Questions related to Ciliate
I am in the process of making an experiment that requires dPCR testing so I cannot stain the Ciliates I use for analysis and because of time constraints. Due to the time constraints, I am thinking of using a computer program like ImageJ to measure the size of the individual; however, I am worried that ImageJ might not work for the ciliates because of the lack of a stain on the cell. My question is if anyone has experience on using ImageJ on unstained cells like ciliates and how well it worked for you.
We are trying to see if there is any pattern between SSU copy number and the size of the cell in Paramecium tetraurelia so we can more accurately determine the actual quantity of cells in a water sample for later experiments. The reason for not measuring by eye is because my supervisor is suggesting we do triplicate cultures in parallel with ten individuals per culture and we want to make sure that they are all on the same growth stage for better control on the size/copy number.
We are analyzing the behavior of groups of Stylonychia mytilus and have already some interesting preliminary results. Unfortunately our strain died and we are not able to find a new supplier. Is there a culture collection - possibly i Europe - that can provide the species or does someone work with the organism and can help us?
I am looking for ways to get rid of ciliates in cultures of Tetraselmis. We believe they are contaminating via the air lines. Any ideas are welcome!
We are trying to compare the complexity of the myoneme structures in different families ciliates. Due to protargol not being on the market anymore and the insane price of Gold(III)chloride I was wondering if there are any other methods which will elucidate these structures.
I'm trying to grow up a rotifer culture, but I have a lot of problem with ciliates contamination.
I have tried several times to clean all the culture with a 55 um sieve, clean with bleach all the material that I use, but after one day ciliates are there again.
Do you have any advice?
Hello everyone, greeting, hope you are doing well, I need some significant information, which is related to the use of silver nanoparticles in the aquatic ecosystem. My question is this when we apply different concentrations of Ag-NPs on Ciliates to check the toxicity of silver nanoparticles. We know that silver nanoparticles kill the ciliates, disturb the aquatic ecosystem. Anxiously waiting for your kind response. Thank You
Md. Masud Parvez.
I'll be looking at air-liquid interface sections of primary human airway epithelial cells and am interested in multiciliated cells.
There are multiple references in support of both ac-a-tubulin and b-tubulin IV, but to the best of my ability I can't find whether there's any real difference or advantage to using one over the other.
Has anybody grown algal biofilms from stream inocula on ceramic tiles and observed such bare areas as in the photos? They look like a virus infection to us. We have observed this phenomenon a few times already and it disturbs grazing experiments… The first bare spots appear after some 7 days, grow up to 5-6 mm diameter, more appear, and after another two weeks (approx.) they slowly start to vanish again from their centre. Of course, we have also protist grazers (ciliates etc) in our biofilms but they are not responsible for these spots, we think.
Thanks for any helpful information on what that might be and how it could be prevented!
Susanne Worischka, Felix Grunicke and Thomas Petzoldt
I am looking for a software that would allow me to record real-time videos of my ciliated epithelia primary cell cultures using an inverted microsope and Canon camera.
Currently, I am using QuickPHOTO Camera 3.0 which does not allow me to record videos (only time-lapse with intervals 13s between images).
Dr. Martina Schrallhammer,
I have received an e -mail form you depending on a contribution to a Special issue at Diversity as “Biodiversity of Ciliates and their Symbionts”.
I would like learn ıf thıs is really from you or a predatory one.
Thank you for your cooperation.
sırma çapar dinçer
Hi, I am looking for some information about Vorticella morphology. In some Vorticellas I found lot of granules I think it is a reserve granules but I am not sure. Some publications called they as " refractile reserve granules" - what does it mean? What does they large numer mean? Also why are they iridescent yellow sometimes?
We would like to perform experiments concerning virus infection (prevention) of mucosa of the upper aerodigestive tract. I am not very familiar with virology, so does anybody know a kind of "handicapped" virus, which can infect ciliated epithelium cells, but is not pathogenic?
One of the main calculation method for ciliates abundances is using Madoni(1984) sub-sample methodology.
However for ciliates is anybody using other methods and how, to calculate abundance in lake?
I am trying to specifically kill ciliates in a community of cyanobacteria. Our growth medium is high pH and high alkalinity, and has to stay that way so the community doesn't change.
