Plankton: We catch live plankton weekly and would like to preserve the specimens.  We would like to collect a long term sequence we can use as a data set>

No votes yet
Publication Date: 08 June 2016
Asked By: rsear9
Showing 1-1 of 1 Responses


In Brief

Plankton collection samples are usually fixed and preserved before they are analysed for estimation of biomass, enumeration (counting) and identification of plankton genus/species. Data obtained is used for estimation of faunal and species biodiversity of the study area or ecosystem.

Science ASSIST recommends 70% alcohol for use in schools for the preservation of plankton. Under these conditions, without prior fixation with formaldehyde, it should be noted that the shelf life of the specimens will be expected to be in the order of 1-2 years. Science ASSIST does not recommend formaldehyde for use in schools.

Ethanol1 (Ethyl alcohol) usually comes in the 95% concentrated form. It is also a suitable preservative and method of choice for long-term preservation and storage for most plankton. It is usually diluted with distilled water to 70-75% strength. This is the lowest concentration at which preservation will be maintained. Samples will become a bit brittle in alcohol, a lot of the pigment will be extracted and there are evaporation issues. Some reports state that the addition of 1% glycerol aids in maintaining some flexibility of the samples and helps retard evaporation2. Alcohol is highly flammable, usually safe to handle, but can cause irritation to the skin in cases of prolonged contact.

Simple 2 stage method using 70% ethanol for the preservation of plankton in schools3

(Note: % v/v is used for concentrations of solutions of liquids and is calculated as [(volume solute)/(volume of final solution)] x 100%. For example, 70% v/v means that 100 mL of solution contains 70 mL of the solute.)

Stage 1: At the collection site add 95% ethanol to the sample of seawater/zooplankton in a ratio of 50:50. You will initially get a white milky colouration of the solution but this will slowly disappear.

This first stage is done fairly quickly after collection as the zooplankton will start to eat each other and begin to rot.

Stage 2: Back in the lab carefully tip off the solution and replace with fresh 70% ethanol solution and store in wide mouthed clear glass jars so students can see the specimens clearly. It is important to use tight fitting lids to prevent evaporation. The use of Parafilm or some silicone sealant can be used to provide a good seal. Note: You need to be careful if using plastic containers. Some become very brittle and craze with the alcohol.

70% alcohol will not overly dehydrate the tissue. Concentrations higher than this are not recommended as they can excessively dehydrate the tissue. At 70%, ethanol is an effective biocide. The preservative should be changed within the first 6 months for better shelf life of samples.

Store under conditions to prevent any deterioration i.e. a cool dry place in low light levels and out of direct sunlight. There are evaporation and flammability issues with the use of alcohol so the specimens should be monitored regularly and topped up as needed and stored in the flammable liquids cabinet4.

Note: A good activity is to encourage students to look at the zooplankton live as they are very interesting to examine. Many can survive for 24hrs in a bucket if kept in the dark.

Additional information

The chemicals used to fix and preserve specimens can be hazardous. Science ASSIST recommends you refer to the specific SDS for any chemicals being used and conduct a site specific risk assessment to assess and control any risks. You will need to make sure that all chemicals are approved for use in your jurisdiction and educational sector and are disposed of appropriately following local guidelines.

Fixation: should be carried out as soon as possible after collection or narcotising (if required) to avoid damage to tissue by bacterial action and autolysis. The choice of fixative should preserve the tissue against microbial activity, osmotic damage and autolysis. It should also allow the structure of the tissue to remain as close as possible to its original state. Some plankton react to the fixative used by contracting and distorting that can leave them in an unidentifiable state.

Formaldehyde5 is toxic, carcinogenic, highly irritating and acts as a potent sensitizer. Whilst formaldehyde at a concentration of 4-5% in distilled water is regarded as the best fixative to maintain taxonomic and morphological characters of mixed marine plankton1, it is toxic by all routes of exposure, has irritating fumes to the eyes, skin and mucous membranes and is a known human carcinogen6,7.  It is for these reasons that Science ASSIST does not recommend formaldehyde for use in schools. See Science ASSIST List of recommended chemicals for science in Australian schools.

Narcotisation: Some specimens require narcotising to relax the specimen allowing them to be fixed without any distortion8,9. However, narcotising is not usually done in schools unless you specifically want to do some specialised work on some of the zooplankton sample, e.g. histology.

If narcotising specimens is required samples are concentrated into sample buckets and then transferred to 500 ml plastic sample storage bottles. Samples should be refrigerated as soon as possible after collection,8,9,10. The narcotising solution is added drop by drop to the water containing the specimens and left to stand for up to 30 minutes in the refrigerator.

