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PTEN Redundancy: Overexpressing lpten, a Homolog of Dictyostelium discoideum ptenA, the Ortholog of Human PTEN, Rescues All Behavioral Defects of the Mutant ptenA

  • Daniel F. Lusche,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Deborah Wessels,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Nicole A. Richardson,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Kanoe B. Russell,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Brett M. Hanson,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Benjamin A. Soll,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • Benjamin H. Lin,

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

  • David R. Soll

    david-soll@uiowa.edu

    Affiliation: Monoclonal Antibody Research Institute and Developmental Studies Hybridoma Bank, Department of Biology, The University of Iowa, Iowa City, Iowa, United States of America

PTEN Redundancy: Overexpressing lpten, a Homolog of Dictyostelium discoideum ptenA, the Ortholog of Human PTEN, Rescues All Behavioral Defects of the Mutant ptenA

  • Daniel F. Lusche, 
  • Deborah Wessels, 
  • Nicole A. Richardson, 
  • Kanoe B. Russell, 
  • Brett M. Hanson, 
  • Benjamin A. Soll, 
  • Benjamin H. Lin, 
  • David R. Soll
PLOS
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Abstract

Mutations in the tumor suppressor gene PTEN are associated with a significant proportion of human cancers. Because the human genome also contains several homologs of PTEN, we considered the hypothesis that if a homolog, functionally redundant with PTEN, can be overexpressed, it may rescue the defects of a PTEN mutant. We have performed an initial test of this hypothesis in the model system Dictyostelium discoideum, which contains an ortholog of human PTEN, ptenA. Deletion of ptenA results in defects in motility, chemotaxis, aggregation and multicellular morphogenesis. D. discoideum also contains lpten, a newly discovered homolog of ptenA. Overexpressing lpten completely rescues all developmental and behavioral defects of the D. discoideum mutant ptenA. This hypothesis must now be tested in human cells.

Introduction

PTEN is one of the most commonly mutated tumor suppressor genes in the progression of human cancers [1][3]. It has been demonstrated to play a prominent role in several cellular behaviors, including basic cell motility, chemotaxis and invasion [4][10]. PTEN functions as a phosphatase that regulates the signal transduction molecule phosphatidylinositol-3, 4, 5-triphosphate (PIP3) [11]. There are three homologs of the PTEN gene in the human genome [12][16]. In addition, Poliseno et al. (2010) [17], [18] found that a PTEN pseudogene, PTENP1, regulates the level of PTEN protein and acts as a growth suppressor. The presence of PTEN homologs in the human genome, therefore, raises the possibility that one of them may be able to substitute functionally for a mutated PTEN under inducing conditions, thus suppressing tumorigenesis, a possibility heretofore not tested.

The amoeba Dictyostelium discoideum, an exceptional model for studying the regulation of human cell motility and chemotaxis [19][27], contains the gene ptenA, an ortholog of the human PTEN gene. Deletion of ptenA in D.discoideum causes major defects in lateral pseudopod suppression, motility, chemotaxis and natural aggregation [28][34]. As is the case for human PTEN, PtenA in D.discoideum dephosphorylates phospahtidylinositol (3,4,5)-trisphosphate (PIP3) to form phophatidylinositol (4,5)-bisphosphate (PIP2) [35], [36] and mediates PIP3 oscillations [37][41], which correlate with actin polymerization and pseudopod extension [30], [39][43]. PtenA was originally thought to be the sole phosphatase for the dephosphorylation of PIP3 to PIP2 in D. discoideum. However, after global stimulation of ptenA cells with the chemoattractant cAMP, the concentration of PIP3 increases, but then declines [36], indicating that PIP3 is degraded to PIP2 in the absence of PtenA, presumably by another phosphatase. Moreover, Hoeller and Kay [32] demonstrated that when suspensions of ptenA cells were pulsed with cAMP to induce chemotactic responsiveness, they were able to undergo efficient chemotaxis. However, unlike earlier studies in which the concentration of the cAMP gradient, generated in vitro was in the range of that estimated for the gradient in the front of a natural cAMP wave [44], Hoeller and Kay [32] employed a cAMP gradient generated in a concentration range 10 times higher than that employed in the prior studies of ptenA chemotaxis [29], [30] and, therefore, 10 times higher than that estimated for the natural cAMP wave that induces chemotaxis in natural populations [44]. The studies of PIP3 degradation in ptenA cells after global cAMP stimulation [36] and chemotaxis of ptenA cells in high cAMP concentration gradients [32], suggested to us that there might be an alternative PIP3 phosphatase that could substitute for ptenA.

We therefore searched the D.discoideum database (http://dictybase.org/) and found a second ortholog of human PTEN and homolog of ptenA [28], [29], which we named lpten because it contained unique LIM domains. Here we show that cells of the lpten deletion mutant, lpten, exhibit defects in behavior similar to those in ptenA cells, but the defects are far weaker. To test for redundant function, we overexpressed lpten in a ptenA background. Overexpression resulted in the complete normalization of the defective behaviors of ptenA cells. The ptenA defects that were normalized included the following: abnormal aggregation, the absence of multicellular morphogenesis, the loss of lateral pseudopod suppression, increased turning, decreased cellular velocity, aberrant chemotaxis in a cAMP gradient generated in the standard concentration range and aberrant natural aggregation. We further show that pulsing ptenA cells with cAMP, which induces chemotactic competency in a high cAMP concentration gradient [32], is accompanied by up-regulation of lpten expression. We therefore conclude that lpten plays a similar, but less prominent in pseudopod suppression, motility and chemotaxis role than its homolog ptenA, but when overexpressed in the ptenA mutant, rescues all of the ptenA defects. This raises the question of whether any of the homologs of human PTEN might also be induced to function redundantly in cancer cells carrying mutations in PTEN.

Material and Methods

Strain maintenance, growth and development

The ptenA strain DBS0252655 [32] and the parental wild type strain Ax2 [45] were provided by the Dictyostelium stock center (http://dictybase.org/StockCenter/StockCenter.html). Methods for growing cells, initiating development and obtaining aggregation-competent amoebae have been described previously in detail [30], [46][48]. In brief, development was initiated by washing growth phase cells with buffer and distributing them on filterpads or on HAB04700 nitrocellulose filter pads (Millipore, Billerica, MA, USA) saturated with buffered salts solution (BSS) [49], as previously described [48], [50], [51].

DNA, RNA purification, cloning and sequencing

Isolation, purification, amplification and sequencing of all the genomic DNA, RNA and cDNA fragments from D. discoideum Ax2, mutant strains and plasmids was done as previously described [48]. Plasmids and competent cells were obtained from Life Technologies, (Carslbad CA, USA) [48]. For RNA, recombinant RNasin Ribonuclease (Promega, Madison, WI, USA) was added to inhibit RNA degradation. RNA was additionally purified from residual genomic DNA by using RNAeasyPlus (Qiagen, Ventura, CA, USA) according to the manufacturer's instructions. The primers used in this study are listed in a Table S1. Transformants were generated as described [48] and selected for using either 10 µg/ml Blasticidin S (Enzo Life Science, Farmingdale, NY, USA) and/or 20–70 µg/ml G418 (Sigma-Aldrich, St.Louis, USA). For clonal growth selection of the ptenA/lptenoe and lpten/lptenoe strains, cells were sorted by FACS as described [48].