For my master thesis I need to analyse Illumina 18S rRNA sequencing data with regard to the composition of Ciliates (protozoa) in my samples. So the OTU´s that really drive my interest are only a very small proportion of all the OTU´s in my OTU table. The samples were taken from prefiltered seawater, but sometimes some metazoa got into several but not all samples and for example once or twice 1/3 of the total reads (sample depth) consists of one Taxa, which I will not take into account in the ordination techniques, because I only focus on ciliates.
When I use standardization techniques like rarefying or ANCOM or DESeq2 do I use it on the whole OTU table, or do i discard the taxa which I will not use for further analysis in advance?
I am looking forward for your answers!
I have some samples (few cells of ciliates) are preserved in RNAlater. So is there any problem if I start my work by adding lysis buffer for RNA extraction in my preserved samples stored in RNAlater. Becuase my cells are very small and very few. If I remove RNA later completely then I can lose my samples. And what is the best way to remove RNAlater for ciliate RNA extraction?
I am looking for a fairly easy method such as lower/raise pH or salinity. Any experiences ?
I know that solation of T. suecica cells is one method but this will take too long before a new clean culture is up and running.
I want to analyse my ciliates data for ecological network modeling purpose, but i don't know how to make matrix formation using R.
We (= Evolution Lab of Faculty of Science in Zagreb) have collected fresh samples of swamp water from bog in continental Croatia a few days ago in which we found a lot of Paramecium bursaria specimens. Since this ciliate species is very interesting for research and for teaching students on endosymbiosis, we are interested where to find information, published or unpublished protocol how to maintain acidic medium similar to that in bog in lab conditions (I assume it is by adding some swamp-similar buffer and it would be very nice to know its compounds). We have gotten info that P. bursaria is very in the long run, we need something better. Thank you for your time and answers in advance.
Is anyone aware of any attempt at separating ciliated from non ciliated cells by means of fluorescence activated cell sorting (FACS) of live cells?
I would like to use genetically encoded biosensors selectively expressed at the cilium and purify cilium positive cells to perform functional assays with them.
In the deep Skagerrak I found several specimens of Nephtys hystricis at different stations with ciliates attached to its gills. Obviously only this species was suitable to host the ciliates. Other Nephtys-species and also other polychaetes were not "infected". I konw the paper by Alvarez-Campos et al. (2014) describing ciliate species on Syllidae. Maybe somebody knows about similar observation on Nephtyidae.
I am working on the evolution of protozoans in activated sludge and am trying to collate as much published and unpublished data on diversity in activated sludge from around the world. Any data sources or unusual references or links would be really helpful. Thanks
Hi, I am do phytoplankton taxonomy and I am debating whether the following is a Mallomonas sp. or a ciliate (or something else). Thanks for your suggestions
I have found this ciliate in hay infusion and do not know what it is. I expect it is quite common so I went through the pictures on Google and found some opaline ciliates as the most similar. But I really do not know. Does anyone know what it is? Sorry about the quality of the picture, it is taken by cell phone.
The data is from RNAseq sequences of one ciliate species (unicellular protist). I used program getorf to do the translate. Getorf gave 6 result for each contig ( nucleotide sequence). How can I recognize which one is the correct one? Should I choose the longest one, or should I refer the blastX information? Any other suggestions are appreciated as well.
I need a method to measure the rate of photosynthesis (apart from DO method) in micoralgae, wherein my algae is in mixed culture of bacteria and ciliates.
Also, how do I measure the health status of the algal cells (anything apart from fv/fm ratio calculation and microscopy).
It is look like a leaf under microscope, but it could be a plankton. Earlier I heard that it was a ciliate, but I didn't get this picture again in my samples. This too found in Bay of Bengal waters. Please help me to identify this specimen.
Is there any good resource of ciliates that talks about species specific feeding habits (eg feeding type, trophic role, clearance rate)?
I transformed the fresh water ciliate Tetrahymena termophila with GFP. The transformation was successful, as they conferred resistance to a selective antibiotic.
The expression is inducible with Cadmium chloride (at 1ug/ml). When I did fluorescence microscopy, I got no signal in living cells, but a visible signal in Glutaraldehyde fixed cells. I am now wondering why. Has someone experienced similar things? Or can someone explain why?
