taxonID	type	description	language	source
E82F87CABE5BFFD10EB4F535FCA3B1AF.taxon	description	Anatomy A few specimens from the aforementioned collections were selected for anatomical analysis. Shells were inspected visually with the assistance of a Leica M 205 C stereomicroscope equipped with a Leica MC 170 HD digital camera at the Centro para Documentação da Biodiversidade (FFCLRP-USP, Ribeirão Preto, Brazil). Shell measurements were taken using callipers and LEICA APPLICATION SUITE X 4.12 sofware. Other anatomical structures were examined on ethanol-preserved specimens using stereomicroscopes, scanning electron microscopy, and computed tomography (CT), following the methods outlined below. Anatomical structures were identified and described following previous descriptions of Drymaeus species (e. g. Breure 1979, Breure and Eskens 1981, Simone and Amaral 2018, Simone et al. 2020). Te anatomical nomenclature used herein aligns with Simone and Amaral (2018) and Simone et al. (2020). Abbreviations: aa, anterior aorta; ac, albumen chamber; ag, albumen gland; an, anus; au, auricle; bc, bursa copulatrix; bd, bursa copulatrix duct; bm, buccal mass; ce, cerebral ganglion; cs, circulatory system; cv, pulmonary (efferent) vein; da, digestive gland anterior lobe; dd, duct to digestive gland; df, dorsal folds of buccal mass; dg, digestive gland posterior lobe; ds, digestive system; eh, epiphallus; es, oesophagus; fo, free oviduct; fp, genital pore; F, foot; go, gonad; hd, hermaphrodite duct; in, intestine; jw, jaw; ki, kidney; mb, mantle edge; mo, mouth; ne, nephrostome; ns, central nervous system; oc, odontophore cartilage; om, ommatophore; pe, penis; pm, penis muscle; pn, pneumostome; pp, pedal ganglion; ps, penis sheath; pt, prostate; pu, pulmonary cavity; pv, pneumostome right flap; ra, radula; rc, renopericardial canal; re, reproductive system; rn, radular nucleus; rt, rectum; sd, salivary duct; sr, seminal receptacle; st, stomach; ut, uterus; ve, ventricle; vg, vagina; vm, visceral mass. Computed tomography Specimens preserved in 70 % ethanol were immersed individually in 30 mL of a contrasting solution consisting of 1 % phosphotungstic acid and 1 % dimethyl sulphoxide diluted in 70 % ethanol for 7 – 15 days to enhance the contrast of sof tissues. CT scanning was conducted at the Centro para Documentação da Biodiversidade using a Phoenix v | tome | x S 240 Industrial High-Resolution CT & X-Ray System (General Electric, USA). Tis system is equipped with a digital high-contrast detector DXR 250 RT and a 180 kV high-power nanofocus source. High-resolution X-ray computed tomographies were captured with the following setings: source at 70 kV and 200 µA, 1000 projections, binning of 1 × 1, averaging three frames with one frame skipped, exposure time of 333.09 ms, default offset and gain correction, and no filter applied. Te resulting 16 - bit greyscale images measured 990 × 1000 pixels. Tree-dimensional (3 D) reconstructions were processed using GE Phoenix Datos X 2 sofware, and visualization and editing of the 3 D models were performed with VGStudio Max ® 3.0 (Volume Graphics, Germany). To reconstruct specific organs and structures in 3 D, CT images were segmented manually using AMIRA 5.3.2 (Visage Imaging Inc.). Interpolation was applied across intervals of up to five slices to optimize processing time. Afer segmentation, models were saved and exported in. stl format for further visualization in various sofware platforms, including VGStudio Max ® 3.0. Te final 3 D models are available at MorphoMuseuM (Rosa et al. 2025). Scanning electron microscopy Scanning electron microscopy was used to aid in the visualization and characterization of radular morphology. Te radula was extracted using standard dissection methods and coated with gold using a Quorum Q 150 R ES sputer coater at the Centro para Documentação da Biodiversidade. Imaging was conducted with a JEOL JSM- 6610 LV scanning electron microscope at the Laboratório Multiusuário de Microscopia Eletrônica (FMRP-USP, Ribeirão Preto, Brazil). DNA extraction and sequencing Tissue clips were obtained from selected specimens of D. magus and other potentially related species for DNA extraction (Table 1). Four specimens of D. magus from different localities were used, representing two conchological morphotypes. DNA extraction was done using