The caudal regeneration blastema is an accumulation of rapidly proliferating stem cells in the flatworm Macrostomum lignano
- Bernhard Egger1, 4Email author,
- Robert Gschwentner1,
- Michael W Hess2,
- Katharina T Nimeth1,
- Zbigniew Adamski3,
- Maxime Willems4,
- Reinhard Rieger^1 and
- Willi Salvenmoser1
© Egger et al; licensee BioMed Central Ltd. 2009
Received: 19 March 2009
Accepted: 15 July 2009
Published: 15 July 2009
Macrostomum lignano is a small free-living flatworm capable of regenerating all body parts posterior of the pharynx and anterior to the brain. We quantified the cellular composition of the caudal-most body region, the tail plate, and investigated regeneration of the tail plate in vivo and in semithin sections labeled with bromodeoxyuridine, a marker for stem cells (neoblasts) in S-phase.
The tail plate accomodates the male genital apparatus and consists of about 3,100 cells, about half of which are epidermal cells. A distinct regeneration blastema, characterized by a local accumulation of rapidly proliferating neoblasts and consisting of about 420 cells (excluding epidermal cells), was formed 24 hours after amputation. Differentiated cells in the blastema were observed two days after amputation (with about 920 blastema cells), while the male genital apparatus required four to five days for full differentiation. At all time points, mitoses were found within the blastema. At the place of organ differentiation, neoblasts did not replicate or divide. After three days, the blastema was made of about 1420 cells and gradually transformed into organ primordia, while the proliferation rate decreased. The cell number of the tail plate, including about 960 epidermal cells, was restored to 75% at this time point.
Regeneration after artificial amputation of the tail plate of adult specimens of Macrostomum lignano involves wound healing and the formation of a regeneration blastema. Neoblasts undergo extensive proliferation within the blastema. Proliferation patterns of S-phase neoblasts indicate that neoblasts are either determined to follow a specific cell fate not before, but after going through S-phase, or that they can be redetermined after S-phase. In pulse-chase experiments, dispersed distribution of label suggests that S-phase labeled progenitor cells of the male genital apparatus undergo further proliferation before differentiation, in contrast to progenitor cells of epidermal cells. Mitotic activity and proliferation within the blastema is a feature of M. lignano shared with many other regenerating animals.
A single type of cells in flatworms is responsible for regeneration, growth and tissue maintenance, the so-called neoblasts. These likely totipotent stem cells have a high nucleus to cytoplasm ratio, are the only dividing cells in juveniles and adults and have been shown to differentiate into diverse cell types [1–3].
The formation of a regeneration blastema is a response to amputation involving mainly cell proliferation, and describes the accumulation of undifferentiated or dedifferentiating cells at the wound site, often visible as an unpigmented bulge in an otherwise pigmented animal. Blastemas have not only been described in various flatworms , but also in annelids , molluscs , nemerteans , echinoderms , crustaceans , teleost fish , urodele amphibians , larval anuran amphibians , lizards  and some mammalians .
Even though the formation of a regeneration blastema after amputation or fission is a common occurrence in many bilaterians, flatworms show some peculiarities. One notable difference compared to vertebrates is that in flatworms seemingly no dedifferentiated cells contribute to the formation of the blastema, although redetermination of already determined stem cells may take place [15, 16]. Another specialty of the blastema in triclad flatworms (usually referred to as "planarians") is a high mitotic activity at the border between blastema and differentiated tissue, the so-called postblastema .
Within flatworms, blastema formation is described in acoels [3, 18], polyclads , triclads  and some – but not all – macrostomorphans [21, 22]. In catenulids, stem cells accumulate at the wound site, but these cells are split up into two groups, and are not forming a single blastema . Regeneration processes in rhabdocoels involve a small buildup of "cells of embryonic character" at the wound site  and can be interpreted as blastema formation.
Two species of the Macrostomorpha have been examined more closely: Head regenerates of Microstomum lineare, a species reproducing asexually by paratomy, show a similar distribution of S-phase cells as controls, and do not form a blastema . Contrary, regeneration in Macrostomum lignano involves the formation of a blastema, characterized morphologically by a bulge of unpigmented cells at the wound site [22, 25–27].