Generation of a Dictyostelium discoideum knock out strain

A plasmid was generated that contained a bsr resistance cassette containing the gene coding for blasticidin deaminase flanked by lpten genomic fragments, as described by Torija et al [52] and diagrammed in Figure 1. In brief, a genomic fragment (F1) (Figure 1C) containing the lpten open reading frame and upstream and downstream regions was cloned and incubated in the presence of a PvuII-digested EZTN-plasmid (Epicenter, Madison, WI, USA), which contained a transposon bearing the Blasticidin S resistance marker [53]. Transposase was used to insert the transposon carrying the bsr gene into the lpten-containing plasmid (Epicentre). Transformed bacteria were selected for by tetracyclin (15 µg/ml) and kanamycin (50 µg/ml). Bacterial colonies bearing the plasmid that had a transposon within the genomic fragment were identified using primer M13, T7 and EZTN-R (Table S1). For D. discoideum Ax2 [32], [45] transformation, a fragment of the plasmid carrying the insert containing the bsr-resistance cassette close to the 5′ end of the lpten coding region was amplified as described by Torija et al. [52], except for the use of Expand Long Template PCR Polymerase (Roche, Indianapolis, IN, USA) [48]. Selection was done with increasing Blasticidin S concentrations. Surviving cells were clonally plated on nutrient plates in the presence of 30 µg/ml Blastidicin S and Klebsiella aerogenes. Colonies were harvested using MasterAmp Buccal Swab DNA extraction solution (Epicentre) and subjected to D. discoideum colony PCR [48], [52].

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Figure 1. Lpten is a homolog of ptenA and an ortholog of human PTEN.

lpten was disrupted to produce the lpten null mutant lpten. A. A comparison of Lpten and PtenA. The number of amino acids, the two conserved domains, CDC14 and PTEN-C2, and the LIM domains, are indicated. B. RT-PCR revealed that lpten is up-regulated during aggregation. lpten expression during development was assessed by RT-PCR and quantified by densitometry. lpten expression was up-regulated more than 10 fold. P1and P2 (see Table S1) demark the positions of the primers used to amplify the 300bp lpten cDNA fragment (F). RT-PCR of the large subunit ribosomal RNA, rnlA, was assessed for comparability of gel loading. C. Scheme for lpten disruption. The positions of primers P3 to P7 (see Table S1) are demarcated for amplification of lpten in control Ax2 and lpten cells, to generate the undisrupted lpten genomic fragment F1, the disrupted lpten genomic fragment of lpten, F2 genomic fragment F2, and a partial lpten genomic fragment with a partial bsr cassette, F3. D. Verification of lpten disruption by PCR. See panel C for the positions of the primers to generate fragments F1, F2 and F3. E. Verification that the lpten transcript is missing in the lpten mutant using RT-PCR with the primers LptenFW and PtencDNArv for ptenA, and PtenAcDNAFW and ptencDNArv to demonstrate the presence of ptenA in lpten. See Table S1 for description of primers. F. The completion of multicellular morphogenesis by the formation of fruiting bodies in control Ax2 cells. G. The absence of morphogenesis by ptenA cells. H. The completion of multicellular morphogenesis by lpten cells.

http://dx.doi.org/10.1371/journal.pone.0108495.g001

Generation of lpten overexpression constructs

To obtain an RFP-Lpten fusion, we amplified and cloned the coding region of lpten into the extrachromosomal plasmid pDM354 [54]. Cloning and recombination of the lpten cDNA were performed as described [48]. Transformed bacterial clones were identified by colony PCR.

RNA expression analyses

To study expression levels, RT-PCR was performed using the LongRange 2Step RT-PCR Kit (Qiagen) [48]. 2 µg of total RNA, pretreated at 65°C for 5 min, underwent the reverse transcription reaction in a total volume of 20 µl using OligodT primer supplied by the manufacturer. The resulting cDNA was amplified using the Long Range Expand Polymerase Kit (Roche, Indianapolis, IN) and primer P1 and P2 (Table S1, Figure 1). RNA expression levels were quantified under subsaturation conditions as described [55], using the densitometry function of the 2D-DIAS software program [56].

Analyses of basic cell behavior and chemotaxis

For analyses of basic motility in the absence of chemoattractant and during chemotaxis, cells were harvested from developmental filters at the onset of aggregation, when velocity and chemotactic responsiveness were maximal [57]. For basic behavior in buffer, cells were analyzed on the glass wall of a Sykes-Moore chamber perfused with the buffer BSS according to methods previously described [20], [58][60]. The methods for measuring chemotaxis in a Zigmond chamber have also been described in detail elsewhere [60][63]. For a “low cAMP concentration” gradient, the source well contained 1 µM cAMP. For a “high cAMP concentration” gradient, the source well contained 10 µM cAMP.

2D- and 3D-DIAS analyses of cell behavior

Cell images were digitally acquired using iStopMotion software (Boinx Software, www.boinx.com) and converted to QuickTime format for edge detection, perimeter reconstruction and motion analysis of cell behavior with 2D-DIAS software [64], as previously described [58], [65]. Descriptions of motility and chemotaxis parameters are presented in table S2 [58], [64], [65]. For 3D reconstruction, cells were optically sectioned and analyzed as previously described [20], [58], [59], [66][68], except that the resulting QuickTime movies of optical sections were exported into jpeg files and converted into JDIAS movies using an up-graded version of 3D-DIAS ([20], [58], [69], JDIAS 4.1 (Soll et al. 2014 in prep.). The in-focus perimeters were automatically outlined in each optical section using a pixel complexity algorithm [64], [70]. Pseudopods were manually traced.

Analyses of cell behavior in a natural wave

Natural waves were relayed in populations of cells aggregating on a plastic surface in submerged cultures in 35 mm Petri dishes (Fisherbrand, Pittsburg, PA). Cell behavior was recorded and motion analyzed as previously described [30], [66], [71], [72]. Cell behavior in this case was analyzed using JDIAS 4.1.

cAMP-pulsing of cells in suspension

Cells were pulsed as described by Hoeller and Kay [32]. In brief, 2×107 cells from a growth culture were washed free of nutrients, shaken in a suspension culture for 1h in buffered salts solution, and subsequently pulsed with 80 nM cAMP at 6 min intervals for 6 h, until aggregate formation was visually observed.

Results

Lpten is a homolog of ptenA

PtenA of D. discoideum [28], [29] contains two functionally important and conserved domains, which are present in human PTEN, a CDC14-dual specificity phosphatase (protein cluster COG2453) [73], found in members of the protein tyrosine phosphatase superfamily, and the lipid-C2-binding domain, Pten-C2 (PFAM10409) [74] (Figure 1A). A database search of the genome sequence of D. discoideum revealed a second ortholog of the human PTEN gene, lpten, (accession number KF430369), which encodes a protein that also contains the conserved CDC14 dual specificity phosphatase domain and the lipid-C2 binding domain (Figure 1A). In addition, this homolog contains five LIM domains that together contain a total of 38 putative zinc-binding sites (Figure 1A). Because of the LIM domains, we have named this ortholog lpten. The amplified cDNA of lpten encodes a putative protein of 114 KDa.

Expression of lpten

The ptenA expression was previously shown to be low during D. discoideum growth and to increase during the preaggregative period of development [75], [76]. A reverse transcriptase-polymerase chain reaction (RT-PCR) was employed to assess lpten expression in parental Ax2 cells during growth and at the end of the preaggregative period preceding chemotaxis, using a 300 bp probe (F) that spanned exons 3 and 4, as diagrammed in Figure 1B. Lpten was expressed in log phase cells (0 hours) at a very low level and was dramatically up-regulated, approximately ten fold or more in developing cultures at the onset of aggregation (8 hours) (Figure 1B).