the QIAGEN DNEasy ® Blood & Tissue Kit mostly following the manufacturer’s standard protocol, but modifying the final step to increase yield: one-quarter of the suggested amount of buffer AE was used, and a repetition of the step was added. Te combination of genetic markers used in this study was the same as in the studies by Breure and Romero (2012) and Salvador et al. (2023), to allow the inclusion of our data in their phylogenetic framework of the subfamily Peltellinae. Te markers (and primers) used were as follows: the barcoding fragment of the mitochondrial COI gene (Folmer et al. 1994; primers LCO / HCO); a fragment of the nuclear H 3 (histone 3) gene (Uit de Weerd and Gitenberger 2013; primers H 3 pulF / H 3 pul 3); and a fragment of nuclear DNA including the 3 ′ end of the 5.8 S rRNA gene, the ITS 2 region, and the 5 ′ end of the 28 S rRNA gene (Wade and Mordan 2000, Wade et al. 2006; amplified in two parts using the primer pairs LSU- 1 / LSU- 3 and LSU- 2 / LSU- 5). Te PCR amplification protocols were the same as those used by Salvador et al. (2023), starting with initial denaturation at 95 ° C (3 min), then having specific cycles as follows: for COI, 35 cycles of denaturation at 95 ° C (30 s), annealing at 48 ° C (1 min), and extension at 72 ° C (2 min); for H 3, 40 cycles of denaturation at 95 ° C (30 s), annealing at 57 ° C (30 s), and extension at 72 ° C (40 s); and for ITS 2 + 28 S, 40 cycles of denaturation at 95 ° C (30 s), annealing at either 50 ° C (ITS 2 section) or 45 ° C (28 S section) (1 min), and extension at 72 ° C for either 5 min (ITS 2 section) or 2 min (28 S section). Te PCR ended with a final extension at 72 ° C (5 min) for all markers. Te success of amplification was assessed visually via agarose gel electrophoresis. Te successful PCR products were then cleaned with ExoSAP-IT ™ (Affymetrix Inc.) following the manufacturer’s standard protocol. Samples were then prepared for sequencing and sent to Macrogen Europe (Amsterdam, Te Netherlands) for Sanger sequencing. Te resulting sequences were quality checked and de novo assembled in GENEIOUS PRIME (v. 2023.2.1, Biomaters Ltd.). Te consensus sequences were extracted and uploaded to GenBank (for accession numbers, see Table 1). Phylogenetic analysis We have included our new samples in the phylogenetic framework recently published by Salvador et al. (2023). To that end, we used their entire dataset of subfamily Peltellinae, using one Bulimulinae and one Strophocheilidae as outgroups. Te taxa used in the phylogenetic analysis, alongside their GenBank accession numbers and locality data, can be found in Table 1. Te alignment of genetic sequences of each marker was done in GENEIOUS PRIME using the MAFFT plugin (Katoh et al. 2002, Katoh and Standley 2013) with the default setings. Te resulting alignment of each marker was proofed visually for inconsistencies. Alignment of the ITS / 28 S marker was run through GBLOCKS (Castresana 2000, Talavera and Castresana 2007) to eliminate poorly aligned or data-deficient positions that could impact the analysis. Te alignments were then concatenated, resulting in a total of 2033 bp (COI = 654 bp, H 3 = 267 bp, and ITS 2 / 28 S = 1112 bp). Te Bayesian inference analysis was conducted with MRBAYES (v. 3.2.7; Ronquist et al. 2012), via the CIPRES Science Gateway (Miller et al. 2015). It consisted of two concurrent runs, each with four Markov chains of 100 million generations (the first 20 % discarded as ‘ burn-in’), the default priors, nst = 6, rates = invgamma, temperature parameter = 0.1, sampling every 1000 generations, and with substitution model parameters unlinked across the markers (COI, H 3, and ITS / 28 S). Markov chain Monte Carlo convergence was assessed by examining the SD of split frequencies (~ 0.001) and the potential scale reduction factor (PSRF ~ 1.0), in addition to the trace plots (Ronquist et al. 2009). Occurrence records Te distribution of D. magus was reviewed by combining data from the aforementioned natural history collections, field observations, published literature, and the iNaturalist citizen science platform (htps: // www. inaturalist. org /), which contains geolocated records accompanied by photographs of living animals or empty shells. All specimens had their identifications reviewed, and misidentified specimens were excluded from the