The following narcotising solutions are recommended for use 9,10,11

  • 70% ethyl alcohol –  add the alcohol drop by drop to the sample water concentrate
  • Carbonated water( soda water) 1:20 by volume – combine 1 part soda water with 19 parts of  sample water concentrate
  • Clove oil –  place tip of pipette with clove oil just under the surface of the sample water concentrate and add 1 to 2 drops at a time
  • Magnesium sulphate (Epsom salts) 20-30% aqueous solution – slowly add the solution drop by drop to the sample water concentrate


Label the container to include collectors name, type of specimen, type and date of preservative and any other field information. Label both inside and outside of the storage container. This will lessen the likelihood of the specimen and label being separated. It is important to use paper intended for long-term preservation in fluids. There are a several papers that will do including laundry tag paper. See Resistall labels and specimen tags: Soft lead pencil can be used to write on the paper and there are certain inks or ink pens that can be used as well. Any inks used should be of archival quality, resistant to fading and smearing, and be insoluble in the preservative solution. Suitable inks and ink pens can be found in some art or office supply stores and museum supply companies. It is recommended to allow the ink to completely dry before placing the label into the storage solution. Ordinary ballpoint pens should not be used for labelling as they generally dissolve in most preservative solutions. See the Science ASSIST School science suppliers  list for local museum supply companies for similar products.


Plankton is a diverse group of small and microscopic organisms (phytoplankton – plants and zooplankton – animals) drifting or floating in the sea or fresh water. Plankton consists mainly of diatoms, protozoans, small crustaceans, and the eggs and larval stages of larger animals12. Many animals are adapted to feed on plankton, especially by filtering the water. Plankton play a vital role in the marine food chain and an important role in the study of the biodiversity of aquatic ecosystems.

Zooplankton includes a wide range of macro and microscopic invertebrate animals. They feed on phytoplankton and in turn represent an important food source to animals higher up in the food chain including fish. Zooplankton are ubiquitous and are found in any aquatic ecosystem. The majority are microscopic unicellular or multicellular forms ranging in size from a few microns to a millimetre or more.

Phytoplankton are photosynthesizing microscopic organisms that inhabit the upper sunlit layer of almost all oceans and bodies of fresh water. They include self-feeding, single celled algae that live near the water surface where there is sufficient light to support photosynthesis. Among the more important groups are the diatoms, cyanobacteria and dinoflagellates.

Further reading:

Science ASSIST previously answered a similar question see: preserved specimens

The extensive list of references contain much recommended reading on this topic.


1‘Ethanol', Safety Data Sheet, Chem-Supply website, (October 2015)

2Johnson, W.S. and Allen, D.M. 2005. Zooplankton of the Atlantic and Gulf Coasts: A Guide to Their Identification and Ecology. Appendix 3 Relaxing, fixing and preserving zooplankton.  JHU Press, 2005. (Accessed July 2016)

3Personal Communication, Professor Iain Suthers. School of Biological, Earth and Environmental Sciences, University of NSW July 2016

4Suthers, Iain M and Rissik, David (Eds.). 2009. Plankton: A guide to their ecology and monitoring for water quality. CSIRO Publishing,

5 ‘Formaldehyde', Safety Data Sheet, Chem-Supply website, (January 2016)

6 'Known and Probable Human Carcinogens', American Cancer Society website, (Accessed July 2016)

7 ‘Formaldehyde’, IARC Monograph 100F, IARC website, (Updated July 2018)

8Steedman, H.F (Ed.) 1976. Zooplankton fixation and preservation, UNESCO Press: Paris, UNESCO website,

9National Institute of Oceanography. 2004.  'Zooplankton Methodology, Collection & Identification – a  field manual', NIO website,

10Behringer, Marjorie. 1973. Techniques and Materials in Biology, McGraw-Hill, Inc. Library of Congress USA.

11Dungey, Barbara. 2006. The Laboratory: a science reference and preparation manual for schools (Rev. ed), National Library of Australia: Traralgon, Vic.

12 ‘Plankton’, Wikipedia website, (Accessed June 2016)


Black, A.R. and Dodson, S.I. 2003. ‘Ethanol a better preservation technique for Daphnia’, Limnology and Oceanography,: Methods 2003: 45–50, ASLO website, (The link to this reference has been removed because it is no longer freely available; October 2017).

'DNA barcoding plankton', Department of the Environment Australian Antarctic Division website,  (December 2015)

Johnson, W.S. and Allen, D.M. 2005. Zooplankton of the Atlantic and Gulf Coasts: A Guide to Their Identification and Ecology. Appendix 3 Relaxing, fixing and preserving zooplankton.  JHU Press, 2005.

National Institute of Oceanography. 2004.  'Zooplankton Methodology, Collection & Identification – a field manual', NIO website,  

Richardson AJ, Eriksen RS & Rochester W. 2015. Plankton 2015: State of Australia’s oceans. CSIRO Report. IMOS website,

'Sampling'. Institute of Food and Agricultural Sciences School of Forest Resources & Conservation Program for Fisheries and Aquatic Sciences, University of Florida website,  (Accessed June 2016)

'Standards in the Care of Wet Collections.' Conservation Centre for Natural History Museum, London website, (Accessed June 2016)

Steedman, H.F (Ed.) 1976. Zooplankton fixation and preservation, UNESCO Press: Paris, UNESCO website,

United States Environmental Protection Agency. 2005. Standard Operating Procedure for Zooplankton Sample Collection and Preservation and Secchi Depth Measurement Field Procedures.

Wilson. R. 2005. Marine invertebrate sample processing procedures, Museum Victoria website,

'Zooplankton’, Marine Education Society of Australasia website, (Accessed June 2016)

07/09/2016 Edit: added details of personal communication

Thank you for submitting an answer to this question. Your response has been sent to our administration team for moderation.