Disruption of lpten and mutant rescue

To disrupt lpten, Ax2 cells were transformed with an integrative construct, as diagrammed in Figure 1C. Integration was confirmed by PCR (Figure 1D), using primers P5 and P6 to generate fragment F2, as diagrammed in Figure 1C. To further confirm integration, a portion of the disrupted lpten gene was amplified with primers P7 and P6, to generate fragment F3 (Figure 1C and D). Sequencing of the product F3 confirmed integration. In contrast to ptenA cells, which exhibited a major increase in generation time from 9 to 14 hours [30], [31], lpten cells exhibited a generation time of approximately 8 hours, similar to that of the parental strain Ax2 cells. And in contrast to ptenA cells, which do not complete aggregation (Figure 1G), lpten cells underwent aggregation and multicellular morphogenesis, forming fruiting bodies (Figure 1H). The lpten mutant was rescued by transformation with a plasmid containing lpten fused to rfp under the regulation of the actin 15 promoter. The complemented mutant strain, lpten/lptenoe, grew with the same generation time as parental Ax2 cells, aggregated and formed fruiting bodies (data not shown). Therefore, deleting lpten resulted in no measurable growth or obvious developmental defect.

lpten cells exhibit a minor defect in basic cell motility

Using computer-assisted 2D and 3D reconstruction and motion analysis systems, we previously demonstrated that aggregation-competent ptenA cells perfused with a K+-based buffer [30], [77] lacking chemoattractant exhibited a 50% decrease in velocity, a major increase in turning and a four-fold increase in lateral pseudopod formation [30]. Using the same computer-assisted methods, we found that lpten cells exhibited basic behavioral defects similar to those of ptenA [30] cells, in instantaneous velocity, percent cells with velocities ≥9 µm per minute and turning (Figure 2A). However, the defects although significant (p value <0.05), were less pronounced. The defects were evident in comparisons of computer-reconstructed cell perimeter tracks (Figure 2C), when compared to those of parental Ax2 cells (Figure 2B) or complemented lpten/lptenoe cells (Figure 2D). 3D reconstructions performed with 3D-DIAS software [58], [64], [70] revealed that lpten cells, like ptenA cells [30], formed lateral pseudopods, which initiate turns, at frequencies higher than Ax2 and lpten/lptenoe (Figure 2E, G and F, respectively). 2D measurements of the frequency of lateral pseudopods formed by reconstructed control (Ax2) cells, lpten cells and lpten/lptenoe cells, supported this conclusion (Figure 2G). The frequency of the mutant was over twice that of Ax2 and lpten/lptenoe cells (Figure 2G).

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Figure 2. lpten cells translocating in buffer in the absence of chemoattractant exhibit defects in velocity, turning and the suppression of lateral pseudopod formation.

Cells were analyzed in a perfusion chamber through which buffer without attractant was pumped. A. 2D motility parameters of Ax2, lpten and ptenA/lptenoe cells assessed with 2D-DIAS software. B, C, D. 2D-DIAS reconstructions of cell perimeters to generate tracks. Arrows denote net direction, and the blue-filled perimeters represent the last cell positions in the tracks. E, F. 3D-DIAS reconstructions at 0° (top view) and 90° (side view) of representative Ax2 and lpten cells, respectively, denoting pseudopods (red). Note that the multiple lateral pseudopods formed by lpten cells, were primarily off the substrate. a, anterior end of cell; p, posterior end of cell; lps, lateral pseudopod. G. 2D analysis of lateral pseudopod formation. Inst. vel., instantaneous velocity; No. turns per 10 min., number of turns per 10 minutes; Percent mot. cells, percent motile cells. Parameters are presented as the means ± standard deviations. T-test was used to determine p values. Parameters are defined in Table S2.

http://dx.doi.org/10.1371/journal.pone.0108495.g002

lpten cells undergo normal cAMP chemotaxis, but still are defective in suppressing lateral pseudopod formation

We previously demonstrated that ptenA cells undergoing positive chemotaxis in a spatial gradient of cAMP generated in the concentration range estimated for the front of a natural wave [44] (i.e., low cAMP concentration gradient), exhibited approximately a 50% decrease in velocity and a similar decrease in directional persistence [30]. Moreover, the efficiency of chemotaxis, measured by the chemotactic index (CI), was reduced by more than 50% [30]. Under identical conditions, lpten cells moved with an average velocity, average directional persistence, average chemotactic index (CI) and percent cells with a positive CI, statistically indistinguishable, using the student T-test (data not shown), from that of parental Ax2 cells and complemented lpten/lptenoe cells (Figure 3A). Computer-reconstructed perimeter plots revealed similar directionality up a low cAMP concentration gradient (Figure 3B, C, D), but lpten cells were still defective in suppressing lateral pseudopod formation (Figure 3C), as is evident when the perimeter tracks of mutant cells are compared to those of Ax2 (Figure 3B) and lpten/lptenoe cells (Figure 3D). This was demonstrated in the analysis of the frequency of lateral pseudopod formation (Figure 3E). 3D reconstructions revealed that the majority of the excess lateral pseudopods in cAMP gradients were formed by lpten cells off the substratum (data not shown), as was evident in buffer in the absence of cAMP (Figure 2A, F). Lateral pseudopods that contact the substratum force turns [78]. Hence, the formation of excess lateral pseudopods off the substratum did not result in a significant increase in turning, which may explain why there was no significant decrease in the CI.

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Figure 3. lpten cells undergo normal chemotaxis in the low cAMP concentration gradient generated in the estimated for that of the natural wave.

The gradient was generated in BSS buffer, in which K+ and Na+ are the facilitating cations. lpten cells, however, are still defective in suppressing lateral pseudopod formation. A. 2D motility and chemotaxis parameters, assessed by 2D-DIAS software of Ax2, lpten and lpten/lptenoe cells undergoing chemotaxis in a low cAMP concnetration gradient. B, C, D. 2D-DIAS-reconstructed perimeter tracks of representative cells. The large arrows at panel bottoms denote the net direction of the increasing cAMP gradient. “Sink”, trough with buffer alone; “Source”, trough with buffer plus 1 µM cAMP. E. 2D analysis of lateral pseudopod formation. Direct. Persist, directional persistence; chem. index, Chemotactic Index (CI); Percent pos. chem., percent cells with a positive CI. See legend to Figure 2 for additional definitions and details. Parameters are defined in Table S2.

http://dx.doi.org/10.1371/journal.pone.0108495.g003

Generating a ptenA/lptenoe strain

The similarities between the strong behavioral defects of the ptenA mutant and the weaker defects of the lpten mutant, suggested that the two homologs may play overlapping roles in basic cell motility and chemotaxis. We therefore tested whether overexpressing lpten in the ptenA mutant would partially alleviate, or even rescue, the severe defects exhibited by ptenA cells. The ptenA mutant was transformed with an expression plasmid in which the cloned lpten coding region was placed under regulation of the strong actin15 promoter and fused in frame at its 3′ end with red fluorescent protein (rfp) [79] (Figure 4A). Expression of the entire 3.7 Kb lpten rfp mRNA was verified using RT-PCR with primers P8 and P9 (Figure 4A, Table S1). Upon achieving chemotactic responsiveness, aggregation-competent cells of the transformed line ptenA/lptenoe expressed approximately 10 times as much lpten mRNA as the untransformed ptenA mutant (Figure 4B, inserted box). Overexpression of lpten rescued the developmental defects of the ptenA mutant, resulting in normal aggregation (data not shown) and the formation of normal fruiting bodies (compare Figures 4C, D and E).

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Figure 4. Overexpressing lpten in the ptenA mutant.