dataset. Likewise, all iNaturalist records were checked by us, following the same verification protocol applied by Rosa et al. (2022). Data on the reviewed iNaturalist records are available as Supporting Information File S 1. In the text, iNaturalist records are reported using their observation number in the platform. To visualize the record on iNaturalist, simply add that number to the end of the command ‘ htps: // www. inaturalist. org / observations / ’, which will become a functioning URL. Field observations Field observations of live specimens of D. magus were carried out to gather data on life appearance, ecology, and natural history. Observations were made in two localities in northern São Paulo state: (i) the University of São Paulo (USP) campus in the municipality of Ribeirão Preto; and (ii) a forested area surrounding the reservoir of the Caconde hydroelectric power plant near the municipality of Caconde. Te localities were chosen owing to both being relatively accessible to the authors and both having previous records of D. magus in the form of specimens in the CMRP and MZSP collections. Fieldwork was conducted mostly at night (~ 19.00 – 00.00 h) during the rainy season (October – February) in 2023 and 2024, but additional searches were carried out at other times and periods when possible. Te specimens found were photographed, and notes on their behaviour were made. Some of the photographs were uploaded to iNaturalist by the authors and other people who helped with the fieldwork. Additional natural history information was also gathered from iNaturalist observations, whenever possible. Te resulting data were compared with the few published accounts on the ecology and natural history of other Drymaeus species (e. g. Breure 1979).	en	Rosa, Rafael M., Salvador, Rodrigo B., Cavallari, Daniel C. (2025): Te disappearing act of the magician tree snail: anatomy, distribution, and phylogenetic relationships of Drymaeus magus (Gastropoda: Bulimulidae), a long-lost species hidden in plain sight. Zoological Journal of the Linnean Society 203, DOI: 10.1093/zoolinnean/zlaf017
E82F87CABE5EFFDB0E97F702FA9AB1EE.taxon	description	Te syntypes of the species consist of two shells. One syntype (ZSM 20020093; Fig. 3 A) perfectly matches the figure from the original description of this species (Spix and Wagner 1827: pl. 7, fig. 1). Terefore, that specimen is here designated as the lectotype of Bulimus magus Wagner, 1827. Te second syntype (ZSM 20240467) belongs to Drymaeus papyraceus (Mawe, 1823). Type locality ‘ Brasilien’ [Brazil], designated herein according to the original label of the lectotype. Te localities reported by Spix and Wagner (1827) are considered erroneous (see Discussion below). Suggested vernacular name Magician tree snail (or magician treesnail), which represents a translation of its Latin epithet. In Portuguese, the translated vernacular name would be ‘ caracol-mago’. Diagnosis Shell small to medium-sized (height = 15 – 25 mm), broad, spire approximately one-third of shell height; colour beige to light brown, with large dark brown sinuous axial patches, occasionally crossed or interrupted by up to three blurred spiral bands; apex, peristome, and umbilicus ofen reddish brown to pinkish red; colour of periumbilical region occasionally distinct from the remainder of the shell and bordered by a continuous dark brown spiral line; umbilicus very narrow. Head dark grey, transitioning sharply at foot margin to pale grey / beige; tentacles coloured similar to head at their base, transitioning gradually to reddish brown distally, with a yellow tip. Albumen gland distinctly very large; bursa copulatrix duct narrow distally; penis small. Redescription Shell: Shell presenting one of two possible morphotypes (Fig. 3). Adult shell either medium-sized (Fig. 3 A – F; height = 22 – 25 mm) or small (Fig. 3 G – J; height = 15 – 17 mm) for the genus, with six convex whorls and typical bulimoid outline; width approximately two-thirds of shell height; spire conical, height approximately one-third of shell height; spire angle ~ 55 °. Ground colour beige to light brown, with large dark brown sinuous axial patches (Fig. 3 A – D, G – I), which are either mostly continuous (Fig. 3 A – D) or crossed or interrupted by up to three blurred spiral bands (Fig. 3 G – I); apex, peristome, and region surrounding