A large number of studies about regeneration and blastema properties in flatworms was undertaken with triclads, which have been chosen for their remarkable regeneration capacity, availability and their manageable size. However, their comparable large size complicates the quantification of a regeneration blastema, and labeling of S-phase neoblasts with the thymidine analogue bromodeoxyuridine (BrdU) was made possible only by supplying food containing BrdU or with micro-injections , and not by simple soaking in a BrdU solution as in M. lignano . Only recently, a soaking method was reported to be successful in the triclad Dugesia japonica, although BrdU incubation was prolonged for six hours instead of a 30 minute pulse . For these reasons, we have chosen the small flatworm Macrostomum lignano with a limited, but well-known regeneration capacity [26, 27] and a thoroughly documented and easily stainable stem cell system [1, 22, 26, 27, 29–31]. Thanks to its small size and its transparency, cells and organ systems can also be studied in vivo squeeze preparations.
In this study we quantified and categorized the tail plate, a body region in the caudal-most part of the flatworm M. lignano before and for the first three days after amputation and analyzed cell proliferation, the differentation of cell types and the build-up of organ primordia within the regeneration blastema.
Live squeeze preparations were made according to . Animals anesthetized in a 2:1 mixture of 7.14% MgCl2.6H2O and artificial seawater (ASW) were observed with interference contrast (Nomarski) microscopy. Measurements of blastema extension were done using pictures of slightly squeezed live animals. For staining of epidermal nuclei, living specimens were treated for 4 minutes with Hoechst 33342 (Sigma-Aldrich) at a concentration of 1:1000 diluted in ASW and then washed thoroughly in ASW. Anesthetized and squeezed animals were observed with fluorescence microscopy. In cell macerations and in fixed animals, Hoechst 33342 unspecifically stains all nuclei, but only epidermal nuclei in intact M. lignano. The chemical is not acutely toxic for the animals, which have been found to survive the treatment for at least seven days (personal observation).
Staining of fixed animals (whole mounts)
Animals were anesthetized in 7.14% MgCl2.6H2O for 5–10 min, fixed in 4% formaldehyde (FA) for 1 hour and washed with phosphate buffer saline with 0.1% Triton (PBS-T) for 10 minutes. Muscle F-actin was revealed using Alexa Fluor 488 phalloidin (Molecular Probes) diluted 1:200 in PBS-T, staining for 1 hour in the dark. For staining of the GYIRFamidergic nervous system, following fixation in FA the animals were washed in PBS-T for 30 min, in BSA-T (add 1% Albumin fraction V, Merck, to PBS-T) for 30 min, then incubated over night in a 1:500 solution of neat GYIRFamide antiserum in PBS at 4°C. The next day, animals were washed in PBS-T several times, in BSA-T for 15 min and then incubated in FITC-conjugated goat anti-guinea pig (DAKO) 1:200 in BSA-T for 1 hour. For labeling of S-phase nuclei, live animals were soaked in a 5 mM solution of 5-bromo-2'-deoxyuridine (BrdU, Sigma-Aldrich) in ASW for 30 min. In BrdU pulse experiments, soaking was performed just before anesthetization and fixation. In BrdU pulse-chase experiments, soaking was performed before amputation to allow for migration and differentiation of labeled cells during regeneration time. After fixation with 4% FA and the washing steps in PBS-T, animals were incubated in 0.15 mg/ml Protease XIV (Sigma-Aldrich) for about 20 min (until the epidermis appeared as a jagged instead of a smooth line) at 37°C and then treated with 0.1 M HCl (on ice) for 10 min. Specimens were then incubated in 2 M HCl at 37°C for 1 hour, rinsed in PBS, incubated in BSA-T for 30 min and then in primary mouse anti-BrdU antibody (1:600 in BSA-T, DAKO) over night at 4°C. Subsequently, animals were rinsed in PBS and then incubated in secondary goat anti-mouse antibody (FITC-conjugated, 1:150 in BSA-T, DAKO) for 1 hour for fluorescence labeling. For fluorescent double-labeling of S-phase cells with mitoses, a rabbit anti-phos-H3 antibody (Upstate Biotechnology) was added to the primary antibody solution in a concentration of 1:150, and visualized with a TRITC-conjugated swine-anti-rabbit antibody (Dako) 1:150 in the secondary antibody solution. For all stainings above, animals were washed in PBS after the last antibody incubation and mounted in Vectashield (Vector Labs). For permanent non-fluorescent labeling, instead of a FITC-conjugated secondary antibody, a biotinylated goat anti-mouse antibody was used to allow for the binding of a streptavidin and biotinylated horseradish peroxidase complex (StreptABComplex/HRP Duet, Mouse/Rabbit, DAKO), that was visualized with a chromogenic peroxidase substrate solution (DAB+ Chromogen, DakoCytomation). Concentrations were used according to manufacturer's instructions.