A. The transformation vector used to generate strains ptenA/lptenoe, in which lpten is under the regulation of the actin 15 (act15) promoter, fused in frame at the 3′ end to the red fluorescent protein gene (rfp) and terminating with a 3′ actin 8 gene sequence. The positions of the primers P8 and P9, for generating the lpten-rfp cDNA, are denoted. Insert shows verification of the lpten-rfp cDNA by PCR. B. lpten is expressed in ptenA/lptenoe cells at levels more than 10 times that in the parent ptenA mutant. The positions of the primers (P1, P2) for RT-PCR of the 300 bp lpten fragment (F) are denoted. In the insert to the right of panel B, RT-PCR products of chemotactically responsive ptenA and ptenA/lptenoe cells reveals overexpression of lpten in the latter. Densitometry measurements revealed>10 fold overexpression. C. Fruiting body formation in Ax2 cultures. D. The absence of fruiting body formation in ptenA cultures. E. Fruiting body formation in ptenA/lptenoe cultures. See Table S1 for description of primers.

http://dx.doi.org/10.1371/journal.pone.0108495.g004

Overexpression of lpten rescues the basic behavioral and chemotactic defects of ptenA cells

As previously demonstrated [29], [30], cells of the ptenA mutant originally generated by Iijima and Devreotes [29], did not undergo morphogenesis on filter pads saturated with a K+-based buffer. Furthermore, when incubated on pads saturated with K+-based buffer to attain chemotactic competence and then assessed for basic motile behavior on the glass surface of a chamber perfused with K+-based buffer lacking cAMP, these cells crawled at less than half the average velocity of control cells and with less than half the directional persistence. These same characteristics were observed in the ptenA mutant used here, which was generated by Hoeller and Kay [32] (Figure 5A). The abnormal behavior of ptenA cells was obvious, when computer-reconstructed perimeter tracks of control and ptenA cells translocating in buffer were compared (Figure 5B and C). The ptenA cells translocating in buffer also formed lateral pseudopods at frequencies close to twice that of control cells (Figure 5E), as was the case for the lpten strains (Figure 2G). Overexpression of lpten in ptenA/lptenoe cells rescued every motility defect in the basic behavior of cells migrating in buffer in the absence of chemoattractant (Figure 5A), resulting in normal perimeter tracks (Figure 5D) and restored suppression of lateral pseudopod formation (Figure 5E).

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Figure 5. Overexpression of lpten rescues the basic behavioral defects of ptenA cells that are translocating in buffer, and both the behavioral and chemotactic defects in a cAMP gradient generated in the concentration range of the natural wave.

A. 2D motility parameters of cells translocating in buffer, assessed by 2D-DIAS software. B, C, D. 2D-DIAS reconstructions of perimeter tracks of Ax2, ptenA and ptenA/lptenoe cells, respectively, translocating in buffer. E. 2D analysis of lateral pseudopod formation in buffer. F. 2D motility and chemotaxis parameters assessed by 2D-DIAS software during chemotaxis in a low cAMP concentration gradient. G, H, I. Perimeter tracks of cells in a low cAMP concentration gradient. J. 2D analysis of lateral pseudopod formation during chemotaxis in a low cAMP concentration gradient. See the legend to Figure 2 for explanations of panels A through E, and the legend to Figure 2 and 3 for explanations of panels F through J.

http://dx.doi.org/10.1371/journal.pone.0108495.g005

And, as previously demonstrated, ptenA cells exhibited the same motility defects in a low cAMP concentration gradient, as they did in buffer alone, as well as a dramatic decrease in chemotactic responsiveness [29], [30] (Figure 5F, H, J). Overexpression of lpten in ptenA/lptenoe cells rescued every motility and chemotaxis defect (Figure 5F), resulting in directed motility tracks up a gradient (Figure 5I) and restored suppression of lateral pseudopod formation (Figure 5J).

Overexpression of lpten rescues the ptenA defect in natural aggregation

Finally, as Wessels et al. [30] demonstrated, ptenA cells [32] are defective in natural aggregation. In a natural aggregation territory, parental Ax2 cells moved in a highly directed (Figure 6A) and cyclic fashion towards aggregation centers, increasing velocity in the front of each relayed, outwardly moving, non-dissipating wave of cAMP (velocity plots for two representative neighboring cells in the lower portion of Figure 6A). This resulted in centroid tracks that were directed at the source of chemotactic waves. Cells decreased velocity in the back of each wave, then reassessed directionality at the onset of the front of each wave, adjusting for deviations in direction during the translocation phase [48], [51]. To assess aggregation centers in ptenA cell populations, which do not complete normal aggregation, we retrospectively identified the point in each putative aggregation territory to which cells made net directional progress. Although the ptenA cells on average did make net progress towards the interpreted aggregation centers (Figure 6B, upper portion) and exhibited cyclic behavior (Figure 6B, lower portion), their centroid tracks were stunted and far less directional (i.e., less oriented on average in the direction of the interpreted aggregation center) (Figure 6B, upper portion) and cycling was more erratic (Figure 6B, lower portion). ptenA cells tended to undergo far more directional changes than control cells, resulting from sharp turns away from the interpreted aggregation center. Overexpression of lpten in ptenA/lptenoe cells restored normal behavior in a natural aggregation territory (Figure 6C). Cells surged in the front of each wave (Figure 6C, lower portion) and moved in a relatively directed fashion, with far fewer sharp turns, towards the aggregation center (Figure 6C, upper portion), in a manner similar to that of parental Ax2 cells (Figure 6A, upper portion).

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Figure 6. Overexpression of lpten rescues the behavioral defects exhibited by homogeneous populations of ptenA cells undergoing chemotaxis in natural aggregation territories in submerged cultures on glass.

A, B, C. The centroid tracks of four neighboring cells representative of the general behavior of Ax2, ptenA and ptenA/lptenoe populations, respectively, are presented in relation to the aggregation centers of Ax2 and ptenA/lptenoe cells, and the interpreted aggregation center of ptenA, deduced retrospectively by the direction of net translocation of groups of cells, in the upper half of each panel. The first (1) and last (150) centered in the centroid tracks are noted. In lower half of each panel, the velocity plots are presented for two respective cells. For normal cells, the peaks of velocity have been shown to correlate with the front of each relayed natural wave.

http://dx.doi.org/10.1371/journal.pone.0108495.g006

Pulsing ptenA cells up-regulates lpten and rescues chemotaxis in high, but not low, cAMP concentration gradients

In performing this study, one apparent controversy had to be resolved. In three previous studies of ptenA cell behavior [29], [30], [32], similar defects in velocity were described, but there was a lack of consensus on the capacity of mutant cells to assess a spatial gradient of cAMP generated in vitro. In all three studies, data were provided for cells that were induced to acquire chemotactic competence by a similar method of pulsing with cAMP [80], [81] (Table 1), rather than incubating them on pads saturated with buffer, as performed for the experiments reported here (Table 1). All three studies employed buffers in the in vitro chemotaxis assays (Table 1) that contained concentrations of cations that facilitated cAMP chemotaxis [48], [51], [59], [77]. However, the studies differed in the concentration range of the cAMP gradients used. Iijima and Devreotes [29] analyzed responsiveness in a gradient of cAMP generated by releasing 1µM cAMP from a micropipette (low cAMP concentration gradient). They observed that ptenA cells exhibited reduced velocity and a loss of chemotactic orientation (Table 1). Wessels et al. [30] analyzed chemotactic responsiveness in a gradient generated in a chamber [61], [63], in which the source well was filled with 1 µM cAMP (low cAMP concentration gradient). They observed a 40% reduction in velocity and a 60% reduction in the chemotactic index (Table 1). The gradients in these two studies were estimated, using the methods of Postma and Van Haastert [82], to be approximately 0.5 and 0.4 nM per µm and in the concentration range of the gradient estimated for the front of a natural wave in an aggregation territory (i.e., 1 µM at the peak of each wave and less than 0.01 µM at the trough) [44]. In contrast, Hoeller and Kay [32] analyzed responsiveness in a cAMP gradient generated by releasing 10 µM cAMP from a micropipette. The gradient generated was estimated to be approximately 5 nM per µm, steeper and in a concentration range 10 times higher than gradients tested by Iijima and Deveotes [29] and Wessels et al., [30]. Hoeller and Kay [32] observed no difference in chemotactic efficiency between Ax2 and ptenA cells, but did report a defect in velocity.