The signal in the fixed cells is relatively weak (1sec exposure time), I thought about increasing the Cadmium concentration. But I don't know if it actually would help something..
Since the taxonomy of ciliates is fastly changing, is there any database
assembling the taxonomy of ciliates. I know that WORMS is pretty good but
is it trustworthy? And is there any other databases for marine species?
I am also interested in fresh and brackish water ciliates' taxonomy.
It was very abundant in hypersaline waters from South Spain (150g/l approximately); it is over 0.5mm long and of black colour. We wonder if it is a ciliate species...
Does anyone know a function of thin thread connecting macronuclear nodules? I want to know it is a phenotype of presence/absence in a single species or a diagnostic character between species.
Zooplankton may have different types of epibionts, like diatoms, green algae, ciliates, bacteria, etc.
Many of these are free-living cells during the reproductive stage, but then attach to the host turning themselves into sessile individuals, attached by a mucilaginous stalk.
I can imagine the free-living cell simply encounters it's host via direct interception, then adheres to the carapace. But how is the in between mechanism? From first contact to final attachment? is the stalk formed immediately? or it is already developed and "waiting" for a trigger? If so, what is the "trigger" and what factors influence a successful attachment?
I am trying to prepare SEM from respiratory epithelial cells, to visualize cilia on the surface of the cells. I see cells and cilia, but everything is covered in a layer of 'mud', or 'webbing'. Does anyone know what could be the reason for that situation? I am a beginner in the area of SEM, so all suggestions are welcome!
cells from nasal brushing washed & attached to collagen-coated cover glasses
Fixation: 4% glutaraldehyde in 0,1M cacodylic acid, 1hr @ RT, 1hr @ 4oC
Wash: 3x 20 min, 0,1M cacodylic acid
Dehydration: 10,30,50,70 % EtOH -2 x 10 min in each conc, ON in 70% EtOH; next day: 90%, 100% - 2x10 min in each conc.
Observation of the wet material (no drying). Tried CPD & HDMS but got similar pictures - all cells were covered in something.
I expect the repeat to be the Oxytricha type [G4T4]n repeat motif, but am struggling to find a way to confirm this in the unknown ciliate.
I would like to find a way to perform a yeast-two-hybrid screening with Paramecium cDNA. Thank you in advance for any help
I am trying to image the chromosome ends of a ciliate using an oligonucleotide probe designed to hybridize with the 3'overhang.
I have search in all the literature about ciliate taxonomy and systematics that I have available and the only information I have found is that family Trichodinidae was first described by Claus in 1874.
I am using the cell line mIMCD3 to study the influence of some proteins in ciliogenesis and from a while I've experienced a new problem. Cells are not ciliated in a homogeneous way; there are clusters of cells among the slide where I have normal cilia (with expected length) and then around these clusters I have cells unable to form cilia or they do form it much later (delayed).
Did any of you experienced this problem? I thawed different vials, that should be fine, but no better outcome. Also I did not change serums or media brand.
I'm planning an experiment where I want to investigate the dietary preferences of four different predatory protists (two sarcodines, two ciliates). I also want to do some controls where they have no food in order to see how long they can survive so that I can better understand their population dynamics.
I can see two potential ways of performing this experiment - one is two put predator and prey together and observe abundances of both for a week or two which, when compared to the controls, will allow me to indirectly see how much feeding is taking place. The other is to either watch the predators under the microscope while they feed or else put them in a high density of prey and then sample them after a set time to see the stomach contents.
In order to do any of these options I need the predators to be free of contaminants. Papers speak of 'washing' the protists but don't seem to give details of how this is done. They also speak of taking individual protists but again, don't give details of how they are able to select one protist at a time.
I'm new to this field and don't have any experience working with protists so these may be very basic skills that every microbiologist knows, but is there anyone who can tell me how to wash protists and how you go about dealing with them on an individual basis?
I tried to predict some 18S rRNA structure of ciliate following recent publications. Especially for the variable region 2 and 4 of 18S rRNA. However, I couldn't get the same with the published results. Depending on the length of input sequence, the results were highly variable from the mfold and RNAstructure.
Could you inform me of a more detailed guide or manual to predict the structure? For example, how to prepare the input seq. The input seq should have stem region in begining of 5' and ending of 3' as a pair?