Feb 22, 2022
Enrichment of motile phototrophs by phototaxis
- Usha Lingappa1,
- Sabeeha Merchant1
- 1University of California, Berkeley
- Merchant Lab UC Berkeley
- UC Berkeley
Protocol Citation: Usha Lingappa, Sabeeha Merchant 2022. Enrichment of motile phototrophs by phototaxis. protocols.io https://dx.doi.org/10.17504/protocols.io.b47wqzpe
License: This is an open access protocol distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited
Protocol status: Working
We use this protocol and it’s working
Created: February 17, 2022
Last Modified: February 22, 2022
Protocol Integer ID: 58326
Keywords: enrichment, phototaxis, phototroph, algae, environmental microbiology, enrichment of motile phototroph, motile phototrophs from environmental sample, enriching motile phototroph, motile phototroph, phototroph, positive phototaxi, phototaxis this protocol, phototaxi, environmental sample, enrichment, sample
Funders Acknowledgements:
Sabeeha Merchant, Moore Foundation Symbiosis in Aquatic Systems Initiative Investigator Award https://doi.org/10.37807/GBMF9203
Grant ID: GBMF9203
Abstract
This protocol describes a method for enriching motile phototrophs from environmental samples by positive phototaxis, or the ability to move towards light. Samples are collected in the field using sterile equipment, and incubated in water and under lights to bloom phototrophs. Phototaxis is conducted in a sealed glass pasteur pipet filled with 0.15% agar, and wrapped in aluminum foil leaving only the tip exposed. Phototrophs must swim through the agar to reach the illuminated tip, separating them from the rest of the starting sample, and thereby generating an enriched fraction from which the phototrophs can be grown and isolated more easily than from a complex starting sample. This protocol is based on the method described in Sack et al, 1994.
Citation
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Materials
Sampling containers (e.g. Falcon tubes or Whirl-Pak bags)
Gloves
Spatula/scoopula
Sterile water
Grow lights
Agar
Sterile glass Pasteur pipets
Sterile bulb
Bunsen burner
Parafilm
Aluminum foil
Tack or needle
Sterile collection tube
Troubleshooting
Sample collection and preparation
Collect environmental samples (e.g. soil, sediment, water, etc. ) into sterile containers (e.g. Falcon tubes or Whirl-Pak bags), using sterile equipment (gloves, spatula/scoopula).
Note
Equipment can be surface-sterilized in the field using ethanol.
Encourage phototrophs to bloom by incubating samples under lights for 2-4 days.
Note
For solid samples, add sterile water at a roughly 1:1 volume:volume ratio so that phototrophs bloom into a liquid extract.
Enrichment by phototaxis
Add 0.15 g agar to 100 mL liquid medium.
Autoclave to sterilize and melt the agar.
Allow to cool to room temperature.
Prepare glass pipets for phototaxis.
Fill pipets. Using a sterile bulb, fill a sterile 9 inch glass Pasteur pipet roughly half full with the 0.15% agar medium (Figure 1A). If your tip is full of liquid to the very end, let 1-2 drips to fall out to create ~2cm of empty space at the tip. This will help you to avoid generating bubbles by boiling the liquid when you put the pipet tip in the flame.
Seal pipets. In one hand, hold the pipet and bulb, maintaining pressure on the bulb to keep the liquid in the narrow part of the tip, allowing only ~2cm of empty space at the end. With the other hand, grasp the end of the pipet tip with forceps. Place the empty part of the pipet tip in the flame. As the glass melts, use the forceps to pull the tip away from the rest of the pipet, drawing out the glass into an increasingly narrow capillary (Figure 1B). Once the tip has detached, hold the melted end of the pipet in the flame for a few seconds longer to fully seal it. Allow the glass a few seconds to cool to room temperature, then gently test that you successfully sealed the end by applying additional pressure to the bulb. Once you have confirmed that the tip is sealed, remove the bulb.
Conduct phototaxis.
Load samples. Add 200-500μL liquid samples or extracts from solid samples onto the top of the prepared glass pipets (Figure 1C). Release the sample gently and against the pipet wall so that it layers neatly above the 0.15% agar medium.
Seal the top of the pipet with parafilm (Figure 1D).
Wrap the finished pipets with aluminum foil, so that the body of the pipet is kept in the dark and just ~2cm of the liquid in the tip is exposed (Figure 1E).
Incubate horizontally under lights for 4-24 hours, to allow motile phototrophs to swim to the illuminated tip (Figure 1E).
Note
Shorter incubation times minimize contamination from non-phototactic organisms, but could exclude slower phototrophs.
Harvest motile phototrophs.
Unwrap pipet.
Using forceps, break open the sealed glass tip.
Using a tack or needle, prick a hole in the parafilm sealing the top, to release the vacuum pressure holding the liquid in the pipet (Figure 1F).
Collect the first few drips of medium that release from the pipet tip (the medium that had been in the illuminated region).
Spread harvested material onto agar plates with a medium of choice for your target phototrophs (e.g. TAP for Chlamydomonas), and incubate under lights until green colonies emerge.
Figure 1. Diagrams illustrating the use of a glass Pasteur pipet for enriching motile phototrophs by phototaxis. A. Fill pipet roughly half full with 0.15% agar in minimal medium (Step 4.1). B. Seal the pipet tip by melting in a flame (Step 4.2). C-D. Gently load sample onto top (Step 5.1) and seal with parafilm (Step 5.2). E. Wrap in foil leaving only the tip exposed (Step 5.3) and incubate horizontally under light (Step 5.4). F. Break open tip (Step 6.2) and prick parafilm seal (Step 6.3) to release medium dropwise (Step 6.4).
Citations
Lawren Sack, Clifford Zeyl, Graham Bell, Timothy Sharbel, Xavier Reboud, Torsten Bernhardt, Hans Koelewyn. Isolation of four new strains if Chlamydomonas reinhardtii (Chlorophyta) from soil samples
https://doi.org/10.1111/j.0022-3646.1994.00770.x