Peptide adsorption: glass, low-bind tubes and sample recovery

Research-use notice: this article is for legitimate laboratory and educational research only. It does not provide guidance for human use, administration, dosing or treatment.

Peptide adsorption is the binding of peptide molecules to the surfaces they touch, such as tube walls, vials and pipette tips, which can remove a measurable share of a dilute peptide from solution. In a 2015 study in PLOS ONE, only 10–20% of three cationic peptides was recovered from 1 µM solutions kept in borosilicate glass vials or polypropylene tubes. Losses depend on the peptide, the surface, the concentration and the solution, so there is no universal loss figure and no single best container. Recovery has to be checked for the system you are using.

What is peptide adsorption?

Adsorption means sticking to a surface, as opposed to absorption into the bulk of a material. Many peptides carry charged or water-repelling side chains, and both kinds can interact with glass or plastic. Once peptide is held on a wall, it is no longer in solution, so the concentration an assay sees can be lower than the concentration calculated from what was added.

The effect matters most when solutions are dilute. A surface can only hold so much peptide, so the same absolute loss is a larger share of a small amount. In the PLOS ONE study, recovery rose as peptide concentration increased, consistent with the surface becoming saturated. It also happens quickly: the authors found that adsorption of one of the peptides to the container walls occurred within the first few seconds.

What the research shows

The evidence here comes from in vitro analytical studies. They show how big the effect can be and which variables matter, rather than giving a loss figure for any particular research peptide.

• Cationic peptides on glass and plastic. Kristensen and colleagues, in PLOS ONE in 2015, studied three cationic peptides, mastoparan X, melittin and magainin 2, in borosilicate glass vials, polypropylene tubes and low-binding polypropylene tubes. Losses at low concentration were large in standard glass and polypropylene. Salt concentration had little effect, whereas adding lipid vesicles to the buffer prevented adsorption. They concluded that low-binding tubes can be a useful tool for minimising surface adsorption.
• Eight endocrine peptides across many surfaces. A 2011 study in Analytical Biochemistry incubated eight radiolabelled peptides, including ghrelin, insulin, leptin and peptide YY, in glass and plastic tubes for 48 hours. The authors found important differences in binding between surfaces. Siliconising tubes decreased recovery, whereas adding bovine serum albumin (BSA) increased it, and lyophilising with BSA in the best tube for each peptide gave more than 89% recovery for all eight.
• One decapeptide, four surfaces. A 2004 study in the European Journal of Pharmaceutical Sciences found that dilute solutions of the decapeptide cetrorelix in distilled water gave a poor and variable high-performance liquid chromatography (HPLC) response. Adsorption fell in the order glass, then polypropylene and polyethylene (equal), then poly(tetrafluoroethylene) (PTFE), with considerable differences between glass vials from different suppliers. Adding ethanol, acetic acid or surfactants to the solution raised the response up to fivefold and made it less variable.
• Autosampler vials in proteomics. A 2013 study in the Journal of Proteome Research compared seven vial types and six sample solutions for storing a peptide digest. Polypropylene vials combined with either a low concentration of polyethylene glycol (PEG) or a concentrated urea and thiourea mixture were the most effective combinations.
• Hydrophobic peptides and new vial materials. A 2025 study in Analytical Chemistry found that hydrophobic peptides preferentially adsorbed to polypropylene vials, causing uneven signal loss. Vials made from polymers with polar units, poly(methyl methacrylate) (PMMA) or polyethylene terephthalate (PET), drastically reduced that loss, giving a fourfold increase in identified peptides at single-cell-equivalent amounts. Non-ionic detergents made performance more consistent, even across different vial materials.
• Losses over time in storage. A 2015 study in the Bulletin of the Korean Chemical Society followed peptide losses from a sample stored in autosampler vials over 145 hours and found that the most reliable recovery depended on the combination of vial material and solution.
• Distorted calibration. A 2013 study in the Journal of Proteomics found that many peptides from a standard protein digest did not give a linear relationship between mass spectrometry signal and amount under standard conditions. Raising the organic-solvent content of the sample solution improved linearity, which, the authors suggest, points to concentration-dependent surface adsorption.

A 2014 review in the Journal of Chromatography A by Maes and colleagues pulls this together for liquid chromatography–mass spectrometry (LC–MS). It treats non-specific adsorption as a cause of both lost signal and carryover, and covers strategies at every stage, from the solvent used to dissolve the analyte to the parts of the analytical system it passes through.

Glass, plastic or low-bind tubes?

The honest answer from these studies is that it depends on the peptide. Charge and hydrophobicity both influence which surfaces bind it.

The 2011 authors’ conclusion is the practical one: choosing the appropriate container avoids unpredictable peptide loss that leads to inaccurate measurements and false conclusions.

How to reduce and measure losses in the lab

These steps are drawn from the studies above. Each one changes the system, so check that it is compatible with your assay.