The tail plates of 20 adult specimens relaxed in MgCl2 were amputated and 10 tail plates each were transferred to 50 μl of calcium- and magnesium-free medium with 1% trypsin and incubated for 1 hour at 37°C. 50 μl of glycerol:glacial acetic acid:distilled water (1:1:6.5) and Hoechst 33342 for a final concentration of 1:1000 were added and the solution was gently pipetted up and down for about 30 min to obtain single cells. Cell countings were made with a Bürker's hemocytometer on a Leica DM 5000 fluorescent microscope.
Animals treated with BrdU, visualized by horseradish peroxidase/DAB+ Chromogen (see above), were dehydrated in a graded series of methanol, transferred in a 1:1 mixture of methanol and Spurr's resin  for at least 1 hour and embedded in Spurr's resin.
Untreated animals were fixed in 2.5% glutaraldehyde in 0.1 M cacodylate buffer with 9% sucrose for one hour and postfixed with 1% OsO4 in 0.1 M cacodylate buffer for one hour, dehydrated in a graded acetone series and embedded in Epon-Araldit  or Spurr's low viscosity resin.
Embedded specimens were cut for sagittal, horizontal and cross sections at 1 μm thickness with a Reichert Jung 2040 microtome and stained with methylene blue or Heidenhain's iron hematoxyline .
Microscopy and photographs
For live squeeze preparations, stained whole mounts and sections, a Reichert Jung Polyvar and a Leica DM 5000 light microscope were used. Photographs were taken with a Pixera Penguin 600CL and a The Imaging Source DFK 41F02 camera. Picture editing and drawing schemes was done with the free programs Inkscape  up to version 0.45 and GIMP  up to version 2.2.13. Some stained whole mounts were observed with confocal Zeiss LSM 510 and 710 microscopes.
Cryo-based transmission electron microscopy
High-pressure freezing and freeze-substitution were used to complement and evaluate data from conventional chemical fixation . Briefly, live animals in their culture medium were pipetted into cup-shaped aluminium specimen holders of a HPM010 high-pressure freezing apparatus (BAL-TEC, Balzers, Liechtenstein) and rapidly frozen at a pressure of approximately 2100 bar. Freeze-substitution was carried out with anhydrous acetone supplemented with 1% OsO4 and 0.2% uranyl acetate (at -90°C, 18 h), followed by Epon embedding. Semithin and ultrathin sections were stained according to standard procedures and viewed by brightfield light microscopy or transmission electron microscopy (with a CM120, FEI-Philips), respectively.
Blastema cell counts
The total blastema cell number and the percentage of BrdU-labeled and unlabeled cells was counted from semithin serial sections. In all sections containing a part of the blastema, all cells or nuclei were counted. In sections of animals labeled with BrdU (pulse or pulse-chase, see staining procedures), both labeled and unlabeled cells (nuclei) were counted.
Subsequently, the average blastema cell dimension was determined, i.e., through how many sections a single cell could be followed. This was done for 15–20 cells (separately for labeled and unlabeled cells) for each blastema. The total number of blastema cells was calculated by dividing the number of counted cells by the average blastema cell dimension, both for labeled and unlabeled cells. Epidermal cells covering the blastema were not included in blastema cell counts.
Cell numbers in the tail plate of intact animals
Cell types and numbers in the tail plate
Duo-gland adhesive systems
Other gland cells
Nerve cells (GYIRFamid)
Male genital apparatus
Other cell types
Nuclei of all epidermal cells were stained in living specimens with Hoechst 33342, which does not penetrate the epidermal layer in live animals and therefore specifically labels epidermal cells (Fig. 2E). The dorsal or the ventral cell number was counted up to the female genital opening and then multiplied by 2, as both sides were found to give similar cell numbers. The average number of epidermal cells posterior of the female genital opening was 1,575 ± 136 (n = 9). In TEM cross sections, 40–50% of all cells can be identified as epidermal cells (Fig. 2A), corroborating the fraction of epidermal cells found in Hoechst stainings.