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Table 1. Chemotactic behavior of ptenA cells pulsed with cAMP to achieve chemotactic competence: a comparison of four different studies involving either “low cAMP concentrations” in the estimated range for natural cAMP waves or “high cAMP concentration gradients”, at concentrations 10 times that of natural cAMP waves.

http://dx.doi.org/10.1371/journal.pone.0108495.t001

These results suggested to us the possibility that pulsing ptenA cells with cAMP might up-regulate expression of lpten to a level that provides them with the capacity to assess the gradient in the high cAMP concentration range, but not the gradient in the low cAMP concentration range. To explore this hypothesis, we analyzed the behavior of cAMP-pulsed parental cells and cells of the ptenA strain of Hoeller and Kay [32], in gradients generated in a gradient chamber [58], [61], [63]. Behavior was analyzed in low cAMP concentration gradient, in which the source well contained 1 µM cAMP (Figures 7A and B) and in a high cAMP concentration gradient, in which the source well contained 10 µM cAMP (Figures 7C, D).

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Figure 7. ptenA cells pulsed in suspension with cAMP to induce chemotactic competence are defective in assessing the direction of a low cAMP concentration gradient in the range of a natural wave, but they can efficiently assess the direction of a cAMP gradient in a concentration range 10 times higher.

Pulsing ptenA cells with cAMP also up-regulates lpten. A, B. 2D-DIAS reconstructions of perimeter tracks of Ax2 and ptenA cells, respectively, in a low cAMP concentration gradient, generated by adding 1 µM cAMP to the source well of the gradient chamber. Motility and chemotaxis parameters assessed by 2D-DIAS software are presented in the lower left hand corner of each panel. C, D. Perimeter tracks of representative Ax2 and ptenA cells, respectively, in a high cAMP concentration gradient, generated by adding 10 µM cAMP to the source well of the gradient chamber. Motility and chemotaxis parameters are displayed in the lower left corner of each panel. E, F. Up-regulation of lpten expression in cAMP pulsed Ax2 and ptenA cells, respectively. In each strain, cells were analyzed by RT-PCR using primers P1 and P2 (Table S1), prior to cAMP pulsing (1 hr), after cAMP pulsing for six hours (6 hr) and after cAMP pulsing with buffer for six hours (6 h). The constitutively expressed large subunit ribosomal RNA (rnlA) was assessed for comparability (see Figure 1 and 4). No RT, no reverse transcriptase added; IV, instantaneous velocity; CI, chemotactic index; %+, percent cells with a positive CI; N, number of cells assessed. Parameters in panels A, B, C and D are defined in Table S2.

http://dx.doi.org/10.1371/journal.pone.0108495.g007

In the low cAMP concentration gradient, cAMP-pulsed parental Ax2 cells underwent chemotaxis with high velocities and high chemotactic indices (Figure 7A). And as previously reported [29], [30] and shown here in Figure 5, both the instantaneous velocity and the CI of ptenA cells were dramatically reduced (Figure 7B). In a high concentration gradient, cAMP-pulsed parental Ax2 cells underwent chemotaxis, but velocity was reduced by 25% and chemotactic efficiency (C.I.) by 35% (Figure 3C), reductions similar to those previously reported by us using the same conditions thirty years ago [63]. However, in a high cAMP concentration gradient, ptenA cells moved with a chemotactic index similar to that of Ax2 cell in a low concentration gradient, with slightly reduced velocity, as previously reported by Hoeller and Kay [32].

To test whether cAMP pulsing caused an increase in lpten expression in ptenA cells, the level of the lpten transcript was compared between Ax2 and ptenA cells by RT-PCR prior to pulsing (1 h), after six hours of pulsing with cAMP and after 6 hours of pulsing with buffer alone. Both in Ax2 cells (Figure 7E) and ptenA cells (Figure 7F), cAMP pulsing up-regulated lpten expression at least 5 fold over that of the initial vegetative cell preparation (0 h). Pulsing ptenA cells with buffer alone also up-regulated lpten expression, but to a lesser degree than pulsing with cAMP (Figure 7E, F). These results demonstrate that pulsing with cAMP up-regulates lpten expression, and, by correlation, may explain why cAMP-pulsed ptenA cells can undergo chemotaxis in a high cAMP concentration gradient. The increased levels of expression of lpten in cAMP-pulsed Ax2 and ptenA cells were still several fold lower than the levels attained in strain ptenA/lptenoe cells developed on pads (data not shown). This may explain why pulsing does not rescue the chemotaxis defect in a low cAMP concentration gradient.

Discussion

Mutations in the human PTEN gene are the most common of the tumor suppressor genes associated with human cancer [2], [3], [12], [83]. Interestingly there are two additional PTEN homologs, TPTE and TPIPlocated on different chromosomes, and a secreted PTEN [12], [13], [15][18], as well as a pseudogene of PTEN, PTENP1 [17]. However, there have been, to our knowledge, no reported studies to test whether any of the human PTEN homologs, when overexpressed, can rescue the behavioral defects caused by a human mutant PTEN cell, a question relevant to cancers that involve this mutation.

Here, we report for the first time that D. discoideum contains not only the human PTEN ortholog ptenA, as previously demonstrated [28], [29], but also a second ortholog, lpten. Both PtenA and Lpten contain the two conserved domains of human PTEN, the dual-specificity phosphatase domain and PTEN-C2, the lipid-C2-binding domain. In addition, Lpten contains five LIM domains, which presumably play a role in protein-protein interactions [84], [85]. Both ptenA and lpten are up-regulated in the period of the D.discoideum developmental program following the onset of starvation and preceding aggregation. Deletion of ptenA causes major defects in chemotaxis and development [29], [30], [32]. The ptenA cells cannot undergo natural chemotaxis, aggregation or morphogenesis. However, deletion of lpten does not block aggregation or development, and does not decrease the efficiency of chemotaxis in a gradient of cAMP generated in vitro in the concentration range of the cAMP gradient in the front of the naturally relayed cAMP wave. Deletion of lpten does, however, affect the suppression of lateral pseudopod formation, which is also the case for the ptenA mutant. The mutant phenotype of lpten, therefore, exhibits a weak phenocopy of ptenA.

Here we have considered the possibility that there may exist at least parallel functions, or partial redundancy of Pten and Lpten. This has led us to test whether overexpressing lpten in a ptenA mutant might rescue the defects of the ptenA mutant. We therefore placed the coding region of lpten under the control of the strong actin 15 promoter in a plasmid and introduced it into the ptenA mutant to create ptenA/lptenoe. Aggregation-competent cells of ptenA/lptenoe expressed the lpten transcript at over 10 times the level observed in wild type or ptenA cells, and close to two orders of magnitude higher than in vegetative cells. We found that overexpression rescued every developmental, cell motility and chemotaxis defect exhibited by mutant ptenA cells [30]. The rescued ptenA defects included the following: 1) a prolonged preaggregative period; 2) abnormal or no aggregation in submerged cultures or on a filter pad substrate; 3) lack of a multicellular developmental program, including lack of fruiting body formation; 4) decreased velocity during basic motile behavior in buffer alone, or during chemotaxis in a shallow gradient of cAMP generated in the concentration range estimated for the front of a natural wave [44] 5) an increased frequency of lateral pseudopod formation and turning; 6) a dramatic decrease in chemotactic efficiency in a low cAMP concentration gradient, in the estimated range for the front of the natural wave; and 7) a dramatic decrease in orientation in the front of relayed cAMP waves in a natural aggregation territory. The complete rescue of the ptenA mutant phenotype by overexpression of the homolog lpten, raises the possibility that overexpressing a human PTEN homolog might suppress the behavioral defects of a mutant PTEN thus suppressing tumorigenesis.

Supporting Information

Table S1.

Primers used in this study.

doi:10.1371/journal.pone.0108495.s001

(PDF)

Table S2.