umbilicus from cream (Fig. 3 A) to reddish brown to pinkish red (Fig. 3 F, J), with the pinkish red either contiguous to remaining shell areas (Fig. 3 F) or bordered and separated from the remainder of the shell by a continuous dark brown spiral line of variable width (Fig. 3 H – J). Protoconch (Fig. 3 K) with approximately two whorls; sculpture consisting of intercrossed axial and spiral lines of similar strength and width, forming a delicate reticulate patern; transition noticeable as a sudden change in sculpture. Teleoconch sculptured by axial growth lines, fine sinuous spiral striae (Fig. 3 B – D), and ofen by coarse axial striae (Fig. 3 G, H) with variable intensity; whorl profile convex; suture shallow but well marked. Aperture (Fig. 3 A – C, G) large, oval, prosocline, height approximately half of shell height, width approximately three-quarters of shell width; peristome lighter coloured from cream to white, slightly reflected, more strongly so at the columellar region, forming a thin fold that partly covers the umbilicus (Fig. 3 B), ofen separated from remainder of shell by a reddish axial band (Fig. 3 C). Umbilicus very narrow (Fig. 3 F, J). Head-foot (Figs 3 I, J, 4 A – G, I – K, N, 5 A, B): Typical in shape; head dark grey, uniform colour, transitioning sharply at foot margin; foot pale grey to beige, uniform; tentacles coloured similar to head at their base, transitioning gradually to reddish brown distally, and yellow at the tip. Mantle organs (Fig. 5 A, B, 6 E): Mantle edge thick, unpigmented. Pneumostome (Fig. 5 B: pn) protected by a right ventral flap. Dorsal fold roughly twice as large as ventral flap, ~ 1.5 times longer. Lung (Fig. 6 E: pu) twice as long as wide, length roughly half a whorl. Pulmonary vein (Fig. 6 A – D: cv) large, located dorsally on pallial cavity. Pulmonary vessels conspicuous along right side of pulmonary vein (Fig. 6 E), bearing clusters of transverse, roughly perpendicular ramifications; vessels less conspicuous on lef side. Remaining lung areas nearly smooth, with sparse inconspicuous vessels. Visceral mass (Fig. 5): Approximately 3.5 whorls in length. Digestive gland (Fig. 7 A – F: dg) bilobed; anterior lobe (da) flattened, posterior to pallial cavity, continuous to kidney; posterior lobe (dg) with ~ 2.5 whorls. Stomach encased by digestive gland, located ~ 1.5 whorls from visceral mass apex. Digestive tract surrounding anterior lobe of digestive gland. Gonad (Fig. 9 A, D – G: go) multi-lobed, encased between posterior lobe of digestive gland and columella (Fig. 5). Circulatory and excretory systems (Fig. 6): Pericardium twice as long as wide, located ventrally and adjacent to posterior end of pallial cavity. Auricle (Fig. 6 A – D: au) located anteriorly, contiguous to the pulmonary vein (Fig. 6 A – E: cv), approximately twice as large as the ventricle (Fig. 6 A – D: ve). Kidney (Fig. 6 A – D: ki) simple, solid, roughly triangular, dorsoventrally flattened, approximately twice as large as pericardium, width approximately two-thirds of length. Nephropore (Fig. 6 F: ne) small, slit-like, located near transition from auricle to pulmonary vein. Ventricle (Fig. 6 A – D: ve) roughly triangular, contiguous to anterior aorta (Fig. 6 A – D: aa). Digestive system (Figs 7, 8): Oral tube wide, muscular. Jaw (Fig. 7 A – I: jw) typical, consisting of a triangular middle plate and 16 imbricated lateral plates of similar width; plate length up to approximately six times width, gradually decreasing distally; colour yellowish brown, translucent. Buccal mass (Fig. 7 A – F, H, I: bm) stubby, roughly rounded, narrower anteriorly, with two ventrolateral expansions congruent with odontophore cartilages (Fig. 7 H, I: oc). Dorsal surface of oral cavity bearing a conspicuous pair of dorsal folds (Fig. 7 J: df). Odontophore cartilages (Fig. 7 H, I: oc) flatened, roughly triangular, each approximately twice as long as wide, fused ventro-anteriorly along approximately one-fifh of ventromedial margin. Radular sac short, slightly protruding posteriorly beyond odontophore cartilages, with contiguous nucleus (Fig. 7 H, I: rn). Radula (Fig. 8) covering odontophore, with multiple rows containing a distinct rachidian tooth and 63 – 72 pairs of lateral teeth (Fig. 8 A – C); teeth closely spaced, with a roughly rectangular base. Rachidian tooth (Fig. 8 