The duo-gland adhesive systems are located at the posterior ventral tip of the tail plate, identifiable as rings protruding from the surface (Figs. 1B, D, 2A). They consist each of two gland cells and an anchor cell . The average number of duo-gland adhesive systems in standard animals was found to be 130 ± 17 (n = 13) for a total of 390 cells by multiplication with 3. Rhabdite glands were counted in live squeeze preparations for a total of 56 ± 6 (n = 9) on the ventral or dorsal side of the tail plate. Comparable numbers were obtained for the dorsal and the ventral side. Accounting for both sides gives 112 rhabdites on average per tail plate. The number of prostate glands in the tail plate of adult M. lignano is reported to be up to 35, found by labeling with a monoclonal antibody . Cyanophilic ("slime") glands (for their appearance see Fig. 2A) account for about 50 cells, inferred from ultrathin sections (Rieger, unpublished observations), adding up to about 197 gland cells other than duo-gland adhesive systems in the tail plate.
BrdU-labeling revealed the average number of S-phase cells in the tail plate to be 96 ± 29 (n = 15, Fig. 2D). Bode et al.  report that S-phase cells account for about 27% of the total neoblast population, rendering the average number of neoblasts in the tail plate to be 355 cells.
Muscle cells in the tail plate area were revealed by phalloidin staining. The muscle rings counted from the ventral (n = 7) or the dorsal (n = 5) side gave an average of 48 ± 7 (n = 12) muscle rings – often closely associated in pairs – per tail plate (Fig. 2F). As is known from phalloidin-rhodamine preparations and electron micrographs of M. hystricinum marinum , one muscle ring is composed of about 3 ring muscle cells, so that the calculated average number of ring muscle cells per tail plate is 144. The number of dorsoventral muscle cells in the tail plate of adult M. lignano is reported to be 40 . From the available data, the approximate number of muscle cells in the tail plate of M. lignano can be estimated as 183. Longitudinal muscles were not considered in the present work, because previous studies have shown that during regeneration most longitudinal fibers are elongated without build-up of new cell bodies . Diagonal fibers in Macrostomum are known to branch off of longitudinal fibers  and were not counted as well.
The number of nerve cells contributing to the tail plate was calculated from GYIRFamidergic (Fig. 2G) nervous system stainings in adult animals. Analyzing confocal stacks, the average number of GYIRFamidergic nervous cells was found to be 22 ± 1 (n = 5).
Some gut cells are cut off when amputating the animals posterior of the female genital opening. Being one of the largest cell types in M. lignano, the amputated number of these cells was estimated to be approximately 10 cells, inferred from semithin and TEM sections (data not shown).
The male genital apparatus is made up of the copulatory organ (stylet) and the vesicula granulorum, the seminal vesicle and the false seminal vesicle, each attached to the previous structure (Fig. 1C, F). About 35 prostate glands (see gland cells) reach into the stylet, which consists of about 8 cells and is lined with about 10 epithelial cells. The granular and seminal vesicles are lined with about 10 epithelial and 10 muscle cells, and 5 epithelial and 15 mucle cells, respectively. About 10 ring muscle cells (Fig. 2B) and 10 longitudinal muscle cells contribute to the musculature of the stylet. These estimations were obtained from TEM sections of another Macrostomum species, M. hystricinum marinum (Rieger, unpublished observations). All in all, about 78 cells make up the male genital apparatus (excluding prostate glands and sperm found in the seminal vesicles).
The sperm number in the tail plate may vary, depending on copulation frequency. Isolated worms tend to accumulate sperm in the seminal vesicles. An estimate of the average sperm number in the seminal vesicle and the false seminal vesicle is about 100 from live squeeze preparations, as well as from a confocal stack of Hoechst 33342-labeled sperm nuclei in the seminal vesicles.
Parenchyma cells, different kinds of nerve cells and other, unidentified cell types are estimated to comprise up to 200 cells in the tail plate.
The total number of cells in the tail plate amounts to about 3,110 cells (Tab. 1), about half of which are epidermal cells. In tissue macerations of 20 tail plates, 3,176 ± 40 cells with Hoechst-33342-labeled nuclei were counted in 21 grids of 1 mm2 using a hemocytometer, corroborating the number of about 3,100 cells given above. While not all cell numbers are equally accurate, they may indicate which cell types and numbers are to be regenerated after amputation.
The tail plate blastema
In the first four to six hours after cutting, the wound closure was still fragile and would sometimes break open in slightly squeezed animals anesthetized with MgCl2. After about 8 hours enough epidermal cells surrounding the wound flattened to cover the whole wound area (Fig. 3B).