2D-DIAS parameters.

doi:10.1371/journal.pone.0108495.s002

(PDF)

Acknowledgments

This work was supported by the Monoclonal Antibody Research Institute and the Developmental Studies Hybridoma Bank, the latter a National Resource created by NIH and housed at the University of Iowa.

Author Contributions

Conceived and designed the experiments: DRS DFL. Performed the experiments: DFL NAR KBR BMH BAS BHL. Analyzed the data: DRS DFL DW. Contributed to the writing of the manuscript: DRS DFL DW.

References

  1. 1. Hollander MC, Blumenthal GM, Dennis PA (2011) PTEN loss in the continuum of common cancers, rare syndromes and mouse models. Nat Rev Cancer 11: 289–301. doi: 10.1038/nrc3037
  2. 2. Li J, Yen C, Liaw D, Podsypanina K, Bose S, et al. (1997) PTEN, a putative protein tyrosine phosphatase gene mutated in human brain, breast, and prostate cancer. Science 275: 1943–1947. doi: 10.1126/science.275.5308.1943
  3. 3. Steck PA, Pershouse MA, Jasser SA, Yung WK, Lin H, et al. (1997) Identification of a candidate tumour suppressor gene, MMAC1, at chromosome 10q23.3 that is mutated in multiple advanced cancers. Nat Genet 15: 356–362. doi: 10.1038/ng0497-356
  4. 4. Vitolo MI, Weiss MB, Szmacinski M, Tahir K, Waldman T, et al. (2009) Deletion of PTEN promotes tumorigenic signaling, resistance to anoikis, and altered response to chemotherapeutic agents in human mammary epithelial cells. Cancer Res 69: 8275–8283. doi: 10.1158/0008-5472.can-09-1067
  5. 5. Tamura M, Gu J, Matsumoto K, Aota S, Parsons R, et al. (1998) Inhibition of cell migration, spreading, and focal adhesions by tumor suppressor PTEN. Science 280: 1614–1617. doi: 10.1126/science.280.5369.1614
  6. 6. Davidson L, Maccario H, Perera NM, Yang X, Spinelli L, et al. (2010) Suppression of cellular proliferation and invasion by the concerted lipid and protein phosphatase activities of PTEN. Oncogene 29: 687–697. doi: 10.1038/onc.2009.384
  7. 7. Heering J, Erlmann P, Olayioye MA (2009) Simultaneous loss of the DLC1 and PTEN tumor suppressors enhances breast cancer cell migration. Exp Cell Res 315: 2505–2514. doi: 10.1016/j.yexcr.2009.05.022
  8. 8. Tibarewal P, Zilidis G, Spinelli L, Schurch N, Maccario H, et al. (2012) PTEN protein phosphatase activity correlates with control of gene expression and invasion, a tumor-suppressing phenotype, but not with AKT activity. Sci Signal 5: ra18. doi: 10.1126/scisignal.2002138
  9. 9. Liliental J, Moon SY, Lesche R, Mamillapalli R, Li D, et al. (2000) Genetic deletion of the PTEN tumor suppressor gene promotes cell motility by activation of Rac1 and Cdc42 GTPases. Curr Biol 10: 401–404. doi: 10.1016/s0960-9822(00)00417-6
  10. 10. Raftopoulou M, Etienne-Manneville S, Self A, Nicholls S, Hall A (2004) Regulation of cell migration by the C2 domain of the tumor suppressor PTEN. Science 303: 1179–1181. doi: 10.1126/science.1092089
  11. 11. Maehama T, Dixon JE (1998) The tumor suppressor, PTEN/MMAC1, dephosphorylates the lipid second messenger, phosphatidylinositol 3,4,5–trisphosphate. J Biol Chem 273: 13375–13378. doi: 10.1074/jbc.273.22.13375
  12. 12. Chen H, Rossier C, Morris MA, Scott HS, Gos A, et al. (1999) A testis-specific gene, TPTE, encodes a putative transmembrane tyrosine phosphatase and maps to the pericentromeric region of human chromosomes 21 and 13, and to chromosomes 15, 22, and Y. Hum Genet. 105: 399–409. doi: 10.1007/s004390051122
  13. 13. Kim YJ, Jahan N, Bahk YY (2013) Biochemistry and structure of phosphoinositide phosphatases. BMB Rep 46: 1–8. doi: 10.5483/bmbrep.2013.46.1.261
  14. 14. Tapparel C, Reymond A, Girardet C, Guillou L, Lyle R, et al. (2003) The TPTE gene family: cellular expression, subcellular localization and alternative splicing. Gene 323: 189–199. doi: 10.1016/j.gene.2003.09.038
  15. 15. Walker SM, Downes CP, Leslie NR (2001) TPIP: a novel phosphoinositide 3-phosphatase. Biochem J 360: 277–283. doi: 10.1042/0264-6021:3600277
  16. 16. Hopkins BD, Fine B, Steinbach N, Dendy M, Rapp Z, et al. (2013) A secreted PTEN phosphatase that enters cells to alter signaling and survival. Science 341: 399–402. doi: 10.1126/science.1234907
  17. 17. Poliseno L, Salmena L, Zhang J, Carver B, Haveman WJ, et al. (2010) A coding-independent function of gene and pseudogene mRNAs regulates tumour biology. Nature 465: 1033–1038. doi: 10.1038/nature09144
  18. 18. Johnsson P, Ackley A, Vidarsdottir L, Lui WO, Corcoran M, et al. (2013) A pseudogene long-noncoding-RNA network regulates PTEN transcription and translation in human cells. Nat Struct Mol Biol 20: 440–446. doi: 10.1038/nsmb.2516
  19. 19. Artemenko Y, Lampert TJ, Devreotes PN (2014) Moving towards a paradigm: common mechanisms of chemotactic signaling in Dictyostelium and mammalian leukocytes. Cell Mol Life Sci.
  20. 20. Soll DR, Wessels D, Kuhl S, Lusche DF (2009) How a cell crawls and the role of cortical Myosin II. Eukaryot Cell 8: 1381–1396. doi: 10.1128/ec.00121-09
  21. 21. Soll DR, Wessels D, Lusche DF, Kuhl S, Scherer A, et al. (2011) Role of extracellular cations in cell motility, polarity, and chemotaxis. Research and Reports in Biology 2: 69–88. doi: 10.2147/rrb.s13701
  22. 22. Williams RS, Boeckeler K, Graf R, Muller-Taubenberger A, Li Z, et al. (2006) Towards a molecular understanding of human diseases using Dictyostelium discoideum. Trends Mol Med 12: 415–424. doi: 10.1016/j.molmed.2006.07.003
  23. 23. Ludtmann MH, Boeckeler K, Williams RS (2011) Molecular pharmacology in a simple model system: implicating MAP kinase and phosphoinositide signalling in bipolar disorder. Semin Cell Dev Biol 22: 105–113. doi: 10.1016/j.semcdb.2010.11.002
  24. 24. Annesley SJ, Fisher PR (2009) Dictyostelium discoideum – a model for many reasons. Mol Cell Biochem 329: 73–91. doi: 10.1007/s11010-009-0111-8
  25. 25. Escalante R (2011) Dictyostelium as a model for human disease. Semin Cell Dev Biol 22: 69. doi: 10.1016/j.semcdb.2010.12.001
  26. 26. Carnell MJ, Insall RH (2011) Actin on disease – studying the pathobiology of cell motility using Dictyostelium discoideum.. Semin Cell Dev Biol 22: 82–88. doi: 10.1016/j.semcdb.2010.12.003
  27. 27. Nikolaeva I, Huber RJ, O'Day DH (2012) EGF-like peptide of Dictyostelium discoideum is not a chemoattractant but it does restore folate-mediated chemotaxis in the presence of signal transduction inhibitors. Peptides 34: 145–149. doi: 10.1016/j.peptides.2011.12.014