D, E) reduced, approximately half as wide and approximately three-quarters as long as lateral teeth, flatened, roughly triangular, tricuspidate; central cusp five times longer and four times wider than basal cusps, with blunt tip; basal cusps symmetrical, much smaller, triangular, with sharp tip. Lateral teeth (Fig. 8 D – H) markedly distinct from rachidian, twice as wide and 1.25 times longer, asymmetrical, slightly arched laterally towards the radular margin, tricuspidate; base roughly rectangular, becoming slightly narrower and longer in teeth closer to the radular margin; proportions of cusps varying gradually towards the radular margin; inner basal cusp triangular, with a sharp tip, approximately half as long and wide as remaining cusps initially (Fig. 8 D), becoming similar in length / width and shape to outer basal cusp (Fig. 8 G) and more detached from central cusp towards the radular margin (Fig. 8 H); central cusp roughly rectangular, ~ 1.5 – 2 times wider and longer than remaining cusps, with a rounded blunt tip; outer basal cusp triangular with a sharp tip, approximately half as long and nearly as wide as central cusp initially, eventually becoming bifid (Fig. 8 J, L) or even trifid (Fig. 8 J) near the 30 th lateral teeth and onwards, with sharper tips; occasional atypical bicuspidate lateral teeth can be observed in the same position in all rows (Fig. 8 G). Marginal teeth overall smaller than lateral teeth (approximately three-quarters as wide and long), with a proportionally narrower and longer base, tricuspidate (Fig. 8 K); cusps proportionally shorter and blunter than that of adjacent lateral teeth (Fig. 8 I, K); inner basal cusp triangular, with a sharp tip, approximately three-quarters as long and wide as remaining cusps; central cusp triangular, with a sharp tip, approximately one-quarter longer and wider than remaining cusps; outer lateral cusp bifid, approximately three-quarters as long and one-quarter wider than central cusp. Salivary ducts (Fig. 7 A – F, H, I: sd) running dorsally along both sides of anterior oesophagus (Fig. 7 A – F, H, I: es), inserting into buccal mass near transition to oesophagus. Oesophagus (Fig. 7 A – F, H, I: es) approximately four times longer than buccal mass, with numerous dorsal folds. Stomach (Fig. 7 C – F: st) curved, encased by digestive gland, located ~ 1.5 whorls from visceral mass apex; gastric walls thin, smooth. Duct to digestive gland (Fig. 7 K: dd) branched, located at transition to intestine. Intestine (Fig. 7 A – F: in) long, smooth, with a sigmoid loop across the anterior region of the digestive gland. Rectum (Figs 6 E, 7 A – F, L: rt) and anus (Fig. 7 A – F, L: an) located on the right posterior side of pneumostome. Anus (Fig. 7 A – F, L: an) sessile, slit-like, located inside pneumostome, inner surface with seven longitudinal simple folds (Fig. 7 L: an). Reproductive system (Fig. 9): Gonad position described above (visceral mass), composed of four lobes (Fig. 9 A, D – G: go). Hermaphroditic duct (Fig. 9 A, D – G: hd) narrow and thoroughly entangled, width relatively uniform, insertion on lef side of seminal receptacle. Seminal receptacle (Fig. 9 E: sr) small, sac-like. Fertilization complex simple, located at anterior end of seminal receptacle, completely immersed in albumen gland, insertion on posterior end of spermoviduct. Albumen gland (Fig. 9 A, D – G: ag) solid, elliptical, coiled, half a whorl long, four times larger than gonad; albumen gland duct subterminal, connected to distal end of spermoviduct; albumen chamber (Fig. 9 A, D – G: ac) length approximately one-sixth of spermoviduct length, volume approximately one-fifh of spermoviduct volume. Spermoviduct approximately one and a quarter whorls long, width inconstant along its length, surface irregular, intensely folded. Prostate (Fig. 9 A, D – G: pt) surface approximately one-third of spermoviduct surface, volume approximately one-quarter of spermoviduct volume. Uterus (Fig. 9 A, D – G: ut) volume approximately three-quarters of spermoviduct volume, external wall thick. Free oviduct (Fig. 9 A, D – G: fo) length ~ 1 / 20 th of spermoviduct length. Vagina (Fig. 9 A, B, D – G: vg) length ~ 1 / 10 th of spermoviduct length, inner surface with five longitudinal folds (Fig. 9 B: vg). Bursa copulatrix + duct (Fig. 9 A, D – G: bc, bd) as long as spermoviduct; bursa