The blastema was examined in vivo and in serial sagittal sections at three different time points: 24, 48 and 72 hours after amputation.
24 hours after amputation
An average of 5 ± 3 mitoses (n = 17) was identified in the blastema region in serial sections (Fig. 5A) and fluorescent confocal stacks (see Additional file 1A). Most of the mitoses were located at the anterior-most border (27%) and in the middle of the blastema (56%), but some mitoses were also found in the caudal-most part of the blastema (17%), even bordering epidermal cells at the posterior tip. About one tenth (9%) of all mitoses were situated in the dorsal third of the blastema. In BrdU pulse serial sections an average of 178 ± 36 (n = 2) S-phase cells was counted in the blastema, which made up 37% of all cells in the blastema (Fig. 5C–E). A majority of S-phase cells was found in the ventral and middle area of the blastema (Fig. 5E), only about one fifth (22%) of labeled cells were located in the dorsal blastema region. In BrdU pulse-chase experiments more than 200 cells were labeled with BrdU (210 ± 28, n = 2), constituting 58% of all blastema cells. Labeled cells were distributed evenly in the blastema (Fig. 5F, G).
New epidermal cells, identifiable by darker (ribosome-rich) cytoplasm, a round instead of a lobulated nucleus (Fig. 2C) and shorter cilia (see also Additional file 2), migrated to the wound area to replace lost epidermis (Fig. 5A), although labeled epidermal nuclei were not yet found in 24 hours BrdU pulse-chase experiments (Fig. 5F, G). Longitudinal and also circular muscle fibers could be detected in the blastema region. The main lateral nerve cords were already reconnected in a caudal loop (data not shown).
At this stage, several gland cells were already present in the blastema. Although rhabdite glands were predominantly found at the ventral and dorsal border of the blastema, sporadically they were also located at the posterior blastema border (Fig. 4B). Duo-gland adhesive systems were neither detected in sections nor in live squeeze preparations (Fig. 4A, B). Some dorsoventral muscle fibers were already restored (Fig. 5B). Necrotic cells by injury or apoptosis could be identified in serial sections, predominantly located at the anterior border of the blastema (Fig 5A inset). Cells within the blastema generally had a large nucleus and a prominent nucleolus and varied mainly in the staining intensity, with color ranging from light to dark blue in sections stained after Heidenhain (Fig. 5A, B).
48 hours after amputation
An average of 16 ± 4 (n = 17) mitoses was found in serial sections (Fig. 6A) and in fluorescent confocal stacks (see Additional file 1B). 49% of all mitoses were located at the anterior border and 41% in the central area of the blastema – few (10%) mitoses were found at the posterior tip. Only 16% of all mitoses were situated in the dorsal area of the blastema. In a BrdU pulse experiment (Fig. 6B, C), 236.6 S-phase cells were counted in serial sections, constituting 28% of all blastema cells. About one quarter (24%) of labeled cells were located in the dorsal blastema region. In BrdU pulse-chase experiments (Fig. 6D, E), the average number of S-phase cells found in serial sections was 363 ± 34 (n = 2), which is a fraction of 39% of all blastema cells.
BrdU pulse-chase experiments revealed several labeled cells in the epidermis after 48 hours (Fig. 6D, E). 22 ± 10 (n = 7) regenerated duo-gland adhesive systems were found in live animals and in serial sections (Figs. 4D, 6A), none of which showed BrdU label at this time point. Rhabdites were found interspersed between epidermal cells throughout and also at the caudal tip of the blastema, the former wound area (Fig. 6A). In one animal, the first presumptive signs of the regenerating male genital apparatus appeared. In the area of the emerging copulatory organ (i.e. the organ primordium) of a BrdU pulse animal, no labeled cells were present (Fig. 6C). No other formation of cells or clusters were apparent in serial sections of 48 hour regenerates.