  28. 28. Funamoto S, Meili R, Lee S, Parry L, Firtel RA (2002) Spatial and temporal regulation of 3-phosphoinositides by PI 3-kinase and PTEN mediates chemotaxis. Cell 109: 611–623. doi: 10.1016/s0092-8674(02)00755-9
  29. 29. Iijima M, Devreotes P (2002) Tumor suppressor PTEN mediates sensing of chemoattractant gradients. Cell 109: 599–610. doi: 10.1016/s0092-8674(02)00745-6
  30. 30. Wessels D, Lusche DF, Kuhl S, Heid P, Soll DR (2007) PTEN plays a role in the suppression of lateral pseudopod formation during Dictyostelium motility and chemotaxis. J Cell Sci 120: 2517–2531. doi: 10.1242/jcs.010876
  31. 31. Pramanik MK, Iijima M, Iwadate Y, Yumura S (2009) PTEN is a mechanosensing signal transducer for myosin II localization in Dictyostelium cells. Genes Cells 14: 821–834. doi: 10.1111/j.1365-2443.2009.01312.x
  32. 32. Hoeller O, Kay RR (2007) Chemotaxis in the absence of PIP3 gradients. Curr Biol 17: 813–817. doi: 10.1016/j.cub.2007.04.004
  33. 33. King JS, Teo R, Ryves J, Reddy JV, Peters O, et al. (2009) The mood stabiliser lithium suppresses PIP3 signalling in Dictyostelium and human cells. Dis Model Mech 2: 306–312. doi: 10.1242/dmm.001271
  34. 34. Kortholt A, King JS, Keizer-Gunnink I, Harwood AJ, Van Haastert PJ (2007) Phospholipase C regulation of phosphatidylinositol 3,4,5-trisphosphate-mediated chemotaxis. Mol Biol Cell 18: 4772–4779. doi: 10.1091/mbc.e07-05-0407
  35. 35. Iijima M, Huang YE, Luo HR, Vazquez F, Devreotes PN (2004) Novel mechanism of PTEN regulation by its phosphatidylinositol 4,5-bisphosphate binding motif is critical for chemotaxis. J Biol Chem 279: 16606–16613. doi: 10.1074/jbc.m312098200
  36. 36. Huang YE, Iijima M, Parent CA, Funamoto S, Firtel RA, et al. (2003) Receptor-mediated regulation of PI3Ks confines PI(3,4,5)P3 to the leading edge of chemotaxing cells. Mol Biol Cell 14: 1913–1922. doi: 10.1091/mbc.e02-10-0703
  37. 37. Arai Y, Shibata T, Matsuoka S, Sato MJ, Yanagida T, et al. (2010) Self-organization of the phosphatidylinositol lipids signaling system for random cell migration. Proc Natl Acad Sci U S A 107: 12399–12404. doi: 10.1073/pnas.0908278107
  38. 38. Taniguchi D, Ishihara S, Oonuki T, Honda-Kitahara M, Kaneko K, et al. (2013) Phase geometries of two-dimensional excitable waves govern self-organized morphodynamics of amoeboid cells. Proc Natl Acad Sci U S A 110: 5016–5021. doi: 10.1073/pnas.1218025110
  39. 39. Gerisch G, Ecke M, Wischnewski D, Schroth-Diez B (2011) Different modes of state transitions determine pattern in the Phosphatidylinositide-Actin system. BMC Cell Biol 12: 42. doi: 10.1186/1471-2121-12-42
  40. 40. Maeda YT, Inose J, Matsuo MY, Iwaya S, Sano M (2008) Ordered patterns of cell shape and orientational correlation during spontaneous cell migration. PLoS One 3: e3734. doi: 10.1371/journal.pone.0003734
  41. 41. Gerisch G, Schroth-Diez B, Muller-Taubenberger A, Ecke M (2012) PIP3 waves and PTEN dynamics in the emergence of cell polarity. Biophys J 103: 1170–1178. doi: 10.1016/j.bpj.2012.08.004
  42. 42. Sasaki AT, Janetopoulos C, Lee S, Charest PG, Takeda K, et al. (2007) G protein-independent Ras/PI3K/F-actin circuit regulates basic cell motility. J Cell Biol 178: 185–191. doi: 10.1083/jcb.200611138
  43. 43. Chen L, Janetopoulos C, Huang YE, Iijima M, Borleis J, et al. (2003) Two phases of actin polymerization display different dependencies on PI(3,4,5)P3 accumulation and have unique roles during chemotaxis. Mol Biol Cell 14: 5028–5037. doi: 10.1091/mbc.e03-05-0339
  44. 44. Tomchik KJ, Devreotes PN (1981) Adenosine 3′,5′-monophosphate waves in Dictyostelium discoideum: a demonstration by isotope dilution – fluorography. Science 212: 443–446. doi: 10.1126/science.6259734
  45. 45. Bloomfield G, Tanaka Y, Skelton J, Ivens A, Kay RR (2008) Widespread duplications in the genomes of laboratory stocks of Dictyostelium discoideum.. Genome Biol 9: R75. doi: 10.1186/gb-2008-9-4-r75
  46. 46. Yarger J, Stults K, Soll DR (1974) Observations on the growth of Dictyostelium discoideum in axenic medium: evidence for an extracellular growth inhibitor synthesized by stationary phase cells. J Cell Sci 14: 681–690.
  47. 47. Cocucci SM, Sussman M (1970) RNA in cytoplasmic and nuclear fractions of cellular slime mold amebas. J Cell Biol 45: 399–407. doi: 10.1083/jcb.45.2.399
  48. 48. Lusche DF, Wessels D, Scherer A, Daniels K, Kuhl S, et al. (2012) The IplA Ca2+ channel of Dictyostelium discoideum is necessary for chemotaxis mediated through Ca2+, but not through cAMP, and has a fundamental role in natural aggregation. J Cell Sci 125: 1770–1783. doi: 10.1242/jcs.098301
  49. 49. Sussman M (1987) Cultivation and synchronous morphogenesis of Dictyostelium under controlled experimental conditions. Methods Cell Biol 28: 9–29. doi: 10.1016/s0091-679x(08)61635-0
  50. 50. Soll DR (1979) Timers in developing systems. Science 203: 841–849. doi: 10.1126/science.419408
  51. 51. Wessels D, Lusche DF, Steimle PA, Scherer A, Kuhl S, et al. (2012) Myosin heavy chain kinases play essential roles in Ca2+, but not cAMP, chemotaxis and the natural aggregation of Dictyostelium discoideum. J Cell Sci 125: 4934–4944. doi: 10.1242/jcs.112474
  52. 52. Torija P, Robles A, Escalante R (2006) Optimization of a large-scale gene disruption protocol in Dictyostelium and analysis of conserved genes of unknown function. BMC Microbiol 6: 75.
  53. 53. Abe T, Langenick J, Williams JG (2003) Rapid generation of gene disruption constructs by in vitro transposition and identification of a Dictyostelium protein kinase that regulates its rate of growth and development. Nucleic Acids Res 31: e107. doi: 10.1093/nar/gng095
  54. 54. Veltman DM, Akar G, Bosgraaf L, Van Haastert PJ (2009) A new set of small, extrachromosomal expression vectors for Dictyostelium discoideum. Plasmid 61: 110–118. doi: 10.1016/j.plasmid.2008.11.003
  55. 55. Srikantha T, Daniels KJ, Pujol C, Kim E, Soll DR (2013) Identification of genes upregulated by the transcription factor Bcr1 that are involved in impermeability, impenetrability, and drug resistance of Candida albicans a/alpha biofilms. Eukaryot Cell 12: 875–888. doi: 10.1128/ec.00071-13
  56. 56. Soll DR, Wessels D, Voss E, Johnson O (2001) Computer-assisted systems for the analysis of amoeboid cell motility. Methods Mol Biol 161: 45–58. doi: 10.1385/1-59259-051-9:045
