explains how disposable and safety scalpels help reduce sharps exposure while improving workflow efficiency in educational and research environments. The guide also covers best practices for safe scalpel handling, sharps disposal compliance, teaching lab safety protocols, and injury prevention strategies for students, educators, lab managers, and research staff.

When imaging is part of the science, dish material matters. Glass bottom dishes outperform plastic across every optical metric relevant to fluorescence microscopy, confocal, TIRF, and live cell imaging. Plastic polystyrene introduces autofluorescence that degrades signal-to-noise ratio, falls outside the optical correction range of high-NA objectives, and conducts heat poorly, creating temperature gradients during long time-lapse experiments. Glass eliminates these variables: it has negligible autofluorescence, matches standard coverslip thickness (~170 µm) for full objective compatibility, and equilibrates thermally for stable live cell conditions. Plastic remains practical for routine culture, but glass is the correct choice whenever imaging quality affects your conclusions.

When your research depends on delivering extremely small, highly controlled volumes,
precision isn’t optional. It’s essential. Micro syringe pumps are designed to meet this
challenge, enabling accurate and repeatable injections at the microliter and nanoliter
scale. In this guide, we’ll explore how these systems work, when they’re needed, and
what features matter most for reliable microinjection results.

WPI will be exhibiting at ARVO 2026 in Denver (Booth #6002), showcasing TEER measurement systems, organ-on-chip technology, and microinjection tools for ophthalmology research.

With over 1,380 peer-reviewed citations, the UMP3 Microinjection Syringe Pump has become a trusted standard for precise, repeatable fluid delivery at the micro- and nanoliter scale. This article highlights how researchers across neuroscience, ophthalmology, pharmacology, and microfluidics rely on the UMP3 to ensure consistent dosing, reduce variability, and produce reproducible results in demanding experimental environments.

Neuroscience research demands exceptional precision when accessing and manipulating delicate neural structures. From cranial opening and microdissection to probing, retraction, and controlled microinjection, high-quality surgical instruments play a critical role in experimental accuracy and reproducibility. WPI offers a comprehensive range of precision tools, including microscissors, spatulas, forceps, hooks, and microsyringe systems, engineered to support reliable, repeatable workflows in university, research, and laboratory environments.

Unstable TEER readings can result from a range of technical and biological factors, from electrode condition and temperature changes to media variability and air bubbles. This article helps researchers identify the most common sources of measurement inconsistency and provides practical solutions to improve stability and reproducibility. It also clarifies how to distinguish true biological changes in barrier integrity from unwanted measurement noise, ensuring more confident interpretation of results.

This article explains how to convert raw resistance measurements into standardized TEER values (Ω·cm²) for accurate comparison of barrier integrity across experiments. It walks through the TEER formula, defines each component, and provides a clear step-by-step calculation with examples. By understanding how to properly subtract blank resistance and apply surface area normalization, researchers can generate more reliable, reproducible, and publication-ready data.

Microinjection accuracy becomes more difficult at sub-microliter volumes because small mechanical inconsistencies can change the delivered dose. Dead volume, trapped air bubbles, micro-leaks, plunger behavior, and manual technique differences all contribute to variability between injections and between users. A true gas-tight, zero-dead-volume syringe system helps maintain stable pressure and reduces sample loss, improving confidence that what you load is what you deliver. For repeatability-focused workflows, pairing the syringe with a microinjection pump can further standardize flow rate and volume, producing more consistent dosing outcomes across sessions and experiments.

Improper handling of surgical instruments in laboratory settings can compromise research quality, instrument performance, and experimental reproducibility. Precision instruments used for dissection, microsurgery, and animal research are especially vulnerable to mechanical damage, loss of sterility, and material degradation when mishandled. These issues can lead to increased costs, inconsistent results, and reduced procedural accuracy. By adopting proper handling, cleaning, sterilization, and storage practices, laboratories can extend instrument lifespan and maintain reliable performance. Choosing high-quality, research-grade surgical instruments and training staff on correct handling techniques helps protect both scientific outcomes and long-term laboratory investments.