72 hours after amputation
On average, 7 ± 2 mitoses were found per blastema (n = 6) in serial sections and confocal stacks. Most mitoses were found in the anterior (46%) or middle parts (48%) of the blastema. Regarding the dorso-ventral axis, most mitoses occured in the ventral (48%) or central (34%) rather than the dorsal area (18%). In a BrdU pulse experiment, labeled cells contributed to 10% (158 cells) to the blastema, no longer showing a dense accumulation of S-phase cells (Fig. 7F–H). As already seen in 48 hour blastemas, the growing anlage of the male genital primordium showed no label in BrdU pulse experiments (Fig. 7G). In BrdU pulse-chase experiments (n = 2), half (50% or 629.0 cells) of all blastema cells were labeled, including most cells of the male genital primordium (Fig. 7J–L). An increased number of epidermal cells was labeled in BrdU pulse-chase experiments compared to 24 and 48 hour blastemas. The label in cells of the genital primordium was generally weaker than in epidermal cells, often showing a sparse, freckled distribution.
After three days of regeneration, the differentiation of the largest organ system of the tail plate, the male genital apparatus, was at full activity. The tip of the stylet was already visible in vivo (Fig. 4E) as well as in sections (Fig. 7A, L). Attached to the base of the stylet was the developing vesicula granulorum lined with muscles (Fig. 7A–E). Long sensory cilia appeared at the caudal tip. A large number of duo-gland adhesive systems (51.0 ± 9.9, n = 3) was regenerated and could already be used for attaching to the substrate (see also Figs. 4F, 7A, G, H). Large gland cells with sizable secretion granules were already restored in the tail plate. The first duo-gland adhesive systems with labeled nuclei were found at this time point (Fig. 7K).
Four to five days after amputation of the tail plate, the stylet grew to full size, and at the same time the first sperm appeared in the rebuilt seminal vesicle, connected via the ductus ejaculatorius with the vesicula granulorum. In this time, M. lignano was able to restore the basic functionality of the tail plate, that is the ability to copulate and to transfer sperm, and the ability to effectively attach to the substrate. The further regeneration of the duo-gland adhesive systems happened only gradually and took between 2 and 6 more days (see also [26, 27]). Thus, the regeneration of the full number (about 130) duo-gland adhesive systems can be used as a final marker for complete regeneration.
Cryo-based specimen preparation
For the first time, rapid cryo-immobilisation by means of high-pressure freezing was used as a primary fixation technique for ultrastructural preparations in flatworms. Excellent fine structure preservation was achieved, comparable to published data on Caenorhabditis elegans and other multicellular organisms (see [40, 45] for reviews). Semi- and ultrathin sections from these preparations provided a good reference for evaluating the quality of chemically fixed samples of M. lignano, including our classification and counting of cell types. Generally, the morphological features reported from conventionally fixed samples (e.g. ) could be confirmed by this novel approach. In addition, the more reliable preservation of fine structure and antigenicity obtained with rapid freezing bears a great potential to allow more detailed insights into flatworm morphology. Finally, natively cryo-immobilised specimens should facilitate immuno-labeling of fixation-sensitive and/or easily translocated constituents .
Wound healing and blastema formation
The wound is closed about 2 hours after amputation by flattening of surrounding epidermal cells (Fig. 3A), but is still susceptible to pressure and will break open easily during the first 4–8 hours. Compared to other taxa, e.g. holothurians, which require 2–3 weeks for wound healing , wound healing in flatworms is a very rapid process. The flattening of epidermis cells was already described for M. lignano  and is a common process also found in many other flatworms, among them catenulids , triclads , rhabdocoels , and other macrostomorphans . A tail plate blastema is readily apparent 24 hours after amputation in M. lignano, but is most likely already present some time earlier. As the early blastema is located at the ventral side of the animal due to the contraction of ventral longitudinal muscle fibers , it can not easily be observed in vivo until about 24 hours after amputation.
A regeneration blastema may be defined as the accumulation of undifferentiated (or dedifferentiated) cells at the wound site as a response to amputation or injury, covered by old and new epithelial cells. Injury, both by artificial amputation and by fission for asexual reproduction, is a stimulus for forming a blastema, although the molecular nature of the stimulus is still unknown . One trigger causing the formation of a blastema is thought to be contact of the epidermis with the mesenchyme or the gut, or the dorso-ventral interaction of the epidermis at the wound site (see literature in ). However, intercalary regeneration (if the middle piece is removed and the anterior and posterior end are brought together) is not relying on these triggers .
In M. lignano, the tail plate blastema (as an accumulation of proliferating stem cells) changes into differentiating organ primordia at about 72 hours after amputation, when the majority of amputated body parts have already been regenerated and the ratio of S-phase and mitotic neoblasts decreases compared to earlier blastemas.