copulatrix duct as wide as spermoviduct proximally, twice as wide at mid-section, gradually much narrower distally (Fig. 9 A, D – G: bd); bursa copulatrix globose, laterally compressed, encased between pericardium and adjacent intestinal loop (Fig. 9 A, D – G: bc). Penis (Fig. 9 A, B, D – G: pe) length approximately half of spermoviduct length; penis muscle (Fig. 9 F: pm) very short (length ~ 1 / 20 th of penis length), with terminal insertion; epiphallus (Fig. 9 A, D – G: eh) distinguishable from remaining penis through more irregular inner surface, length ~ 1 / 10 th of penis length; inner penial surface without subchambers, posterior region bearing five narrow longitudinal folds, middle region smooth, anterior region bearing five narrow longitudinal folds (Fig. 9 B: pe); penis sheath (Fig. 9 A, D – G: ps) covering approximately the anterior quarter of the penis. Genital pore (Fig. 9 A, D – G: fp) round, simple. Central nervous system (Fig. 10): Pair of cerebral ganglia (Fig. 10: ce) located dorsally above oesophagus near transition from buccal mass; widely fused, cerebral commissure externally indistinguishable; nerves originating from anterolateral region of cerebral ganglia. Cerebral and pedal ganglia connected by parallel connectives surrounding oesophagus. Pair of pedal ganglia (Fig. 10: pp) located ventrally, more posterior than cerebral ganglia, fused as a single mass, slightly larger than cerebral ganglia. Distribution WidespreadinsoutheasternBrazil, withrecordsfromthestatesof Minas Gerais, São Paulo, Rio de Janeiro and Paraná (Fig. 2). In our review, we identified 49 occurrence records for Drymaeus magus: 11 from the investigated collections (3 from CMRP and 8 from MZSP), 36 from iNaturalist (Supporting Information File S 1), and 2 from previous studies (Oliveira et al. 1981). Records with uncertain identification or imprecise locality data, including the lectotype, were excluded. Most records are from São Paulo (35) and southern Minas Gerais (13). Tree potentially non-native records from the states of Rondônia (northern Brazil; iNaturalist obs. 108923731) and Mato Grosso do Sul (midwestern Brazil; iNaturalist obs. 120650892 and 120650890) were also found (see Discussion below). Additionally, a few published records from the state of Santa Catarina (e. g. Agudo-Padrón 2008; 2009, 2014, 2018, 2022) lack photographic evidence or voucher specimens and are therefore excluded from consideration. Habitat and ecology Dwells on tree trunks and leaves, mostly in seasonal semideciduous forests of the inland Atlantic Forest and Cerrado. Also recorded in anthropogenic habitats, including urban areas and coffee crops (Rezende 1967). Nocturnal and more active during the rainy season, like most land snails (Salvador and Tomotani 2024) and consistent with previous observations of Drymaeus (Rezende 1975, Breure 1979). Material examined BRZIL. No specific data: ZSM 20020093, one shell, lectotype. Minas Gerais: Arceburgo, Sítio Areias de Minas, 9 June 2023, MZSP 164980, one specimen. São Paulo: Pedregulhos, Parque Estadual das Furnas do Bom Jesus, 20 ° 15 ′ 22.7 ″ S, 47 ° 27 ′ 36.4 ″ W, 13 April 2024, CMRP 1211, three specimens; Ribeirão Preto, University of São Paulo campus, 21 ° 09 ′ 56.6 ″ S, 47 ° 51 ′ 49.1 ″ W, 12 January 2023, CMRP 1049, one specimen; 24 January 2023, CMRP 1056, one specimen; 11 October 2023, CMRP 1118, two specimens; Cava do Bosque, 21 ° 10 ′ 23.9 ″ S, 47 ° 47 ′ 58.8 ″ W, 1 January 1981, MZSP 083293, two shells; 1 April 1980, MZSP 132081, two shells; Caconde, forested area surrounding the Caconde hydroelectric power plant reservoir, 21 ° 36 ′ 11.6 ″ S, 46 ° 37 ′ 29.0 ″ W, 28 January 2023, CMRP 1059, one specimen; 7 March 2023, CMRP 1087, one specimen; 8 April 2023, CMRP 1090, one specimen; 13 January 2024, CMRP 1169, two shells; Serra Negra, 22 ° 37 ′ 08 ″ S, 46 ° 42 ′ 15 ″ W, 9 September 2023, MZSP 166927, one specimen; Porto Feliz, 3 January 1936, MZSP 016772, nine shells; Praia Grande, 1 January 1994, MZSP 083926, two shells.	en	Rosa, Rafael M., Salvador, Rodrigo B., Cavallari, Daniel C. (2025): Te disappearing act of the magician tree snail: anatomy, distribution, and phylogenetic relationships of Drymaeus magus (Gastropoda: Bulimulidae), a long-lost species hidden in plain sight. Zoological Journal of the Linnean Society 203, DOI: 10.1093/zoolinnean/zlaf017