• Test containers for your peptide. Compare candidate tubes or vials with the same solution and measure what is recovered, rather than relying on a general rule.
• Keep the volume-to-surface ratio high. Kristensen and colleagues recommend a high sample volume relative to the container surface, and fewer transfers mean fewer surfaces.
• Consider a carrier or additive. BSA, PEG, lipid vesicles, surfactants and a higher organic-solvent content have each been used to limit losses in the studies above, but each one also becomes part of the sample and can interfere with some measurements.
• Be wary of pre-coating. Kristensen and colleagues caution that a container pre-saturated with peptide could act as a reservoir, releasing peptide back into later solutions.
• Measure, do not assume. Where concentration matters, measure it in the final container and include a recovery control that goes through the same handling as the samples.
• Record the consumables. Note the tube or vial type and lot alongside the peptide batch, so a change of plastics can be ruled in or out if the data shift.

For assays built on mass spectrometry, consensus recommendations published in Clinical Chemistry in 2016 cover the generation, quantification, storage and handling of peptide standards, and are worth reading alongside the adsorption literature.

Adsorption, aggregation or degradation?

A lower-than-expected measurement has several possible causes, and they can occur together:

• Adsorption removes intact peptide from solution onto surfaces. Losses are typically worse in dilute solutions and differ between container types.
• Aggregation leaves the peptide in solution but in a different physical state, which may not be measured or may behave differently. See our article on peptide aggregation.
• Chemical degradation, such as methionine oxidation, changes the molecule itself and usually shows up as new peaks or mass shifts.
• A content problem means the starting material held less peptide than assumed, for example because the solid also contains water and counterions. Check the batch laboratory report or certificate of analysis (COA); see How to read a peptide COA and our batch report lookup.

Not every loss in a vial is adsorption. The 2015 autosampler study observed losses of hydrophilic peptides whatever the vial material, and found that some hydrophobic peptide losses had causes other than adsorption to the vial. Comparing containers, concentrations and time points usually separates these possibilities. Adsorption losses change with container type and are proportionally larger at low concentration; degradation products appear in a chromatogram or mass spectrum. Our peptide storage guide covers handling records in more detail.

Peptide adsorption FAQs

What is peptide adsorption?

The binding of peptide molecules to surfaces such as tubes, vials and pipette tips. It lowers the amount of peptide left in solution, especially when the solution is dilute.

Do peptides stick to glass or plastic?

Both, depending on the peptide. Studies have found large losses of cationic peptides in both borosilicate glass and polypropylene, and preferential loss of hydrophobic peptides to polypropylene.

Are low-bind tubes worth using for peptides?

They can reduce losses, and one study described them as a useful tool for minimising adsorption. They do not remove the problem entirely, so recovery should still be checked.

Can adsorption affect LC–MS quantification?

Yes. Because losses are proportionally larger at low concentration, adsorption can bend a calibration curve and cause carryover between runs. Studies have reduced these effects by changing the sample solvent or the vial material.

How can I tell whether I have lost peptide to adsorption?

Run a recovery control: prepare a known amount, take it through the same containers and handling as the samples, and measure what remains. Comparing container types or concentrations shows whether surface loss is the cause.

Sources

• Kristensen K, Henriksen JR, Andresen TL. Adsorption of cationic peptides to solid surfaces of glass and plastic. PLOS ONE. 2015;10(5):e0122419. Primary study; in vitro.
• Goebel-Stengel M, Stengel A, Taché Y, Reeve JR Jr. The importance of using the optimal plasticware and glassware in studies involving peptides. Analytical Biochemistry. 2011;414(1):38–46. Primary study; in vitro.
• Grohganz H, Rischer M, Brandl M. Adsorption of the decapeptide Cetrorelix depends both on the composition of dissolution medium and the type of solid surface. European Journal of Pharmaceutical Sciences. 2004;21(2–3):191–196. Primary study; in vitro.
• Stejskal K, Potěšil D, Zdráhal Z. Suppression of peptide sample losses in autosampler vials. Journal of Proteome Research. 2013;12(6):3057–3062. Primary study; in vitro.
• Kune C, Tielens S, Baiwir D, et al. Significant impact of consumable material and buffer composition for low-cell number proteomic sample preparation. Analytical Chemistry. 2025;97(7):3836–3845. Primary study; in vitro.
• Maes K, Smolders I, Michotte Y, Van Eeckhaut A. Strategies to reduce aspecific adsorption of peptides and proteins in liquid chromatography–mass spectrometry based bioanalyses: an overview. Journal of Chromatography A. 2014;1358:1–13. Review.
• Warwood S, Byron A, Humphries MJ, Knight D. The effect of peptide adsorption on signal linearity and a simple approach to improve reliability of quantification. Journal of Proteomics. 2013;85:160–164. Primary study; in vitro.
• Cho HR, Park JS, Wood TD, Choi YS. Longitudinal assessment of peptide recoveries from a sample solution in an autosampler vial for proteomics. Bulletin of the Korean Chemical Society. 2015;36(1):312–321. Primary study; in vitro.
• Hoofnagle AN, Whiteaker JR, Carr SA, et al. Recommendations for the generation, quantification, storage, and handling of peptides used for mass spectrometry-based assays. Clinical Chemistry. 2016;62(1):48–69. Consensus recommendations.

Published by Thistle BioLabs, a UK supplier of research materials. This article summarises external research, not studies conducted by Thistle. Educational information only; no medical advice or recommendation for personal use.