Indication of late determination or redetermination in neoblasts
In BrdU pulse-chase experiments with M. lignano, intact animals are incorporating BrdU into S-phase cells. Still, in serial sections it is evident that many of the cells labeled prior to amputation have become part of the blastema. This is especially obvious in the case of the male genital apparatus, whose cells are almost completely labeled in a pulse-3-days-chase experiment. An intact animal is not required to rebuild the genital apparatus, and after amputation of the tail plate only neoblasts distant from the genital apparatus remain. It appears unlikely that these distant S-phase cells were already committed to become part of the genital apparatus prior to entering S-phase.
Possible explanations are that these cells were not yet committed to follow a specific fate at replication time, or that they were committed, but were able to be redetermined during or after S-phase to contribute to the genital apparatus.
In an interesting experiment using Dugesia lugubris, a triclad with mixed ploidy (the same individual is characterized by different, but specific ploidies in testes, ovaries and somatic cells), it was shown that cells originally belonging to the gonads were contributing to building somatic tissue within the blastema , i.e. these gonadal cells were either dedifferentiated or, more likely, redetermined. Expression patterns of molecular markers led Agata and Watanabe  to suggest that neoblasts are already determined before going into S-phase in triclads, but lack of S-phase labeled cells makes interpretation of these results difficult.
Neoblasts are not replicating at the place of organ differentiation
None of the cells in the developing male genital apparatus were labeled in BrdU pulse experiments, neither after two days (Fig. 6C), nor after three days (Fig. 7G) of regeneration. Not a single mitosis was observed in this organ system. In a pulse-72-hours-chase experiment, all cells of the male genital apparatus were labeled, suggesting that the progenitor cell(s) of this organ undergo replication – but not at the place of organ differentiation. Replicating or dividing cells were absent in the epidermis as well. Epidermal replacement occurs by migration of mesodermally located neoblasts into the epidermis in Macrostomum and in triclads [1, 2]. The present study indicates that migration of determined neoblasts is not only essential in epidermal replacement, but also in the formation of complex organs such as the male genital apparatus.
Progenitor cells of complex organs might undergo multiple divisions before differentiation
In sections of BrdU pulse-3-days-chase experiments, nuclei of differentiating epidermal cells and cells of the duo-gland adhesive system exhibit a stronger label than cells contributing to the male genital apparatus (Fig. 7K, L). Labeled epidermal progenitors seem to divide just once and to differentiate directly into an epidermal cell without further proliferation, recognizable by a strong BrdU label of the nucleus. Cells contributing to the male genital apparatus, however, are weakly stained compared to epidermal cells (Fig. 7K, L) and S-phase neoblasts (Fig. 7G, H). Provided the differently labeled nuclei are not a staining artefact, this is an indication that neoblasts contributing to the genital organ are going through several S-phases, thus dispersing the BrdU label among a couple of daughter cells. Another explanation for weakly stained nuclei of cells contributing to the genital apparatus is a slower S-phase of its progenitor cells, thereby taking up less BrdU than e.g. epidermal cell progenitors. However, we observed such a weak, spot-like label only in pulse-chase, and not in pulse experiments, suggesting it is neither a staining artefact, nor the result of a slow S-phase.
Cell proliferation and differentiation in the blastema
After three days chasing time, cells labeled in S-phase before amputation and their progeny supply 50% of all blastema cells. The migration patterns of neoblasts into the blastema are not elucidated, but a previous study found that the response of the stem cell system to amputation in M. lignano is a local event restricted to the body regions near the wound .
In BrdU pulse-chase experiments, the first labeled epidermis cells covering the blastema appeared after two days, suggesting that about two days are required for replicating neoblasts to differentiate into an epidermal cell. However, newly built epidermal cells covering the blastema can already be observed after one day of regeneration (Fig. 5A). Similarly, duo-gland adhesive systems appeared in the blastema 48 hours after regeneration, whereas the first labeled duo-gland adhesive systems only appeared after 72 hours in pulse-chase experiments. The earliest differentiated cells in the blastema are likely the progeny of a pool of neoblasts arrested in G2-phase [29, 30], which are activated for tissue maintenance and also for regeneration .
The fraction of blastemal cells in S-phase is reduced from almost 40% at 24 hours to about 30% at 48 hours, and drops to only 10% 72 hours post-amputation. This and the ongoing differentiation of the male genital apparatus from its primordium hint at the eventual breakup of the blastema as an accumulation of undifferentiated cells at this time point.