  57. 57. Varnum B, Edwards KB, Soll DR (1986) The developmental regulation of single-cell motility in Dictyostelium discoideum. Dev Biol 113: 218–227. doi: 10.1016/0012-1606(86)90124-7
  58. 58. Wessels D, Kuhl S, Soll DR (2009) 2D and 3D quantitative analysis of cell motility and cytoskeletal dynamics. Methods Mol Biol 586: 315–335. doi: 10.1007/978-1-60761-376-3_18
  59. 59. Lusche DF, Wessels D, Soll DR (2009) The effects of extracellular calcium on motility, pseudopod and uropod formation, chemotaxis, and the cortical localization of myosin II in Dictyostelium discoideum.. Cell Motil Cytoskeleton 66: 567–587. doi: 10.1002/cm.20367
  60. 60. Zigmond SH, Hirsch JG (1973) Leukocyte locomotion and chemotaxis. New methods for evaluation, and demonstration of a cell-derived chemotactic factor. J Exp Med 137: 387–410. doi: 10.1084/jem.137.2.387
  61. 61. Zigmond SH (1977) Ability of polymorphonuclear leukocytes to orient in gradients of chemotactic factors. J Cell Biol 75: 606–616. doi: 10.1083/jcb.75.2.606
  62. 62. Zigmond S (1973) Leucocyte locomotion and chemotaxis. Nouv Rev Fr Hematol 13: 886–887.
  63. 63. Varnum B, Soll DR (1984) Effects of cAMP on single cell motility in Dictyostelium. J Cell Biol 99: 1151–1155. doi: 10.1083/jcb.99.3.1151
  64. 64. Soll DR, Voss E (1998) Two and three dimensional computer systems for analyzing how cells crawl. In: Soll DR, Wessels D, editors. Motion Analysis of Living Cells: John Wiley, Inc. 25–52.
  65. 65. Soll DR (1995) The use of computers in understanding how animal cells crawl. Int Rev Cytol 163: 43–104. doi: 10.1016/s0074-7696(08)62209-3
  66. 66. Zhang H, Heid PJ, Wessels D, Daniels KJ, Pham T, et al. (2003) Constitutively active protein kinase A disrupts motility and chemotaxis in Dictyostelium discoideum. Eukaryot Cell 2: 62–75. doi: 10.1128/ec.2.1.62-75.2003
  67. 67. Wessels D, Srikantha T, Yi S, Kuhl S, Aravind L, et al. (2006) The Shwachman-Bodian-Diamond syndrome gene encodes an RNA-binding protein that localizes to the pseudopod of Dictyostelium amoebae during chemotaxis. J Cell Sci 119: 370–379. doi: 10.1242/jcs.02753
  68. 68. Wessels D, Voss E, Von Bergen N, Burns R, Stites J, et al. (1998) A computer-assisted system for reconstructing and interpreting the dynamic three-dimensional relationships of the outer surface, nucleus and pseudopods of crawling cells. Cell Motil Cytoskeleton 41: 225–246. doi: 10.1002/(sici)1097-0169(1998)41:3<225::aid-cm4>3.3.co;2-9
  69. 69. Wessels D, Kuhl S, Soll DR (2006) Application of 2D and 3D DIAS to motion analysis of live cells in transmission and confocal microscopy imaging. Methods in molecular biology (Clifton, NJ) 346: 261–279. doi: 10.1385/1-59745-144-4:261
  70. 70. Heid PJ, Geiger J, Wessels D, Voss E, Soll DR (2005) Computer-assisted analysis of filopod formation and the role of myosin II heavy chain phosphorylation in Dictyostelium. Journal of cell science 118: 2225–2237. doi: 10.1242/jcs.02342
  71. 71. Escalante R, Wessels D, Soll DR, Loomis WF (1997) Chemotaxis to cAMP and slug migration in Dictyostelium both depend on migA, a BTB protein. Mol Biol Cell 8: 1763–1775. doi: 10.1091/mbc.8.9.1763
  72. 72. Wessels D, Reynolds J, Johnson O, Voss E, Burns R, et al. (2000) Clathrin plays a novel role in the regulation of cell polarity, pseudopod formation, uropod stability and motility in Dictyostelium. J Cell Sci 113 (Pt 1): 21–36.
  73. 73. Doi K, Gartner A, Ammerer G, Errede B, Shinkawa H, et al. (1994) MSG5, a novel protein phosphatase promotes adaptation to pheromone response in S. cerevisiae.. EMBO J 13: 61–70.
  74. 74. Lee JO, Yang H, Georgescu MM, Di Cristofano A, Maehama T, et al. (1999) Crystal structure of the PTEN tumor suppressor: implications for its phosphoinositide phosphatase activity and membrane association. Cell 99: 323–334. doi: 10.1016/s0092-8674(00)81663-3
  75. 75. Rot G, Parikh A, Curk T, Kuspa A, Shaulsky G, et al. (2009) dictyExpress: a Dictyostelium discoideum gene expression database with an explorative data analysis web-based interface. BMC Bioinformatics 10: 265. doi: 10.1186/1471-2105-10-265
  76. 76. Parikh A, Huang E, Dinh C, Zupan B, Kuspa A, et al. (2010) New components of the Dictyostelium PKA pathway revealed by Bayesian analysis of expression data. BMC Bioinformatics 11: 163. doi: 10.1186/1471-2105-11-163
  77. 77. Lusche DF, Wessels D, Ryerson DE, Soll DR (2011) Nhe1 is essential for potassium but not calcium facilitation of cell motility and the monovalent cation requirement for chemotactic orientation in Dictyostelium discoideum.. Eukaryot Cell 10: 320–331. doi: 10.1128/ec.00255-10
  78. 78. Wessels D, Vawter-Hugart H, Murray J, Soll DR (1994) Three-dimensional dynamics of pseudopod formation and the regulation of turning during the motility cycle of Dictyostelium. Cell Motil Cytoskeleton 27: 1–12. doi: 10.1002/cm.970270102
  79. 79. Fischer M, Haase I, Simmeth E, Gerisch G, Muller-Taubenberger A (2004) A brilliant monomeric red fluorescent protein to visualize cytoskeleton dynamics in Dictyostelium.. FEBS Lett 577: 227–232. doi: 10.1016/j.febslet.2004.09.084
  80. 80. Robertson A, Drage DJ, Cohen MH (1972) Control of Aggregation in Dictyostelium discoideum by an External Periodic Pulse of Cyclic Adenosine Monophosphate. Science 175: 333–335. doi: 10.1126/science.175.4019.333
  81. 81. Gerisch G, Fromm H, Huesgen A, Wick U (1975) Control of cell-contact sites by cyclic AMP pulses in differentiating Dictyostelium cells. Nature 255: 547–549. doi: 10.1038/255547a0
  82. 82. Postma M, van Haastert PJ (2009) Mathematics of experimentally generated chemoattractant gradients. Methods Mol Biol 571: 473–488. doi: 10.1007/978-1-60761-198-1_31
  83. 83. Govender D, Chetty R (2012) Gene of the month: PTEN. J Clin Pathol 65: 601–603. doi: 10.1136/jclinpath-2012-200711
  84. 84. Koch BJ, Ryan JF, Baxevanis AD (2012) The diversification of the LIM superclass at the base of the metazoa increased subcellular complexity and promoted multicellular specialization. PLoS One 7: e33261. doi: 10.1371/journal.pone.0033261
  85. 85. Brown S, Coghill ID, McGrath MJ, Robinson PA (2001) Role of LIM domains in mediating signaling protein interactions. IUBMB Life 51: 359–364. doi: 10.1080/152165401753366113