This protocol allows us to generate genetically modified ants to understand the function of genes in communication and behavior in a social environment. Manipulating the genetic system of eusocial insects is challenging, as many species do not mate and reproduce in laboratory settings. The striking phenotype plasticity in the ant hypernasal cell floor allows us to establish CRISPR-mediated mutant lines.
Demonstrating the procedure will be Kayli Sieber, a graduate student from a laboratory. Maintain wild-type colonies of H.saltator in transparent plastic boxes in an ant rearing room at 22 to 25 degrees Celsius and a 12 hour light, 12 hour dark lighting schedule. Use small boxes to rear individual workers or small colonies and medium or large boxes to rear larger colonies.
To create nest boxes, use plaster to make the floors. As the wet plaster is drying in the medium and the large boxes, press a foam block into the plaster a few centimeters deep and a few centimeters from the back of the box to designate a lower nest region. Once the plaster has dried, cover the designated nest region with a square piece of glass.
Feed colonies with live crickets twice per week, and apply water regularly to the plastic nest box flooring using a wash bottle. Whenever feeding occurs, remove trash and dead individuals. Freeze all waste and dead ants overnight at minus 30 degrees Celsius before disposing of these materials as regular garbage.
Periodically add a pinch of dried sawdust to the colonies to help larvae as they undergo pupation and to help workers keep the nest box clean. Use a micro pipette puller to pull glass microinjection needles. Ensure that the glass being used has been stored in a dust-free and clean environment.
Use a two-step process to pull microinjection needles. For the first step, Set the heat to 575, filament to 3, velocity to 35, delay to 145, and the pull to 75. For the second step, set the heat to 425, filament to 0, velocity to 15, delay to 128, and the pull to 200.
Ensure that the resulting needle has a 2-millimeter taper and a tip of 0.5 micrometers. After pulling the needles, keep them in a dust free and clean environment until use. Prepare the microinjection mixture of casein proteins and in-vitro synthesized small guide RNAs.
Keep the mixture on ice until it is time to load a microinjection needle. When not in use, store the microinjection mixture at minus 80 degrees Celsius. Set the injection parameters to an injection pressure of 140 hectopascal, a constant pressure of 70 hectopascal, and a time of 0.4 seconds.
Adjust constant pressure such that material only flows in one direction, and adjust the injection pressure and time only if no material is flowing from the needle into the embryo. Load a microinjection needle with two microliters of the mixture using microloader pipette tips. Do this slowly to ensure that no bubbles are formed in the mixture.
Break just the tip of the needle along the edge of the tape, such that a narrow taper is still maintained. Ensure that the needle is broken just enough that the tip is opened, but not so much that the taper is broken off. Then mount the needle to the micro manipulator.
Select embryos for microinjection from the syncytial stage, which is when nuclei divide without cytokinesis. Line the embryos on a plate of double-sided tape stuck to a glass microscope slide, making sure that they are secured well to the tape to prevent movement during injection. Lay the embryos in a vertical orientation such that the lateral side of each embryo is at the edge of the tape.
Place the slide and lined embryos onto the stage of the microscope at a designated microinjection workstation. Align the needle with the first embryo to be injected using the micromanipulator, and laterally puncture the first embryo along its dorsal or ventral axis under a microscope. Inject the microinjection mixture, and look for slight movement of the embryo, indicating an increase in internal pressure due to the injected liquid.
Additionally, watch for the formation of a small droplet containing visible traces of tissue or lipid on the outer membrane of the embryo. Gently remove the needle from the embryo and proceed to the next embryo by adjusting the position of the microscope slide. Repeat until all embryos have been injected.
Once all embryos on the slide have been successfully injected, transfer the slide to a humid box for one hour to give the embryos time to recover before being removed from the slide. After the incubation, wash the slide with ethanol, gently remove the injected embryos from the tape using featherweight forceps, and transfer them to a tube filled with a small amount of 70%ethanol. Invert the tube several times.
Using a small and soft paintbrush, transfer all injected embryos to 1%agar plates with 2%antibiotic antimycotic. Incubate the plates at 25 degrees Celsius for approximately four weeks, checking regularly for hatching. Once the first embryo has hatched into a larva, return all embryos and larvae to a nest box with a few young nurse workers to care for the hatchlings.
Maintain the colony following the previously demonstrated methods. This protocol was used to successfully perform genome editing in Harpegnathos saltator embryos. Results were validated via PCR and pGEM cloning of DNA extracted from injected embryos, followed by DNA sequencing.
Efficiency of somatic mutagenesis using this protocol reached approximately 40%F1 mutant males were mated to wild type females to produce heterozygous F2 females which, if not mated, produced F3 males. Mutant F3 males were mated to heterozygous females to produce F4 homozygous mutant females. As a result of successful mutagenesis, unusual behaviors that correlated with the loss of the target gene were observed.
The loss of Orco is associated with a loss of pheromone sensing, inability to detect prey, impaired fecundity, and wandering from the colony. When performing this protocol, embryo damage during injection needs to be minimized. This can be done by ensuring the needle tip is not opened too wide, and by moving the needle slowly when injecting.
Similar techniques can be used to generate and maintain transgenic ants, which will provide more sophisticated tools for probing neuronal activity and behavior. CRISPR-mediated neurogenesis has been used in other eusocial insect species, such as honeybees, clonal raider ant, and fire ants. Genetic modifications will facilitate the functional studies on development, physiology, and social behavior in eusocial insects.