Rate of regeneration
The caudal regeneration blastema in M. lignano is apparent 24 hours after amputation and grows rapidly by proliferation of neoblasts within the blastema. The regeneration process in this small flatworm can be readily quantified: during the first three days, 400–500 blastema cells are regenerated each day, starting with about 420 regenerated cells at 24 hours, 920 cells at 48 hours and 1420 cells at 72 hours after amputation. If replaced epidermal cells are included in the cell count, then 75% of the amputated tail plate, consisting of about 3,100 cells, have been replaced 72 hours after amputation. The largest organ of the tail plate, the male genital apparatus, is fully restored 4–5 days post-amputation.
This regeneration speed and the capacity of the obligatory sexually reproducing species M. lignano to regenerate reflects a likely adaptive response to known parasites and other environmental factors leading to the loss of body parts in their natural habitat . Asexually reproducing flatworms often show a higher regenerate rate than M. lignano: for instance, the macrostomorphan Microstomum lineare and the catenulid Stenostomum leucops only need 1–2 days for regeneration of the head [21, 53]. A particularly fast regenerating triclad is Dugesia tahitiensis, where 44% of all cells were described to be neoblasts or neoblast-like cells and which is reported to regenerate a head 2.5 days after regeneration .
Mitotic activity within the blastema
The tail plate blastema in M. lignano shows distinct mitoses in anterior, middle and even posterior parts of the blastema at all observed time points. About half of these mitoses\are located at the anterior border of the blastema, near the stump, which seems to be a preferred site for cell divisions.
In a 24 hour blastema, the majority of S-phase neoblasts is located at the ventral side of the blastema, which is possibly connected with the location of the main nerve cords that are presumably responsible for directing the regeneration process [4, 30]. The distribution pattern of neoblasts as found in the intact tail plate is reestablished after 3 or 4 days of regeneration.
Mitoses within the blastema have also been reported in an acoel flatworm . In annelids  and nemerteans , mitotic divisions take place within the blastema as well. In crustaceans, the blastema grows through mitotic divisions of immigrated cells . Deuterostomes that build a regeneration blastema show a similar spatial pattern regarding cell proliferation and mitoses: in crinoids, the blastema is one of the prefered sites of cell proliferation . In urodeles, mitoses occur throughout the regeneration blastema, especially at the anterior border . In teleost fish such as zebrafish, the blastema is formed by immigration of proliferating cells undergoing division within and at the base of the blastema . Interestingly, blastemas in triclad flatworms have been described as lacking mitoses within the blastema itself, having mitoses only in the so-called postblastema, an area of the stump adjacent to the blastema .
Flatworms are popular organisms for stem-cell and regeneration research due to a widespread and pronounced regeneration capacity and a likely totipotent stem-cell system even in adult animals. Macrostomum lignano is a well-suited model for quantitative regeneration studies, as it is comparably small and particularly amenable to cell proliferation markers and new fixation techniques such as high pressure freezing.
In this study we provide a detailled profile of cell proliferation and differentiation dynamics in the caudal blastema of the small flatworm M. lignano. We can clearly show that the blastema is a highly active center of proliferation, and that mitoses commonly occur within the blastema. This data set opens the way for successive studies on the migration of neoblasts into the blastema and the control of neoblasts in cell and tissue renewal. Comparative studies on blastema formation in other flatworms, particularly in triclads, are warranted to gain insights into common and derived patterns of regeneration in flatworms.
In memoriam Reinhard Rieger, a great friend and teacher. David Halton and Angela Mousley kindly provided a GYIRFamide antibody. Bernd Pelster provided access to a laser scanning microscope. We thank Karin Gutleben for technical assistance with cryopreparations for TEM, and Zeiss for the recording of stacks on an LSM 710 for demonstration purposes. This work was supported by a postdoctoral grant from the Francqui Fondation and a grant from the Austrian Exchange Service (PL 04/2008) to B. E., by the Austrian Science Fund projects 15204 and 16618 granted to R. R., by grants from Österreichische Nationalbank-Jubiläumsfonds (P-11050), Tiroler Wissenschaftsfonds (P-UNI-0404/100) and from Tiroler Landeskrankenhaus – Universitätskliniken to M. W. H. and by a doctoral grant from the Institute for the Promotion of Innovation through Science and Technology in Flanders to M. W. 3 anonymous reviewers are to be thanked for helpful suggestions improving the manuscript.
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